Abstract
As life expectancy increases worldwide, age-related neurodegenerative diseases will increase in parallel. The lack of effective treatment strategies may soon lead to an unprecedented health, social and economic crisis. Any attempt to halt the progression of these diseases requires a thorough knowledge of the pathophysiological mechanisms involved to facilitate the identification of new targets and the application of innovative therapeutic strategies. The metzincin superfamily of metalloproteinases includes matrix metalloproteinases (MMP), a disintegrin and metalloproteinase (ADAM) and ADAM with thrombospondin motifs (ADAMTS). These multigenic and multifunctional proteinase families regulate the functions of an increasing number of signalling and scaffolding molecules involved in neuroinflammation, blood–brain barrier disruption, protein misfolding, synaptic dysfunction or neuronal death. Metalloproteinases and their physiological inhibitors, the tissue inhibitors of metalloproteinases (TIMPs), are therefore, at the crossroads of molecular and cellular mechanisms that support neurodegenerative processes, and emerge as potential new therapeutic targets. We provide an overview of current knowledge on the role and regulation of metalloproteinases and TIMPs in four major neurodegenerative diseases: Alzheimer’s disease, Parkinson’s disease, amyotrophic lateral sclerosis and Huntington’s disease.
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Introduction
Humans have not evolved to last long in nature. As the forces of natural selection disappear with the improvement of life and health conditions, average life expectancy has exceeded 80 years in many countries of the world. The concomitant consequence is the soaring of aging-related neurodegenerative disorders that cannot be cured or significantly slowed down, thereby affecting millions of patients and even more caregivers. These disorders generally start with mild symptoms that alter motor, behavioural and cognitive functions. The gradual loss of large amounts of neurons inevitably leads to a worsening of these symptoms, which often end up with a loss of global autonomy before the patient’s death. Neurodegenerative diseases are associated with genetic and environmental stimuli that act in synergy to elicit disease-specific dysfunctions, but also share fundamental commonalities: free radicals generation, mitochondrial dysfunction, immunosenescence, protein misfolding or inflammation. The confluence of these pathogenic driving forces makes it difficult to identify a single cause that could be more easily targeted. It is of the utmost importance to elucidate the underlying mechanisms of the pathology to clearly identify molecular targets and help design effective therapeutic strategies. Among the biofactors that can contribute to neurodegenerative processes, matrix metalloproteinases (MMPs) are of particular interest because: (1) MMPs are expressed by all types of central nervous system (CNS) cells; (2) MMPs expression is modulated by potentially neurotoxic proteins, which can in turn undergo cleavage and functional regulation by these same MMPs; (3) MMPs modulate chronic neuroinflammation through cleavage of inflammatory mediators (i.e., cytokines and chemokines) and tight junction proteins that ensure blood–brain barrier (BBB) impermeability; (4) MMPs control the processing of extracellular matrix (ECM) and transmembrane proteins involved in cell–cell interactions; (5) MMPs can initiate or be part of proteolytic cascades that amplify cellular responses in a web of interactions between numerous enzymes and substrates.
In this review, we will discuss the most relevant knowledge on MMPs and their physiological inhibitors, the tissue inhibitors of metalloproteinases (TIMPs), in four neurodegenerative diseases that strike in mid–late-life: Alzheimer’s disease (AD), Parkinson’s disease (PD), amyotrophic lateral sclerosis (ALS) and Huntington’s disease (HD). We will also discuss to a lesser extent the contribution of two other metalloproteinase subfamilies, which, like MMPs, belong to the superfamily of metzincins: a disintegrin and metalloproteinase (ADAM) and ADAMs with thrombospondin motifs (ADAMTS). While ADAMs are membrane-anchored enzymes, chiefly considered as sheddases of membrane proteins, ADAMTS are mostly extracellular matrix (ECM)-degrading enzymes. ADAMs and ADAMTS in the nervous system are extensively discussed in this CMLS special issue by Hsia and colleagues [1] and elsewhere [2].
Metalloproteinases and natural tissue inhibitors of metalloproteinases
Matrix metalloproteinases
Twenty-four proteinases constitute the MMP family in humans. According to their structure and substrate specificity, this multigenic family have been traditionally classified into five categories: gelatinases (-2 and -9), stromelysins (MMP-3 and -10), collagenases (MMP-1, -8 and -13), membrane-type MMPs (MT-MMPs, MMP-14, -15, -16, -17, -24 and -25) and the other MMPs, e.g., MMP-7, MMP-12 or MMP-28 (see for reviews [2,3,4]). Widely expressed in all human cells, MMPs have significant structural homology and this is one of the main reasons that hinder the development of specific inhibitors against each of them. All MMPs possess a 17–29 amino acid hydrophobic signal peptide that targets the proteinase to the secretory pathway, followed by a pro-domain sequence of 77–87 amino acids that interacts with a conserved cysteine residue and the Zn2+ cation of the catalytic site, thereby maintaining the enzyme under a zymogen inactive state. The catalytic domain of ~ 170 amino acids, harbours a Zn2+ binding consensus sequence HExxHxxGxxH with three histidine residues that confer stability to Zn2+. Redox-mediated break-up of the interaction between the cysteine and the metal cation as well as propeptide removal by autocatalysis or by other proteinases, triggers the conversion of inactive pro-MMPs into active MMPs by a mechanism known as “cysteine switch”. Downstream of the catalytic site, a short hinge region followed by the hemopexin domain (~ 200 amino acids) exhibits a relatively variable amino acid sequence, which is crucial for proteinase-substrate specificity. Of note, MMP-7, MMP-23 and MMP-26 lack the hemopexin domain. In addition to this multidomain common structure, the six members of the MT-MMP subfamily contain membrane anchoring domains; a glycosylphosphatidylinositol in the case of MMP-17 (MT4-MMP) and MMP-25 (MT6-MMP) or a transmembrane domain with a short intracytoplasmic moiety in the case of MMP-14 (MT1-MMP), MMP-15 (MT2-MMP), MMP-16 (MT3-MMP) and MMP-24 (MT5-MMP). Moreover, MT-MMPs, MMP-11, MMP-23 and MMP-28 contain a specific di-basic sequence at the end of the pro-domain, which is recognized by the intracellular Ca2+-dependent serine proteinase furin, leading to activation of these enzymes in the trans-Golgi network [4].
MMPs have been usually considered as ECM-degrading enzymes. This view is now changing with the growing number of non-matrix substrates identified among signalling molecules, trophic factors, receptors, cell adhesion molecules, and even nuclear proteins [5,6,7]. It must be emphasized that MMPs are more and more involved in the modulation of neuroinflammatory processes common to many nervous system pathologies through the regulation of: (1) ECM proteolysis [8]; (2) cell proliferation, differentiation and migration [9,10,11]; (3) activation and inactivation of inflammatory mediators [12]; (4) BBB permeability [13]. If we add that proteolytic-independent effects of MMPs are beginning to be unveiled [14], we can conclude that MMPs represent a paradigm of extraordinary and fascinating functional diversity.
Tissue inhibitors of metalloproteinases
TIMPs are pleiotropic secreted proteins, mostly known for their reversible MMP inhibitory activities. The four TIMPs (TIMP-1 to TIMP-4) share 40% of sequence homology and a backbone with twelve conserved cysteine residues and six disulfide bonds that are essential for their biological activities. Besides the signal peptide, TIMPs structure comprises a N-terminal inhibitory domain of MMPs and a C-terminal domain of interaction. TIMP-1, -2 and -4 are found as soluble or cell surface-associated proteins, whereas TIMP-3 preferentially binds to ECM proteins. In general, TIMPs bind all MMPs and some ADAMs, but only TIMP-3 appears to have inhibitory activity against ADAMTS [15]. The N-terminal domain of TIMPs is sufficient to inhibit MMPs, but in the case of ADAM10, TIMP-1 and TIMP-3 also require the interaction of their C-terminal domain with the proteinase. ADAM10 is not inhibited by TIMP-2 and -4 [16]. The binding affinities between TIMPs and MMPs or their modes of interaction differ significantly. For instance, TIMP-1 inhibits soluble MMPs and ADAM10/17, but it is a very poor inhibitor of MT-MMPs. Also, TIMP-1 is able to specifically bind the hemopexin domain of pro-MMP-9, although the biological function of this complex is unknown [17]. TIMP-2 inhibits both soluble and membrane-bound MMPs. In addition, TIMP-2 specifically binds to the hemopexin domain of pro-MMP-2, paradoxically leading to the activation of the enzyme on the plasma membrane; indeed, the N-terminal domain of TIMP-2 interacts with MT1-MMP, whereas the C-terminal domain binds to the hemopexin domain of pro-MMP-2, thus fixing the pro-MMP-2 on the membrane and allowing its activation by cleavage of the pro-peptide by an adjacent MT1-MMP [18]. TIMP-3 inhibits MMPs, ADAMs and ADAMTS. TIMP-4 has the same inhibitory profile as TIMP-2. All TIMPs are ubiquitously distributed, with the exception of TIMP-4, which is predominantly expressed in heart, ovary and brain [19].
Timp-1, Timp-3 and Timp-4 genes are nested in introns of genes coding for synaptic proteins synapsins and Timp-2 is close to the synapsin IV gene [20,21,22]. The intriguing genetic link between TIMPs and synapsins likely underlines functional relations of these proteins in the nervous system that need to be explored, as many neuropathological conditions show significant alterations of their expression.
Alzheimer’s disease
Alzheimer’s disease (AD) is the most common type of neurodegenerative disorder for which we still lack efficient curing, slowing or preventing treatments. Prototypic symptoms of AD start with short-term mild memory deficits that deteriorate with time, progressively leading to severe memory loss, changes in mood, anxiety, depression, agitation, spatial disorientation, motor impairment, and finally dementia. AD affects 45 million people currently worldwide and this figure is expected to rise to 131 million in 2050 unless efficient treatments are found in the meantime [23]. Only a handful of available drugs can transiently and moderately limit clinical symptoms in the early stages of the disease (https://www.alz.org/alzheimers-dementia/research_progress/treatment-horizon). The difficulty in finding effective treatments for AD is due to a multitude of factors, including:
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The multifactorial etiology of AD. Familial forms of the disease represent ~ 1% of cases and are caused by mutations in 3 genes: amyloid precursor protein (App), and presenilins 1 (Psen1) and 2 (Psen2). The overwhelming majority of patients suffer from sporadic forms of the disease of unknown etiology, where genetic and environmental risk factors likely synergize with age to prepare a fertile ground for the development of the disease.
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The difficulty of successfully reproducing valuable preclinical data in human clinical trials.
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Comorbidity with other disorders/injuries may add confounding factors from an etiological standpoint.
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A relatively poor knowledge of the pathophysiological mechanisms involved. To date, most research efforts have focused on studying two pathological characteristics of the disease: the accumulation of the amyloid beta peptide (Aβ) resulting from the proteolytic processing of APP, and the hyperphosphorylation of the tau protein (p-tau). Unfortunately, the results of clinical trials targeting Aβ or p-tau have been well below expectations [24,25,26], prompting researchers to discover alternative targets.
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Clinical trials are conducted on older people after diagnosis, but AD starts 10 or 15 years earlier, meaning that treatments against relevant targets (e.g., Aβ, p-tau) occur too late, when the aging brain has already lost much of its healing ability and resilience.
Despite the diversity of potentially pathogenic mechanisms in AD, metalloproteinases have been mainly involved in the metabolism of APP and Aβ. It is in this context that we will address the following sections.
Main pathogenic pathways linked to APP processing and amyloidogenesis
Almost 30 years after its publication, the amyloid hypothesis of AD remains a valuable tool to study the underlying pathophysiological mechanisms, despite the failure of clinical trials based on its principles. The amyloid hypothesis essentially asserts that excessive accumulation of Aβ is a major pathogenic determinant (see for an updated review [27]). Aβ results from sequential cleavage of APP by two canonical secretases; β-secretase (beta-site APP cleaving enzyme-1, BACE-1) generates a transmembrane fragment of 99 amino acids (C99), which is then cleaved by the γ-secretase complex, thus releasing 4 kDa Aβ monomers, mainly 40 (Aβ40) and 42 (Aβ42) amino acids. Aβ42 aggregates more easily than Aβ40 and it is, therefore, more toxic. Monomers can assemble into oligomers, protofibrils and fibrils, which will eventually give rise to amyloid plaques. Although the latter are a hallmark of AD and provide bona fide post mortem diagnostic, small size oligomers (e.g., dimers, trimers) are increasingly seen as the most toxic forms of Aβ [28]. APP cleavage by β- and γ-secretases occurs following APP endocytosis into the endosomes or during APP targeting to the cell surface through the trans-Golgi network, thereby highlighting the importance of APP cellular trafficking in amyloidogenesis (reviewed in [29]). Aβ accumulation results from a balance between its formation and its degradation/clearance. Several metalloproteinases, including insulin degrading enzyme (IDE), angiotensin converting enzyme, endothelin converting enzyme and neprilysin, play a prime role in Aβ degradation (reviewed in [30]). Moreover, some MMPs (i.e., MMP-2, -3, -9 and MT1-MMP) have also been reported to display Aβ-degrading activity (see [3]). Complementary to proteolytic degradation, the neurovascular hypothesis of AD suggests that tuning down Aβ levels in the brain parenchyma can also be achieved by scavenging systems mostly operating in the BBB microenvironment. Several reports indicate that one of these systems is the apolipoprotein E (APOE) receptor, low-density lipoprotein receptor (LDLR). Thus, overexpression of LDLR in the mouse brain limits amyloid plaque formation and enhances Aβ clearance from brain to blood [31, 32], as well as Aβ uptake and degradation by astrocytes through a mechanism where Aβ directly binds to LDLR, even in the absence of APOE [33]. The low-density lipoprotein receptor-related protein 1 (LRP-1), mainly expressed by glial and endothelial cells, also contributes to Aβ clearance. This is confirmed by experiments in which the decrease/abrogation of LRP-1 expression using antisense oligonucleotides [34] or LRP-1-conditional knockout [35], interferes with Aβ clearance via the BBB, leading to its accumulation in the brain and the consequent learning deficits. Selective knockdown of LRP-1 in astrocytes also reduces Aβ uptake and degradation, which correlates with a downregulation of major Aβ-degrading enzymes MMP-2, MMP-9 and IDE [36]. Unlike, LDLR and LRP-1, the receptor for advanced glycation end products (RAGE) promotes Aβ influx from blood-to-brain (reviewed in [37]). Accordingly, silencing or eliminating RAGE has been shown to preserve BBB integrity in vitro [38] and reduce brain Aβ levels in transgenic AD mice by decreasing β- and γ-secretase activities [39].
It is clear that neurotoxicity derived from APP cleavage can no longer be considered exclusively on the basis of Aβ accumulation. Other APP metabolites generated by different proteinases (e.g., MT-MMPs, δ-secretase) also contribute to Alzheimer’s pathology (reviewed in [40]), paving the way for an assessment of APP breakdown products as components of pathogenic pathways, and therefore, as potential new therapeutic targets.
Non-pathogenic pathways linked to APP processing
In physiological conditions, APP is mainly processed at the plasma membrane level by α-secretases of the ADAM family. This subfamily of metzincins present structural and functional similarities with MMPs (see for review [2]). ADAM10 is the main physiological/constitutive α-secretase [41, 42], while ADAM17 has been identified as responsible of the regulated α-secretase activity [43]. α-secretase cleavage in the middle of the Aβ sequence prevents its formation and concomitantly generates a soluble N-terminal APP fragment (sAPPα) with neurotrophic and neuroprotective properties [44, 45]. Aβ oligomers stimulate transient increase of sAPPα levels and α-secretase activity in cultured cortical neurons, which could be interpreted as a cell self-defence mechanism [46]. While there is little doubt about the neurotoxicity of Aβ accumulation, the physiological roles of the peptide are still poorly understood. Several pieces of evidence converge to show that Aβ is part of the innate immunity arsenal to fight against bacterial, fungal and viral pathogens in the brain [47,48,49,50]. Moreover, physiological Aβ is involved in maintaining basal neurotransmitter release and synaptic activity [51]. It has been shown that picomolar concentrations of Aβ are sufficient to stimulate learning and memory in healthy rodents as well as long-term potentiation (LTP)—a form of synaptic plasticity considered to be a cellular substrate for learning—through the activation of nicotinic receptors [52,53,54]. N-terminal fragments of Aβ found in the cerebrospinal fluid (CSF) of healthy and AD individuals appear to be determinant for these physiological effects, with the YEVHHQ motif located before the α-cleaving site in the Aβ sequence playing a prominent role [55]. It has also been shown that cGMP nucleotide stimulates the release of Aβ by facilitating the approximation in endolysosomal compartments between APP and BACE-1, the main β-secretase. The blockade of Aβ with antibodies in these conditions interferes with cGMP-induced enhancement of LTP and memory [56]. Taken together, these data indicate that the proteolytic regulation of Aβ transcends the idea of its neurotoxicity and raises the question of the potential clinical consequences of lowering Aβ levels below a physiological threshold.
MMPs are mainly considered as Aβ-degrading enzymes, but not only
MMPs with Aβ-degrading activity might be beneficial
Pioneer work in the 90’s linked for the first time AD with MMPs. Tökés and collaborators found upregulated expression levels of inactive pro-MMP-9 in hippocampal neurons of post mortem AD patients. They also demonstrated by mass spectrometry the ability of active MMP-9 to cleave Aβ40 on 3 sites of the membrane-spanning domain, but also at Lys16–Leu17, the so-called α-cleavage site [57]. In the first case, MMP-9 could prevent the formation of the neurotoxic β-sheet. In the second, MMP-9 could act as an α-secretase. Consistent with this idea, MMP-9 overexpressing mice exhibit increased levels of sAPPα associated with enhanced LTP and enhanced learning and memory capabilities [58]. Other authors have corroborated in vitro the ability of MMP-9 to cleave soluble Aβ at the α-site, but the enzyme seems to be more efficient at cleaving in the C-terminus with decreasing processing efficiency towards the N-terminus to generate fragments ending at positions 34, 33, 30, 23, 20 and 16 [59, 60]. In addition, MMP-9 exhibits a rather uncommon feature among Aβ-degrading enzymes because it can cleave preformed Aβ fibrils and compact amyloid plaques, as shown on brain slices from APP/PS1 transgenic mice [59]. This further adds to the possibility that promoting MMP-9 activity may hold therapeutic potential. However, this postulate is subject to caution as it cannot be excluded that proteolytic degradation of plaques could release toxic Aβ assemblages and other neurotoxins contained in their mesh. MMP-2 presents Aβ-degrading profiles roughly similar to those reported for MMP-9, although MMP-2 appears to be more efficient in cleaving Aβ42 [60].
Reactive astrocytes produce MMP-2 and MMP-9 and are systematically associated with Aβ deposits in transgenic mouse models of AD and in post mortem AD brains. In support of a functional link between both observations, the incubation of recombinant Aβ in conditioned media from cultured mouse astrocytes yields breakdown Aβ C-terminal fragments, which can be prevented by selective chemical inhibitors of MMP-2 and MMP-9, and by TIMP-1 [61]. Furthermore, MMP-9 and MMP-2 knockout mice exhibit higher levels of Aβ in the brain compared to wild-type mice, thereby supporting that both MMPs degrade Aβ in vivo [61]. In the same vein, a recent study conducted to investigate the impact of physical activity on Alzheimer’s pathology reported that exercise training in Tg2576 transgenic mice significantly decreases the levels of Aβ40 in the cortex, and Aβ42 in the cortex and hippocampus. Of note, decreased Aβ concentration was concomitant with a rise in the levels of five proteins involved in Aβ clearance, among which MMP-9 [62].
In addition to MMP-2 and MMP-9, other MMPs can also degrade Aβ. For instance, metal ligand clioquinol stimulates Aβ degradation in a cell culture system through a mechanism involving the activation of MMP-3 [63]. MMP-7 was recently reported to cleave Aβ40 and Aβ42, a process that is inhibited by binding of Aβ to Cu2+ [64]. Concerning membrane-anchored MMPs, it was shown that COS cells overexpressing MT1-MMP degrade exogenous soluble Aβ40 and Aβ42, and release 6 different Aβ-derived peptides with cleavage sites mostly located around the α-site, between residues 12 and 18 of the Aβ sequence. Moreover, a soluble variant of MT1-MMP lacking the transmembrane domain was able to degrade in situ parenchymal amyloid plaques in brain slices of Tg2576 mice [65], a feature shared only with MMP-9, neprilysin and IDE among metalloproteinases.
MMPs can be pathogenic in connection with inflammatory processes
Although the degrading action of MMPs on Aβ could in principle be considered beneficial, MMPs are multifunctional enzymes, whose roles may depend not only on the cell types that express them, but also on the substrates involved or the pathological and spatio-temporal context (see for review [2]). In the case of BBB disruption, MMPs have a prominent role as they can proteolyse major components of the basement membranes and tight junctions (see for review [66] in this special CMLS issue). The impermeability of BBB, which ensures selective exchanges between the central and peripheral nervous systems, is compromised in AD patients [67] and in transgenic AD mice [68]. This may contribute to inflammatory and neurodegenerative processes, probably with the participation of resident brain immune cells, as suggested by a study using a co-culture of endothelial cells and astrocytes exposed to Aβ42. In this work, astrocyte-induced BBB opening was related to the activation of MMP-9 and the concomitant decrease in claudin-5, a MMP-9 substrate that contributes to the maintenance of functional tight junctions [69]. Another important source of MMP, reactive microglia, may stimulate Aβ accumulation through a MMP-9-dependent mechanism. In this case, microglial MMP-9 generates C-terminal truncated Aβ fragments that interfere with Aβ clearance across the BBB and promote cerebral aggregation of intracranial-injected Aβ42 in wild-type mice. It is noteworthy that the seeding properties of these C-terminal fragments generated by MMP-9 could, therefore, contribute to the development of sporadic forms of the disease [70]. Recently, another report pointed out that disruption of the blood–CSF barrier 6 h after intracerebral injection of Aβ oligomers was linked to conspicuous inflammation, and was prevented by broad spectrum MMP inhibitor GM6001 and by MMP-3 deficiency in mice, suggesting that the control of MMP activity may have therapeutic potential [71]. Likewise, Aβ42 oligomers dowregulated tight junction scaffold proteins in an in vitro BBB model using bEnd.3 endothelial cells. The weakening effects of oligomers on BBB were blocked by either knocking down RAGE, which was induced by Aβ42, or by GM6001 treatment, which inhibited the activity of concomitantly upregulated MMP-2 and MMP-9 [38]. GM6001 and another MMP inhibitor, minocycline, also proved to efficiently reduce inflammation and oxidative stress associated with cerebral amyloid angiopathy (CAA) in AD mice [72].
Blood-derived immune cells (e.g., macrophages, lymphocytes, granulocytes) are suspected to influence AD pathogenesis, but the extent of their contribution to disease and the underlying mechanisms remain elusive (for review [73]). The question arises as to the role of immune cell MMPs, provided that these cells can reach the brain parenchyma by diapedesis or through a disrupted BBB. Evidences in this direction are rather limited at the moment. The monocytic cell line THP-1 treated with Aβ42 releases more MMP-9, along with tumour necrosis factor (TNF-α), interleukin-1beta (IL-1β) and monocyte chemoattractant protein-1 (MCP-1), compared to untreated cells [74]. Purified neutrophils dramatically increase the production of MMP-9 in response to incubation with highly toxic Aβ25-35 [75]. Interestingly, neutrophils infiltrate the brain of AD patients and are also observed in the brain parenchyma of transgenic AD mice in areas with Aβ deposition [76].
Regulation of MMPs in Alzheimer’s animal models and Alzheimer’s patients
The data above convincingly show that Aβ is a substrate of MMPs. In turn, Aβ modulates the expression of MMPs, probably revealing the existence of feedback regulatory mechanisms. Since early work by Gottschall and collaborators showing that Aβ40 could trigger the expression of MMP-2, -3 and -9 in rat mixed neuronal/astrocyte cultures [77], other authors have confirmed these data. Thus, astrocytes surrounding Aβ plaques in transgenic mice brains show increased levels of MMP-2 and -9 [61]. The increase in the mRNA of both gelatinases is already detected at 4 months of age in the hippocampus of 5xFAD mice, and even earlier (2 months) in some astrocytes close to incipient amyloid plaques [78]. On the other hand, MMP-9 immunostaining is upregulated in the soma and dendrites of cortical neurons in 2-month-old 5xFAD mice [78], indicating altogether that the upregulation of MMP-2 and MMP-9 in Aβ enriched areas starts at pre-symptomatic stages of the pathology and persists over the prodromal-like and symptomatic phases, as they have been defined in the 5xFAD model [79]. Whether this conveys beneficial or detrimental effects cannot be systematically anticipated, as functional duality is a characteristic of both gelatinases. These might be beneficial based on their Aβ-degrading properties, but they might also promote BBB disruption and neuroinflammation [80] or exert direct neurotoxicity in the hippocampus, as reported for MMP-9 [81]. Along this line, AβE22Q and AβL34V mutations associated with hemorrhagic symptoms in early onset CAA stimulate the expression and activation of MMP-2 by endothelial cells in a rather selective manner, which is linked to possible BBB dysfunctions [82]. Moreover, Mizoguchi and collaborators demonstrated that intracerebroventricular (ICV) injections of Aβ upregulated MMP-9 expression in neurons and astrocytes and triggered cognitive deficits. Such deficits were efficiently prevented in mice lacking MMP-9 and also after treatment with chemical MMP inhibitors [83]. In addition to the extensive work on gelatinases, other MMPs have also attracted attention in the field. MT1-MMP content was found increased in neurons and amyloid plaques of 5xFAD mice at 6 months of age—during the symptomatic phase of the pathology—this increase affecting both the active and inactive forms of MT1-MMP [78]. Other authors have shown that MT1-MMP expression is mainly associated with reactive microglial cells in 5xFAD mice [84] and reactive astrocytes in Tg-SwDI transgenic AD mice [65]. Morevoer, Aβ42 increases the mRNA levels of MMP-3, -12 and -13 in a microglial cell line and in primary murine microglia in a PI3/Akt dependent manner [85]. The expression of MMP-1, for which no involvement in APP/Aβ metabolism is known, correlates with neuronal degeneration in the rat hippocampus 1 month after ICV injection of Aβ25-35 [86]. Taken together, these data consistently indicate the upregulation of MMP levels after exposure to exogenous Aβ or in the vicinity of Aβ deposits in transgenic mice, with spatial distributions that may vary depending on the cell type or animal model studied.
Studies in humans mostly reflect the upward trend in MMP levels, although some declines have been noted. Human cerebrovascular smooth muscle cells, constituents of the BBB, show increased expression of MMP-2 and its activating enzyme MT1-MMP after Aβ treatment in culture, which eventually results in increased MMP-2 activity and reduced cell viability [87]. Oligomers of Aβ42 positively regulate the expression of several MMPs (i.e., MMP-1, -3, -9, -10, -12 and -19) in microglia isolated from the brain of AD patients post mortem, compared to controls without dementia [88]. ELISA assay revealed MMP-1 levels significantly elevated by more than 50% in different cortical areas of AD patients [89]. Also in post mortem brain tissue, MT5-MMP immunostaining was detected in amyloid plaques [90] and MT1-MMP in microglial cells neighbouring plaques [84], while MMP-3 was found in both amyloid plaques and the interstitium between myelinated axons and astrocytes, in particular, in the parietal cortex [91]. The concentrations of MMP-3 are higher in the CSF of AD patients compared to healthy controls, in contrast with MMP-9 whose levels are lowered in the AD condition [92]. Similarly, Horstmann and collaborators reported an increase in the levels of MMP-3 in CSF and plasma of AD patients, whereas MMP-2 and MMP-9 decrease in plasma [93]. Interestingly, Lorenzl and collaborators found consistent increased MMP-9 levels in plasma in two studies [94, 95] and another study also showed increased MMP-9/TIMP-1 ratios in CSF from AD patients [96]. Noticeably, this study reported increased MMP-3 and MMP-9 levels, as well as increased MMP-3/TIMP-1 ratio, in the CSF of non-demented individuals carrying AD risk markers (e.g., p-tau, Aβ42 or APOE ε4 allele). A negative correlation was found between plasma levels of MMP-3 and the mini-mental state examination score that assesses cognitive performance [97]. Such negative correlation was also confirmed in the plasma of AD patients for MMP-3 activity measured by casein zymography. Consistent with elevated plasma levels of MMP-3, its substrate gelsolin was decreased in these samples, suggesting that the combined use of gelsolin and MMP-3 could, therefore, hold potential as a plasma biomarker in AD [98]. Even accepting that correlative data do not allow for a causal link between MMP levels and disease progression, it has been proposed that proteolysis limits the amount of circulating Aβ that could reach the brain. This idea is based on the ability of MMPs and ADAMs (e.g., MT1-MMP, MMP-9, ADAM10, ADAM12 and ADAM17) to shed RAGE or LRP-1 [99,100,101,102,103], with the consequent release of the soluble truncated receptors that can bind circulating Aβ; it is estimated that 70% of circulating Aβ40 and 90% of Aβ42 is bound to soluble LRP-1 [104].
Most reports associate MMPs to APP metabolism in AD, however, recent work also unveils the possibility of functional links between MMPs and tau protein. For example, increased levels of active MMP-2 colocalize with p-tau in neurofibrillary tangles (NFT) and dystrophic neurites in the entorhinal cortex of AD patients at early disease stages [105]. The same study reports that MMP-2 can cleave recombinant tau in vitro, but fails to cleave tau contained in NFT, leading to the speculation that inactivation of MMP-2 in NFT might prevent the formation of toxic truncated tau assemblies. MMP-9 and MMP-3 are also described as tau-degrading enzymes, but only MMP-9 can generate fragments prone to generate tau oligomers, which are increasingly considered as the most toxic forms of tau [106]. MMP-3 and MMP-10 levels correlate with tau or p-tau levels in the CSF of AD patients, further stressing the potential interest of MMPs as biomarkers of AD pathology [97, 107].
Overall, these data illustrate a wide range of mechanisms by which MMPs can have beneficial or detrimental effects on AD. Particular mention is given in the following section to MT-MMPs, which are relatively new enzymes in the field of AD and open new avenues for a better understanding of pathophysiology.
Alternative processing of APP by MT-MMPs and contribution to Alzheimer’s pathogenesis
Early work from Higashi and Miyazaki showed that MT1-MMP could process APP outside the Aβ sequence [108]. In this study, MT1-MMP activated by concanavalin A in the HT1080 fibrosarcoma cell line was shown to cleave at the Asn579 and Met580 site of APP770 (VLAN579-M580ISEPR), releasing a soluble truncated APP fragment lacking the MMP-2 inhibitory domain (ISYGNDALMP). This decapeptide was previously reported in a study where MMP-2 was originally identified as a putative α-secretase capable of hydrolizing the Lys16-Leu17 bond within the Aβ sequence [109]. The decapeptide, known as APP-derived peptide inhibitor (APP-IP), specifically inhibits MMP-2 with an IC50 value of 30 nM, well below the 2 µM for MT1-MMP and > 10 µM for MMP-3, -7 and -9. The APP-IP sequence, spanning from amino acids 579–601 (βAPP770 numbering), is present in sAPPα and sAPPβ. The authors concluded that MT1-MMP processing of APP would be a way for the tandem MMP-2/MT1-MMP to regulate ECM proteolysis [108]. Additional work on HEK293T cells demonstrated that MT1-, MT3-, and MT5-MMP could release 5 major APP fragments after being co-expressed with APP770 [110]. In this study, the cleavage sites for MT3-MMP were identified by mass spectrometry at positions Ala463-Met464, Asn579-Met580 (VLAN579-M580ISEPR), His622-Ser623 and His685-Gln686. It is noticeable that cleavage at Asn579-Met580 by MT3-MMP matches the MT1-MMP-mediated cleavage previously identified by Higashi and Miyazaki [108]. It is also interesting to note that although His685-Gln686 cleavage is one residue upstream of the α-cleavage site in the Aβ sequence, MT3-MMP does not modify Aβ levels in HEK293T cells [110]. The authors suggested that MT5-MMP could have cleavage profiles similar to those of MT1- and MT3-MMP, which has been confirmed by a recent study showing that MT5-MMP can effectively cleave the shorter neuronal isoform of APP696 at the VLAN504-M505ISEPR, also known as eta (η) site [111]. According to this study, MT5-MMP (η-secretase) generates a CTF fragment of ~ 30 kDa (CTF-30/η-CTF) that can be further cleaved by α-secretase to produce a peptide (Aη-α, for amyloid eta-alpha) of ~ 12 kDa, which impairs LTP in cultured rat neurons. On the contrary, the concerted action of η- and β-secretase generates the Aη-β peptide, surprisingly lacking neurotoxicity. Together, these data challenge the traditional view of α- and β-secretase as beneficial and detrimental enzymes, respectively. Interestingly, η-cleavage by MT5-MMP is strongly potentiated in the presence of BACE-1 inhibitors, raising concerns about possible side effects mediated by the MMP in the case of therapeutic inhibition of BACE-1. The putative Aη-α peptide was found in the CSF of Alzheimer’s patients and healthy individuals, but the concentrations did not differ between the two groups, making it difficult for the moment to assess the importance of Aη-α in AD pathology. Of note, despite that MT5- and MT1-MMP cleave at the VLAN504-M505ISEPR site, only MT5-MMP and not MT1-MMP was identified in this study as having η-secretase activity in vivo at 10 days postnatal [111].
By the same time, our group tested the implication of MT5-MMP in AD using a different approach; we crossed transgenic 5xFAD mice carrying familial AD mutations in human APP and Psen1 genes [112] with MT5-MMP knockout mice [113]. The resulting bigenic 5xFAD/MT5-MMP-/- strain exhibits dramatic reductions of Aβ burden (e.g., plaques, oligomers, soluble Aβ40 and Aβ42) and C99 levels in cortical and hippocampal regions [114]. The fall in Aβ/C99 levels is concomitant with reduced glial reactivity and reduced levels of IL-1β and TNF-α in different brain areas [114, 115]. Functionally, 5xFAD mice exhibit impaired LTP [116, 117] and impaired learning and memory [118,119,120]. Both deficits are reversed in 5xFAD/MT5-MMP-/- bigenic mice, which show preservation of LTP and olfactory and spatial learning and memory, compared to 5xFAD controls [114, 115]. It is also important to note that the lack of MT5-MMP strongly decreases the release of a soluble N-terminal APP fragment of ~ 95 kDa (sAPP95), complementary of the transmembrane CTF-30 fragment [114], supporting the notion that APP is an in vivo substrate of MT5-MMP. In addition to these in vivo data, MT5-MMP co-immunoprecipitates with APP following MT5-MMP overexpression in HEK293 cells expressing App with the Swedish mutation (HEKswe), resulting in the release of sAPP95 and increases in Aβ40 levels [114, 115]. Although the precise molecular mechanism behind MT5-MMP actions is still elusive, it is known that the proteinase is internalized in the endosomal system [121] and favours APP sorting in endosomes [115], a major site of Aβ formation. In addition, it has been shown that N2a Swedish cells release exosomes containing η-CTF that can be uptaken by neurons [122]. Overall, MT5-MMP could promote trafficking of APP or its metabolites (i.e., CTF-30/η-CTF) into intracellular organelles for more efficient amyloidogenic processing by β- and γ-secretases. This way of cooperative cleavage has been recently shown for asparagine endopeptidase (δ-secretase), whose cleavage of APP upstream the β-cleavage site favours subsequent processing by β-secretase [123]. Not exclusively, it is also conceivable that η-CTF could be used as an exosomal cargo for intercellular propagation (see Fig. 1 for schematic representation of MT5-MMP interactions with APP).
The structurally close MT1-MMP shares about 60% sequence homology with MT5-MMP. While MT5-MMP is primarily expressed in the nervous system, MT1-MMP is ubiquitously distributed in the organism, including the brain. We found that MT1-MMP expression is upregulated in the brains of 5xFAD mice at symptomatic stages of the pathology and its overexpression in HEKswe cells stimulates C99 and Aβ production [78]. Moreover, MT1-MMP interacts with APP in HEKswe cells, and such interaction generates sAPP95 and the complementary transmembrane CTF-30, eventually leading to twofold increase of Aβ40 levels [124]. Consistent with its prominent β-secretase role, it was shown that BACE-1 inhibition with C3 almost suppresses basal Aβ production. Interestingly, such drastic effect of C3 is prevented in the presence of MT1-MMP, which restores Aβ basal levels, suggesting that MT1-MMP may function as a surrogate β-secretase upon BACE-1 inhibition [124]. The β-secretase-like activity of MT1-MMP may reveal functional redundancies with BACE-1, which could be useful for maintaining the physiological levels of Aβ in situations where, for example, BACE-1 would be therapeutically inhibited. From these studies, it appears that MT5-MMP and MT1-MMP behave differently in response to BACE-1 inhibition; while MT5-MMP would generate synaptotoxic peptides (i.e., Aη-α) leveraging on increased APP bioavailability for α-secretase, MT1-MMP would rather compensate for a physiological deficiency in Aβ. Another interesting feature is that sAPP95 release by MT1-MMP partially involves MMP-2 when activated by MT1-MMP. In the absence of MT1-MMP, MMP-2 loses its ability to generate sAPP95, indicating that MT1-MMP is the step-limiting enzyme [124]. It remains to be elucidated whether MMP-2 can also cleave at VLAN579-M580ISEPR, which would indicate the existence of a consensus cleavage site for APP shared by several MT-MMPs and MMP-2. These data highlight a new function for MMP-2—in tandem with MT1-MMP—in addition to its Aβ-degrading properties, thus providing a new example of the dual/multifunctional nature of MMPs.
Like MT5-MMP, MT1-MMP also favours endosomal APP sorting [124]. Gaining insight into endocytosis and recycling of MT-MMPs between the endosomal system and the membrane may be essential to understand the pathophysiological features of these enzymes. In this context, both MT1-MMP [125] and APP [126] are internalized through a clathrin-dependent mechanism that involves specific short sequences of their cytoplasmic tails. MT5-MMP internalization and recycling is mediated by interactions between the last three residues at carboxyl terminus and Mint3, a protein that contains two type III PDZ domains [121]. Mint3 has also been identified as an adaptor protein that promotes the export of APP from the Golgi complex [127]. Together, these data may reflect interdependent trafficking mechanisms between MT-MMPs and APP that enable functional interactions eventually leading to C99/Aβ production (summarized in Fig. 1).
Overall, MT-MMPs appear as new actors in AD pathogenesis, with multiple influences on pathways where proteolytic and non-proteolytic interactions with APP can coexist. A better understanding of such interactions is needed to shed light on the underlying pathogenic mechanisms.
Singular contributions of ADAMs to Alzheimer’s disease
Although the importance of ADAMs in AD has long been recognized for their contribution to α-secretase activity [128, 129], recent research extends their scope to mechanisms other than those involving a direct cleavage of APP. For instance, it has been shown that ADAM30 stimulates APP sorting to lysosomes and its degradation via the activation of cathepsin D [130]. It is also noteworthy that ADAM10 [131, 132] and ADAM17 [133] can shed the triggering receptor expressed on myeloid cells 2 (TREM2), a protein for which some genetic variants are linked to an increased risk of AD (see [134] for review). Mechanistically, lowering cell surface TREM2 results in reduction of microglia phagocytic activity, thereby possibly contributing to Aβ accumulation [131]. Similarly, the shedding of LRP-1 by different ADAMs (e.g., ADAM12) [99] might affect the ability of this receptor to promote endocytic-mediated clearance of Aβ. Finally, ADAMs could also contribute to the control of chronic inflammation by regulating cytokine activity. This could be the case of ADAM17, which sheds membrane-bound TNF-α and releases its soluble form [135]. Increasing experimental evidence suggests that TNF-α contributes to AD pathogenesis and TNF-α inhibitors, some of which are in clinical trials, may improve the pathological and cognitive outcome (reviewed in [136]).
TIMPs in Alzheimer’s disease
Along with the accumulation of data demonstrating the involvement of metalloproteinases in neurodegenerative processes , the interest in their inhibitors has increased in parallel. The list of endogenous MMP inhibitors and their physiological implications in the nervous system is rather extensive and has already been examined elsewhere [3]. We will focus on TIMPs in the context of this review.
Early work reported the presence of TIMP-1 in neuritic lesions of AD and colocalization with APP, as well as with abnormally phosphorylated and truncated tau [137]. Since then, numerous attempts to describe a clear profile of expression for TIMPs have been undertaken with eventually somehow discordant results. It has been shown that TIMP-1 and TIMP-2 levels remain stable when comparing patients suffering from AD or mild cognitive impairment (MCI) with non-demented controls [92]. While plasma levels of MMP-9 were higher in AD, PD and ALS patients compared to healthy individuals, no changes in TIMP-1 and TIMP-2 levels were observed in the same work [138]. A pilot study on a small cohort of AD patients reported moderately elevated levels of TIMP-1 in plasma [139]. The comparison of different types of dementia reveals that plasma levels of TIMP-1 and TIMP-2 respectively decrease in vascular and frontotemporal dementia, compared to AD and MCI [95]. However, TIMP-2 levels are increased in the CSF of Alzheimer patients [138]. Another study showed increased levels of TIMP-1 in bigenic APPSwDI/NOS2-/- mice compared to APPSwDI controls, along with decreased MMP activity and increased Aβ levels, suggesting that TIMP-1 could negatively influence the pathological outcome as a consequence of lowered nitric oxide production [140]. It has been proposed that the concentration of TIMP-1 in the CSF is a distinctive biomarker to differentiate AD patients from those with subcortical vascular disease, the latter having higher levels than the former [107]. In the same vein, Duits and collaborators reported decreased levels of TIMP-1 and TIMP-2 in the CSF of AD patients with cerebral microbleeds, arguing for an imbalance in favour of MMP proteolytic activity, which could eventually contribute to the generation of such lesions [141].
TIMP-1 was found to be secreted by neurons in response to MMP-9 release by mixed neuron/astrocyte cultures when exposed to neurotoxic Aβ25-35, and to stimulate astrocyte proliferation [142], in agreement with our previous work [143]. Coincident with gliosis, TIMP-1 mRNA expression is strongly upregulated at early stages (between 4 and 6 months) of the pathology in the brain of 5xFAD mice, whereas TIMP-2 and TIMP-3 mRNA levels show only moderate changes during the same period [78]. It remains to be assessed whether TIMP-1-mediated gliosis represents a self-defence mechanism to eliminate Aβ and/or a consequence of chronic inflammation. Increased levels of TIMP-1, along with the absence of MMP-9, have been observed in microvessels of AD compared to non-demented controls. The authors correlated this observation with the ability of thrombin to induce TIMP-1 expression in cultured brain endothelial cells. Altogether, these data suggest that changes in angiogenesis in AD brains may involve the modulation of the MMP-9/TIMP-1 balance [144].
Although not directly associated with AD, TIMP-2 mRNA and protein have been proposed as biomarkers of aging in the heart and cerebellum [145]. These results are particularly significant in the context of recent findings from Wyss–Coray’s group showing that TIMP-2 is an essential anti-aging factor as it promotes neuroplasticity, including LTP and hippocampal-dependent cognition. These conclusions were drawn after elegant parabiotic experiments in which plasma from young donor mice enriched with TIMP-2 compensated for cognitive deficits in elderly recipient mice, evoking the effect of an “elixir of eternal youth” [146]. With aging being the main risk factor for AD, TIMP-2, as a rejuvenating factor, could certainly play a role in the prevention of AD and other neurodegenerative diseases.
TIMP-3 inhibits APP cleavage by α-secretases ADAM10 and ADAM17, resulting in increased levels of C99 and Aβ, probably due to increased cleavage of APP by β-secretase [147]. The proposed mechanism implies that α-secretase inhibition by TIMP-3 could stimulate APP trafficking to endosomes, where β- and γ-secretases convert APP to Aβ. Consitent with this hypothesis, TIMP-3 levels are upregulated in brains from both AD patients and transgenic AD mice [147]. In addition, TIMP-3 expression is correlated with NFT in AD patients compared to non-demented individuals [148].
TIMP-4 has been less studied in neurodegenerative diseases than the other three TIMPs. Only one study reports that plasma levels of TIMP-4 are higher in AD patients than in healthy controls and TIMP-4 levels positively correlate with the severity of the disease [149]. While we are still waiting for clear evidence of TIMP-4 functions in the CNS, its inhibitory potential on MMPs suggests that it could contribute to modulate the progression of neurodegenerative diseases.
Parkinson’s disease
PD is the second most common neurodegenerative disorder after AD, characterised by motor symptoms, including rest tremor, bradykinesia, muscle stiffness, impaired posture and balance, and loss of automatic movement. Motor impairment is associated with selective loss of dopaminergic neurons in the substantia nigra and the degeneration of their striatal projections. Although PD is an incurable disease, a number of drugs and surgical interventions have shown to be effective and significantly improve symptoms for a limited period of time. A major feature of PD is the presence of fibrillar intracellular aggregates called Lewy bodies (LBs) in different brain areas. LBs are mainly composed of α-synuclein (α-Syn), a presynaptic protein of 140 amino acids for which three missense mutations (A30P, E46K and A53T) as well as wild-type gene multiplications, have been associated with familial forms of PD [150,151,152,153,154]. α-Syn aggregation has also been reported in sporadic forms of PD of unknown etiology, which constitute the majority of cases [155, 156]. It should be noted that α-Syn neuronal aggregates released into the extracellular space can be internalized by other neurons, reminiscent of a prion-like mechanism that can promote PD progression through the self-propagation of α-Syn [157]. In addition to α-Syn, ninety other molecules have been identified in LBs, including parkin, tau, leucine-rich repeat kinase 2 (LRRK2), DJ-1 and APP [158]. Even though a clear correlation exists between PD and the presence of LBs, the causal role of these aggregates has been questioned by recent studies in which early signs of neuronal dysfunction/death in the substantia nigra precede LBs formation [159]. In this context, other authors have suggested that α-Syn oligomers and protofibrils are true toxic assemblies as opposed to fibrillar structures contained in LBs, which would rather convey neuroprotective roles [158, 160,161,162]. Alternatively, there is also experimental evidence that truncated forms of α-Syn contribute to PD and dementia with Lewy bodies (DLB) pathology. Early work reported the presence of truncated α-Syn in isolated LBs from DLB brains [163] and in transgenic mice harbouring the A53T familial mutation [164]. Subsequently, 3 other C-terminal truncated major peptides (residues 1-78, 1-91 and 1-93) were identified, with the particularity that they were more abundant after digestion of A53T α-Syn compared to wild-type [165]. When the 1-93 peptide was overexpressed in the mouse substantia nigra it selectively killed dopaminergic neurons independently of LB-like formation. Crowther and colleagues demonstrated in vitro the ability of these truncated α-Syn forms to aggregate into filaments [166], while other authors found that stable expression of C-terminal truncated α-Syn increases neuroblastoma cell vulnerability to oxidative stress [167]. These data clearly indicate that α-Syn fragments contribute to PD and DLB pathogenesis, and several reports involve MMPs in α-Syn truncation. One study showed that, in this order of efficacy, MMP-3, MT1-MMP, MMP-2, MMP-1 and MMP-9 cleaved recombinant α-Syn in vitro [168], a cleavage that was confirmed in another study for MMP-1, MMP-3 and MMP-9 [169]. α-Syn fragments generated by MMP-3 are prone to form amyloidogenic aggregates that exhibit higher cytotoxicity compared to intact α-Syn. Further support for a pathogenic role of MMP-3 in PD comes from reports showing elevated expression of the enzyme in dopaminergic neurons of the substantia nigra in a rat model of PD induced by 6-hydroxydopamine (6-OHDA) [168], as well as in the brains of PD patients [165]. In addition, in another PD model induced by the injection of 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine (MPTP), the production of reactive oxygen species and the degeneration of dopamine neurons are attenuated in MMP-3-deficient mice [170], these effects being associated with the prevention of BBB disruption and the improvement of locomotor activity [171]. Along this line, intracellular activation of MMP-3 triggers neuronal apoptosis [172] and the subsequent release of active MMP-3, which stimulates the production of inflammatory cytokines by neighbouring microglia and eventually the exacerbation of dopaminergic neuron death [173]. Cultured microglia undergoes activation in response to α-Syn by a mechanism that involves the upregulation of MMP expression (i.e., MMP-1, -3, -8 and -9), and the consequent proteolytic activation of protease-activated receptor-1 [174]. Under these conditions, the inhibition of MMP-8 effectively reduces the levels of reactive oxygen species and inflammatory mediators such as TNF-α and IL-1β. MMP-3 implication in PD pathology has also been related to its ability to cleave DJ-1. The latter is a protein deglycase with protective antioxidant properties that mediates pleiotropic cellular responses, and whose mutation is associated with autosomal recessive early-onset PD [175]. MMP-3-mediated cleavage of DJ-1 impairs its antioxidant function in cultured dopamine-producing CATH.a cells upon oxidative stress [176]. The same study provided ground for in vivo cleavage, as the decrease in DJ-1 content observed after MPTP treatment was prevented in MMP-3 knockout mice. Interestingly, one of the DJ-1 mutations (L166P) prevents its dimerization and causes its proteolytic digestion by the proteasome [177, 178]. Also noteworthy, the L1669 mutation abrogates the anti-aggregation properties of wild-type DJ-1 with respect to α-Syn [179]. From these data, it follows that MMP-3 processing of DJ-1 could harm its anti-oxidant and anti-α-Syn aggregation properties. In addition, DJ-1 can be cleaved effectively by MT1-MMP as well as by MMP-1, -2, -8 and -9 [180], indicating that DJ-1 is a substrate of several MMPs and that these interactions may have pathophysiological significance in PD.
The functional and regulatory interplay between various MMPs and PD markers further strengthens the implication of MMPs in PD pathogenesis. Thus, α-Syn stimulates the expression of MMP-9 by cultured microglia and astrocytes [181]. Moreover, α-Syn promotes the expression of MT1-MMP and cell adhesion molecule CD44 in microglial cells. Shedding of CD44 by MT1-MMP facilitates microglia detachment from the ECM and promotes its migration in vitro [182]. Accordingly, siRNA-mediated silencing of MT1-MMP dramatically decreases the migration of the microglial cell line BV-2 when transplanted in the injured substantia nigra of 6-OHDA treated mice, suggesting that MT1-MMP stimulates microglia recruitment into injured brain areas and thus accelerates the degenerative process [182]. Mutations in the LRRK2 gene are the most common cause of autosomal dominantly inherited PD [183, 184]. One study on microglia and leukocytes from LRRK2 mutant mice showed that increased levels of inflammatory mediators and decreased levels of anti-inflammatory progranulin (PGRN) were associated with increased and decreased levels of MMP-2 and MMP-9, respectively. Also interesting, hippocampal neurons of LRRK2 mutant mice show high levels of MMP-12 [185], an enzyme that cleaves microglial PGRN, thereby possibly interfering with its anti-inflammatory properties [186]. Together, these data are particularly sound because microglia is a critical regulator of the inflammatory process that accompanies PD pathogenesis (reviewed in [187]).
In order to implement cell-based neuroprotective strategies against PD, conditioned media from cultured mesenchymal stem cells (MSC) have been used to disaggregate preformed α-Syn fibrils in vitro, with the consequent increase in cell viability. Conditioned media of cells treated with MMP-2 siRNA prevented the beneficial effects of normal conditioned media, suggesting that MMP-2 is one of the soluble factors that confer neuroprotection [188]. In line with these observations, reduced levels of MMP-2 in MPTP-treated mice can be restored by the inoculation of MSC. In addition, injection of MMP-2 in the brain of mice pre-inoculated with α-Syn degrades extracellular α-Syn aggregates and oligomers [188]. Also consistent with these data, MMP-2 levels were decreased in the substantia nigra of post mortem PD brains, while those of TIMP-1 were increased [189]. Whether the MMP/TIMP ratio may be used as a marker of PD progression is still unclear, despite studies associating reduced TIMP-2 levels and increased vulnerability of neuroblastoma cells to MPTP or 6-OHDA, which is consistent with TIMP-2 preventing the effects of these neurotoxins [190]. It appears, therefore, that different MMPs display opposite actions in PD; while MMP-3 cleavage of α-Syn could promote its aggregation into neurotoxic fibrils, MMP-2 could rather degrade them, thus providing neuroprotection. Therefore, the distinction between both MMPs should be considered in prospective anti-PD therapies with MMPs as potential targets in PD. In this line, it has been shown that the inhibition of MMP-8 in the LRRK2G2019S mouse model reduces the levels of inflammatory mediators and improves locomotor activity during systemic inflammatory LPS challenge [191]. Likewise, hydroxamate-based MMP inhibitor Ro28-2653, which targets MMP-2, -9 and MT1-MMP, significantly reduces neuronal loss and MMP-9 levels in the substantia nigra of MPTP-treated mice [192].
There are no reports yet linking ADAM function to PD. However, since the contribution of reactive microglia to pathology is increasingly supported by experimental data, it would be justified to explore in this context the modulation by ADAMs of proteins involved in microglial function, such as TREM2. Of note, some authors have reported association between TREM2 variants and increased risk of PD, although the data are not conclusive for the moment [134].
Amyotrophic lateral sclerosis
Amyotrophic lateral sclerosis (ALS) is a rare rapidly progressive neurodegenerative disease that selectively affects motor neurons in the brain, brainstem and spinal cord, leading to severe disability, muscle atrophy, and also cognitive deficits in about 40% of ALS patients. Poor prognosis is a distinctive clinical feature and life expectancy after the diagnosis is less than 20 months in 50% of patients, who often die from ventilatory failure (see for review [193]). Currently, there are no drugs that can cure or prevent ALS and the rapid course of the disease, as well as the lack of reliable biomarkers, make therapeutic strategies particularly challenging. As with many other degenerative diseases, aging is a major risk factor, with a rapid increase in prevalence after age 55 [193]. While the majority of patients have sporadic ALS of unknown multifactorial origin, genetically linked ALS accounts for between 5 and 10% of cases. Deleterious genetic mutations affect genes coding for proteins implicated in RNA processing, and protein transport and clearance, like C9orf72, SOD1, TDP-43 and FUS (reviewed in [194]).
The pathogenesis of ALS is likely the result of a combination of genetic and environmental factors that may influence key biological processes such as excitatory/inhibitory neurotransmitter balance, BBB integrity, protein folding, oxidative stress or neuroinflammation. All of these events are commonly linked with MMP activity, and a number of evidences discussed below support the role of MMPs in the disease.
Many studies on ALS have used transgenic mice expressing Cu2+/Zn2+ superoxide dismutase (SOD1) carrying the G93A familial mutation (SOD1G93A). In these mice, the involvement of MMP-9 in ALS pathogenesis is still under debate because different laboratories have reported conflicting data. One study shows that MMP-9 deletion in SOD1G93A mice accelerates motor neuron disease and increases cell death [195], whereas another study reports decreased neuron loss and greater survival in MMP-9 knockout mice in correlation with decreased TNF-α and FasL immunostaining [196]. Selective expression of MMP-9 in fast-fatigable motor neurons, which are highly vulnerable in SOD1G93A mice compared to the fast-fatigue resistant and slow motor neuron subtypes, is concomitant with the activation of the unfolded protein response and endoplasmic reticulum stress mark characteristic of early pathological stages of SOD1G93A. Genetic deletion of MMP-9 in these mice, as well as pharmacological inhibition or viral gene therapy, delays muscle denervation [197]. In an attempt to interpret selective motor neuron vulnerability, it has been shown that osteopontin, an ECM protein, is selectively expressed in fast-fatigue resistant and slow motor neurons, and stimulates late expression of MMP-9 in these neuronal subtypes, which could contribute to the second wave of degeneration in ALS by a mechanism controlled by MMP-9 [198]. Another study showed that early administration of MMP inhibitor Ro28-2653 increases the survival of SOD1G93A mice [199], suggesting a powerful detrimental activity of MMPs in ALS. in vitro studies further support the possible contribution of MMP-9 to ALS, as MMP-9 inhibition with glycoursodeoxycholic acid in a cell model of SOD1G93A prevents cell degeneration [200]. Although these data suggest that MMP-9 can be a candidate for therapeutic intervention in ALS, caution is required; indeed, in a sporadic model of ALS using rNLS8 mice, MMP-9 knockdown leads to the preservation of motor neurons and muscle function, even if in the long run the reduction of MMP-9 results in premature death of a subset of rNLS8 mice [201]. It is then possible that targeting MMP-9 outside the neuromotor system may cause adverse effects due to the inhibition of more general physiological processes controlled by this MMP. In addition, MMP-9 could also be considered as an early biomarker of the disease. MMP-9 (and also MMP-2) levels measured by gelatin zymography were found to increase in the serum of SOD1G93A mice at the beginning of the symptomatic phases of the pathology, as opposed to significantly lower levels observed during the pre-symptomatic and late-end stages [202].
Beyond a neurocentric interpretation of ALS pathogenesis, astrocytes could also play a deleterious role, thereby justifying attempts to replace diseased astrocytes by healthy astrocytes. Izrael and colleagues intrathecally injected astrocytes derived from human embryonic stem cells into transgenic SOD1G93A mice and rats, and observed an improvement of motor performance and delayed disease onset linked to astrocytic secretion of TIMP-1 and TIMP-2 [203]. On the contrary, a positive correlation has been put forward between TIMP-3 levels and neurodegeneration. Degenerating neurons of SOD1G93A mice exhibit augmented TIMP-3 levels in parallel with increased interactions between Fas and Fas-associated protein with death domain (FADD). Mechanistically, TIMP-3 inhibition of FADD cleavage by MMP-3 would stabilize Fas–FADD interactions, thereby promoting Fas-mediated apoptosis [204].
Few studies have been conducted in patients to explore possible changes in MMP content. Pioneer work in CNS tissue from ALS patients localized increased immunostaining of MMP-2 in astrocytes and MMP-9 in pyramidal neurons of the motor cortex and in spinal motor neurons [205]. In addition, one study reported increased levels of MMP-9 in plasma of ALS patients but not in CSF [206], while another study also reported an increase in MMP-9 levels in CSF [207]. It has been shown by ELISA assay that the concentration of MT1-MMP, MMP-2 and TIMP-1 increases in the CSF of ALS patients compared to healthy controls [208], thus confirming previous work showing increased TIMP-1 levels in the CSF as well [138].
There is scarce information on ADAMs in ALS. One study described enhanced secretion of TNF-α by microglia from SOD1G93A, SOD1L8Q, or SOD1G10V mutants upon shedding by ADAM10 and ADAM17, thereby contributing to microglia inflammatory response [209]. In the same vein, it was shown that iron accumulation in ventral motor neurons of SOD1G93A mice induced oxidative stress and the secretion of TNF-α mediated by increased ADAM17 activity [210]. It has been suggested that the reduction in ADAMTS-4 observed in the spinal cord of SOD1G93A mice may be an adaptive mechanism to counteract the potential neurotoxic effect of this metalloproteinase [211]. The authors reached this conclusion after observing significant motor neuron death following the injection of recombinant ADAMTS-4 in the spinal cord of SOD1G93A mice. Collectively, different ADAMs could, therefore, contribute to the degenerative process that takes place in ALS.
Huntington’s disease
HD (also known as Huntington’s chorea) is the most frequent among inherited neurodegenerative polyglutamine disorders. It is still an incurable disease that causes changes in mood and mental abilities, as well as deficits in motor coordination and ultimately dementia. HD is not properly speaking an aging-related disease since symptoms may appear at the age of 40 or even earlier. The cause of the disease lies on the mutation of the gene coding for huntingtin (Htt), which presents an expanded CAG triplet repeat in exon 1 that encodes a chain of polyglutamine (polyQ) residues close to the N-terminus of Htt. This results in the aggregation of Htt in the nucleus and cytoplasm of neurons and the consequent cell demise that affects mainly the striatum and cortex [212,213,214]. The underlying neurotoxic mechanism is still elusive, but several lines of evidence point to Htt proteolysis by caspases and calpains, which releases N-terminal small fragments thought to be particularly toxic [215,216,217]. More recently, Miller and collaborators expanded the repertoire of proteinases involved in this process to MMPs [218]. They screened 514 siRNA targeting all the proteinases encoded by the human genome to determine those whose inhibition would reduce Htt processing, and more precisely the production of small N-terminal fragments. Among 11 confirmed proteinases, they found MMP-10, MT1-MMP and MMP-23B. They confirmed the upregulation of MMP-10 and MT1-MMP expression in striatal Hdh111Q/111Q cells as compared to Hdh7Q/7Q cells, and established a good correlation between the knockdown of these MMPs and a significant reduction of caspase activation in Hdh111Q/111Q cells. In the same study it was shown that TIMP-1 and TIMP-3 inhibited Htt cytotoxicity in Hdh111Q/111Q cells. Moreover, striatal MMP activity was also increased in Htt YAC128 (glutamine repeat expansion model) and R/62 (N-terminal fragment model) mouse models of HD. While MT1-MMP and MMP-2 do not directly cleave Htt, MMP-10 generates a N-terminal fragment of 48 kDa after cleavage at residue 402, very close to the N-terminus. Importantly, Hdh111Q/111Q cell death was prevented upon knockdown of MMP-10. Further work from the same laboratory confirmed significant alterations of MMPs expression in induced pluripotent stem cell-derived neural stem cells from HD patients (HD-NSCs) with an expanded CAG repeat, compared to the isogenic corrected control [219]. The study shows that the expression of MMP-3 and -10 increases in HD-NSCs compared to control NSCs, in contrast with the decrease observed in MT1-MMP, TIMP-1 and TIMP-2. TIMP-1 levels were restored by TGF-β treatment, in pace with reduced neurotoxicity of Htt, suggesting overall a beneficial effect of TIMP-1-mediated inhibition of Htt proteolysis by MMP-3 and -10 [219]. However, this idea is questionable, as other authors have reported increased levels of TIMP-1 and -2 in the CSF of HD patients [138].
MMP-9 levels are increased in post mortem tissues of HD patients, as well as the content of pro-inflammatory mediators MCP-1, IL-6, IL-8 and the anti-inflammatory IL-10 [220]. Likewise, plasma MMP-9 and IL-6 levels are higher in HD patients compared to healthy controls and this is also observed in R6/2 HD mice compared to wild-type littermates [221]. Moreover, MMP-3 and MMP-9 levels increase in CSF from HD patients in correlation with disease severity [222]. The same authors showed that cultured microglia from YAC128 mice (transgenic mouse model with a 128-glutamine stretch) exhibits increased secretion of cytokines upon stimulation with MMP-3, an activator of microglia. Interestingly, the pro-inflammatory effect of MMP-3 is equivalent to that caused by LPS treatment, linking the action of MMPs in HD to their pro-inflammatory properties. Seemingly, in a rat model of HD induced by intraperitoneal administration of a natural toxin, 3-Nitropropionic acid, MMP-9 expression and gelatinolytic activity are upregulated in injured striatal blood vessels, suggesting the possible implication of MMP-9 in BBB disruption in HD. Noticeably, MMP-9 expression has been reported to be upregulated in subsets of astrocytes and microglial cells in the vicinity of lesions [223]. In contrast with the aforementioned studies, other authors reported recently in HD patients no changes in CSF MMP-9 levels and the lack of neuroinflammation at premanifest stages of the pathology [224].
With regard to ADAMs, one study reports the physiological interaction between ADAM10 and Htt during neurulation [225]. The authors found that Htt inhibits N-cadherin shedding by ADAM10, which promotes neurulation and rosette formation. They also found that ADAM10 activity increased in the Htt-deficient adult brain, suggesting a role for Htt in synapse plasticity and remodelling. The question arises as to whether deficient regulation of ADAM10/N-cadherin in HD brains with dysfunctional Htt could possibly contribute to the disease.
Concluding remarks and perspectives
The traditional view of metalloproteinases as merely non-specific degrading enzymes is definitely obsolete. Their implications in homeostatic or detrimental pathways in many neurodegenerative diseases mobilize finely tuned proteolytic interactions with substrates and the generation of biologically active cleavage products. A plethora of substrates has been identified and we can anticipate that their number will grow in the coming years in the light of new high-throughput proteomic techniques. Table 1 summarizes, in a non-exhaustive manner, some of principal substrates that have been cited in this review.
In some cases, metalloproteinases have a dual effect, as it is the case for MT1-MMP in AD experimental models by degrading Aβ and also contributing to its formation. Likewise, α-secretases (e.g., ADAM10) may generate neuroprotective sAPPα and give rise to synaptotoxic C-terminal fragments in synergy with MT5-MMP. We are witnessing the expansion of APP processing beyond prototypical control by canonical secretases. In this scenario, MT-MMPs appear to play an important role in the generation of new truncated APP fragments, whose functions are still poorly understood. Similar challenges arise when considering the physiological and pathological roles of breakdown products resulting from the metalloproteinase-mediated processing of tau, α-Syn or Htt in AD, PD or HD, respectively. Although proteolysis is clearly the main functional characteristic of metalloproteinases, the field now opens up to study proteolysis-independent protein–protein interactions, such as those reported for ADAM30, which bring to light new ways in which metalloproteinases can influence disease outcomes. Therefore, it is plausible that new strategies will emerge based on the modulation non-proteolytic interactions between metalloproteinases and partner proteins. In addition, this could offer alternatives to targeting the proteolytic activity of metalloproteinases, which often suffers from the lack of specificity due to highly conserved catalytic domains between family members.
Inflammation is a common event in neurodegenerative diseases and many metalloproteinases are produced by brain and peripheral immune cells. Gaining insight into the disease will also require a better understanding of how the metalloproteinases released by these cells contribute to pathology in a given spatio-temporal context and/or how metalloproteinases can activate/inactivate immune cells by controlling the cleavage of key receptors and cytokines (e.g., TREM2, TNF-α, IL-1β, etc).
From all the above, it appears that the study of metalloproteinases warrants a more global approach in which we can learn from their conserved functions as well as their specificities. These concepts should inspire future research on neurodegenerative diseases, where a thorough knowledge of biological processes should pave the way for exciting discoveries that will help to design more effective diagnostic and therapeutic strategies.
Abbreviations
- 6-OHDA:
-
6-Hydroxydopamine
- 5xFAD:
-
Transgenic mice bearing 5 familial mutations on human App and Psen1 genes
- AD:
-
Alzheimer’s disease
- Aβ:
-
Amyloid beta peptide
- ADAM:
-
A disintegrin and metalloproteinase
- ADAMTS:
-
ADAMs with thrombospondin motifs
- ALS:
-
Amyotrophic lateral sclerosis
- APOE:
-
Apolipoprotein E
- APP:
-
Amyloid precursor protein
- BACE-1:
-
Beta-site APP cleaving enzyme 1
- BBB:
-
Blood–brain barrier
- C3:
-
BACE-1 inhibitor IV
- CAA:
-
Cerebral amyloid angiopathy
- CNS:
-
Central nervous system
- CSF:
-
Cerebrospinal fluid
- CTF:
-
C-terminal fragment
- C99:
-
APP-CTF of 99 amino acids
- DAPT:
-
N-[N-(3,5-Difluorophenacetyl)-l-alanyl]-S-phenylglycine t-butyl ester, γ-secretase inhibitor
- DLB:
-
Dementia with Lewy bodies
- ECM:
-
Extracellular matrix
- FADD:
-
Fas-associated protein with death domain
- HD:
-
Huntington’s disease
- HD-NSCs:
-
Neural stem cells from HD patients
- HEKswe:
-
Human embryonic kidney cells that express App gene with the Swedish mutation
- Htt:
-
Huntingtin
- ICV:
-
Intracerebroventricular
- IDE:
-
Insulin degrading enzyme
- IL-1:
-
Interleukin-1
- LBs:
-
Lewy bodies
- LDLR:
-
Low-density lipoprotein receptor
- LRP-1:
-
Low-density lipoprotein receptor-related protein 1
- LRRK2:
-
Leucine-rich repeat kinase 2
- LTP:
-
Long-term potentiation
- MCP-1:
-
Monocyte chemoattractant protein 1
- MMP:
-
Matrix metalloproteinase
- MPTP:
-
1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine
- MSC:
-
Mesenchymal stem cells
- MT-MMP:
-
Membrane-type matrix metalloproteinase
- MTT:
-
3-(4,5-Dimethylthiazol-2-yl)-2,5-diphenyl tetrazolium bromide
- NFT:
-
Neurofibrillary tangles
- NSC:
-
Neural stem cell
- NTF:
-
N-terminal fragment
- PD:
-
Parkinson’s disease
- PGRN:
-
Progranulin
- Psen 1 and Psen 2:
-
Presenilin 1 and 2
- RAGE:
-
Receptor for advanced glycation end products
- sAPPα/β:
-
Soluble APPα/β
- TIMP:
-
Tissue inhibitor of metalloproteinases
- TNF-α:
-
Tumour necrosis factor α
- TREM2:
-
Triggering receptor expressed on myeloid cells 2
References
Hsia H-E, Tüshaus J, Brummer T, Zheng Y, Scilabra SD, Lichtenthaler SF (2019) Functions of ‘a disintegrin and metalloproteases (ADAMs)’ in the mammalian nervous system. Cell Mol Life Sci. https://doi.org/10.1007/s00018-019-03173-7
Rivera S, Khrestchatisky M, Kaczmarek L, Rosenberg GA, Jaworski DM (2010) Metzincin proteases and their inhibitors: foes or friends in nervous system physiology? J Neurosci 30(46):15337–15357. https://doi.org/10.1523/JNEUROSCI.3467-10.2010
Baranger K, Rivera S, Liechti FD, Grandgirard D, Bigas J, Seco J, Tarrago T, Leib SL, Khrestchatisky M (2014) Endogenous and synthetic MMP inhibitors in CNS physiopathology. Prog Brain Res 214:313–351. https://doi.org/10.1016/B978-0-444-63486-3.00014-1
Okada Y (2017) Proteinases and matrix degradation. In: Firestein GS, Budd RC, Gabriel SE, McInnes IB, O’Dell JR (eds) Kelley and Firestein’s textbook of rheumatology, vol 1, 10th edn. Elsevier, Philadelphia, pp 106–125. https://doi.org/10.1016/B978-0-323-31696-5.00008-5
Overall CM, Tam EM, Kappelhoff R, Connor A, Ewart T, Morrison CJ, Puente X, Lopez-Otin C, Seth A (2004) Protease degradomics: mass spectrometry discovery of protease substrates and the CLIP-CHIP, a dedicated DNA microarray of all human proteases and inhibitors. Biol Chem 385(6):493–504. https://doi.org/10.1515/BC.2004.058
Starr AE, Dufour A, Maier J, Overall CM (2012) Biochemical analysis of matrix metalloproteinase activation of chemokines CCL15 and CCL23 and increased glycosaminoglycan binding of CCL16. J Biol Chem 287(8):5848–5860. https://doi.org/10.1074/jbc.M111.314609
Hsu TI, Lin SC, Lu PS, Chang WC, Hung CY, Yeh YM, Su WC, Liao PC, Hung JJ (2015) MMP7-mediated cleavage of nucleolin at Asp255 induces MMP9 expression to promote tumor malignancy. Oncogene 34(7):826–837. https://doi.org/10.1038/onc.2014.22
Rosenberg GA (2017) Extracellular matrix inflammation in vascular cognitive impairment and dementia. Clin Sci 131(6):425–437. https://doi.org/10.1042/CS20160604
Wojcik L, Sawicka A, Rivera S, Zalewska T (2009) Neurogenesis in gerbil hippocampus following brain ischemia: focus on the involvement of metalloproteinases. Acta Neurobiol Exp 69(1):52–61
Ould-yahoui A, Tremblay E, Sbai O, Ferhat L, Bernard A, Charrat E, Gueye Y, Lim NH, Brew K, Risso JJ, Dive V, Khrestchatisky M, Rivera S (2009) A new role for TIMP-1 in modulating neurite outgrowth and morphology of cortical neurons. PLoS One 4(12):e8289. https://doi.org/10.1371/journal.pone.0008289
Ould-Yahoui A, Sbai O, Baranger K, Bernard A, Gueye Y, Charrat E, Clement B, Gigmes D, Dive V, Girard SD, Feron F, Khrestchatisky M, Rivera S (2013) Role of matrix metalloproteinases in migration and neurotrophic properties of nasal olfactory stem and ensheathing cells. Cell Transplant 22(6):993–1010. https://doi.org/10.3727/096368912X657468
Schonbeck U, Mach F, Libby P (1998) Generation of biologically active IL-1 beta by matrix metalloproteinases: a novel caspase-1-independent pathway of IL-1 beta processing. J Immunol 161(7):3340–3346
Rosenberg GA (2002) Matrix metalloproteinases in neuroinflammation. Glia 39(3):279–291. https://doi.org/10.1002/glia.10108
Marchant DJ, Bellac CL, Moraes TJ, Wadsworth SJ, Dufour A, Butler GS, Bilawchuk LM, Hendry RG, Robertson AG, Cheung CT, Ng J, Ang L, Luo Z, Heilbron K, Norris MJ, Duan W, Bucyk T, Karpov A, Devel L, Georgiadis D, Hegele RG, Luo H, Granville DJ, Dive V, McManus BM, Overall CM (2014) A new transcriptional role for matrix metalloproteinase-12 in antiviral immunity. Nat Med 20(5):493–502. https://doi.org/10.1038/nm.3508
Nagase H, Brew K (2003) Designing TIMP (tissue inhibitor of metalloproteinases) variants that are selective metalloproteinase inhibitors. Bioch Soc Symp 70:201–212
Amour A, Knight CG, Webster A, Slocombe PM, Stephens PE, Knauper V, Docherty AJ, Murphy G (2000) The in vitro activity of ADAM-10 is inhibited by TIMP-1 and TIMP-3. FEBS Lett 473(3):275–279
Vandooren J, Van den Steen PE, Opdenakker G (2013) Biochemistry and molecular biology of gelatinase B or matrix metalloproteinase-9 (MMP-9): the next decade. Crit Rev Biochem Mol 48(3):222–272. https://doi.org/10.3109/10409238.2013.770819
Shofuda K, Moriyama K, Nishihashi A, Higashi S, Mizushima H, Yasumitsu H, Miki K, Sato H, Seiki M, Miyazaki K (1998) Role of tissue inhibitor of metalloproteinases-2 (TIMP-2) in regulation of pro-gelatinase A activation catalyzed by membrane-type matrix metalloproteinase-1 (MT1-MMP) in human cancer cells. J Biochem 124(2):462–470
Leco KJ, Apte SS, Taniguchi GT, Hawkes SP, Khokha R, Schultz GA, Edwards DR (1997) Murine tissue inhibitor of metalloproteinases-4 (Timp-4): cDNA isolation and expression in adult mouse tissues. FEBS Lett 401(2–3):213–217
Derry JM, Barnard PJ (1992) Physical linkage of the A-raf-1, properdin, synapsin I, and TIMP genes on the human and mouse X chromosomes. Genomics 12(4):632–638
Pohar N, Godenschwege TA, Buchner E (1999) Invertebrate tissue inhibitor of metalloproteinase: structure and nested gene organization within the synapsin locus is conserved from Drosophila to human. Genomics 57(2):293–296. https://doi.org/10.1006/geno.1999.5776
Rahkonen OP, Koskivirta IM, Oksjoki SM, Jokinen E, Vuorio EI (2002) Characterization of the murine Timp4 gene, localization within intron 5 of the synapsin 2 gene and tissue distribution of the mRNA. Biochim Biophys Acta 1577(1):45–52
Prince M, Comas-Herrera A, Knapp M, Guerchet M, Karagiannidou M (2016) World Alzheimer Report 2016. Improving healthcare for people living with dementia. Coverage, quality and costs now and in the future. Alzheimer’s Disease International, London
Mullane K, Williams M (2013) Alzheimer’s therapeutics: continued clinical failures question the validity of the amyloid hypothesis-but what lies beyond? Biochem Pharmacol 85(3):289–305. https://doi.org/10.1016/j.bcp.2012.11.014
Mikulca JA, Nguyen V, Gajdosik DA, Teklu SG, Giunta EA, Lessa EA, Tran CH, Terak EC, Raffa RB (2014) Potential novel targets for Alzheimer pharmacotherapy: II Update on secretase inhibitors and related approaches. J Clin Pharm Ther 39(1):25–37. https://doi.org/10.1111/jcpt.12112
Mehta D, Jackson R, Paul G, Shi J, Sabbagh M (2017) Why do trials for Alzheimer’s disease drugs keep failing? A discontinued drug perspective for 2010-2015. Expert Opin Investig Drugs 26(6):735–739. https://doi.org/10.1080/13543784.2017.1323868
Selkoe DJ, Hardy J (2016) The amyloid hypothesis of Alzheimer’s disease at 25 years. EMBO Mol Med 8(6):595–608. https://doi.org/10.15252/emmm.201606210
Lesne SE, Sherman MA, Grant M, Kuskowski M, Schneider JA, Bennett DA, Ashe KH (2013) Brain amyloid-beta oligomers in ageing and Alzheimer’s disease. Brain 136(Pt 5):1383–1398. https://doi.org/10.1093/brain/awt062
Tan JZA (1861) Gleeson PA (2019) The role of membrane trafficking in the processing of amyloid precursor protein and production of amyloid peptides in Alzheimer’s disease. BBA-Biomembranes 4:697–712. https://doi.org/10.1016/j.bbamem.2018.11.013
De Strooper B (2010) Proteases and proteolysis in Alzheimer disease: a multifactorial view on the disease process. Physiol Rev 90(2):465–494. https://doi.org/10.1152/physrev.00023.2009
Kim J, Castellano JM, Jiang H, Basak JM, Parsadanian M, Pham V, Mason SM, Paul SM, Holtzman DM (2009) Overexpression of low-density lipoprotein receptor in the brain markedly inhibits amyloid deposition and increases extracellular A beta clearance. Neuron 64(5):632–644. https://doi.org/10.1016/j.neuron.2009.11.013
Castellano JM, Deane R, Gottesdiener AJ, Verghese PB, Stewart FR, West T, Paoletti AC, Kasper TR, DeMattos RB, Zlokovic BV, Holtzman DM (2012) Low-density lipoprotein receptor overexpression enhances the rate of brain-to-blood Abeta clearance in a mouse model of beta-amyloidosis. Proc Natl Acad Sci USA 109(38):15502–15507. https://doi.org/10.1073/pnas.1206446109
Basak JM, Verghese PB, Yoon H, Kim J, Holtzman DM (2012) Low-density lipoprotein receptor represents an apolipoprotein E-independent pathway of Abeta uptake and degradation by astrocytes. J Biol Chem 287(17):13959–13971. https://doi.org/10.1074/jbc.M111.288746
Jaeger LB, Dohgu S, Hwang MC, Farr SA, Murphy MP, Fleegal-DeMotta MA, Lynch JL, Robinson SM, Niehoff ML, Johnson SN, Kumar VB, Banks WA (2009) Testing the neurovascular hypothesis of Alzheimer’s disease: LRP-1 antisense reduces blood-brain barrier clearance, increases brain levels of amyloid-beta protein, and impairs cognition. J Alzheimers Dis 17(3):553–570. https://doi.org/10.3233/JAD-2009-1074
Storck SE, Meister S, Nahrath J, Meissner JN, Schubert N, Di Spiezio A, Baches S, Vandenbroucke RE, Bouter Y, Prikulis I, Korth C, Weggen S, Heimann A, Schwaninger M, Bayer TA, Pietrzik CU (2016) Endothelial LRP1 transports amyloid-beta(1-42) across the blood-brain barrier. J Clin Invest 126(1):123–136. https://doi.org/10.1172/JCI81108
Liu CC, Hu J, Zhao N, Wang J, Wang N, Cirrito JR, Kanekiyo T, Holtzman DM, Bu G (2017) Astrocytic LRP1 mediates brain abeta clearance and impacts amyloid deposition. J Neurosci 37(15):4023–4031. https://doi.org/10.1523/JNEUROSCI.3442-16.2017
Cai Z, Liu N, Wang C, Qin B, Zhou Y, Xiao M, Chang L, Yan LJ, Zhao B (2016) Role of RAGE in Alzheimer’s disease. Cell Mol Neurobiol 36(4):483–495. https://doi.org/10.1007/s10571-015-0233-3
Wan W, Cao L, Liu L, Zhang C, Kalionis B, Tai X, Li Y, Xia S (2015) Abeta(1-42) oligomer-induced leakage in an in vitro blood-brain barrier model is associated with up-regulation of RAGE and metalloproteinases, and down-regulation of tight junction scaffold proteins. J Neurochem 134(2):382–393. https://doi.org/10.1111/jnc.13122
Fang F, Yu Q, Arancio O, Chen D, Gore SS, Yan SS, Yan SF (2018) RAGE mediates Abeta accumulation in a mouse model of Alzheimer’s disease via modulation of beta- and gamma-secretase activity. Hum Mol Genet 27(6):1002–1014. https://doi.org/10.1093/hmg/ddy017
Muller UC, Deller T, Korte M (2017) Not just amyloid: physiological functions of the amyloid precursor protein family. Nat Rev Neurosci 18(5):281–298. https://doi.org/10.1038/nrn.2017.29
Jorissen E, Prox J, Bernreuther C, Weber S, Schwanbeck R, Serneels L, Snellinx A, Craessaerts K, Thathiah A, Tesseur I, Bartsch U, Weskamp G, Blobel CP, Glatzel M, De Strooper B, Saftig P (2010) The disintegrin/metalloproteinase ADAM10 is essential for the establishment of the brain cortex. J Neurosci 30(14):4833–4844. https://doi.org/10.1523/JNEUROSCI.5221-09.2010
Kuhn PH, Wang H, Dislich B, Colombo A, Zeitschel U, Ellwart JW, Kremmer E, Rossner S, Lichtenthaler SF (2010) ADAM10 is the physiologically relevant, constitutive alpha-secretase of the amyloid precursor protein in primary neurons. EMBO J 29(17):3020–3032. https://doi.org/10.1038/emboj.2010.167
Buxbaum JD, Liu KN, Luo Y, Slack JL, Stocking KL, Peschon JJ, Johnson RS, Castner BJ, Cerretti DP, Black RA (1998) Evidence that tumor necrosis factor alpha converting enzyme is involved in regulated alpha-secretase cleavage of the Alzheimer amyloid protein precursor. J Biol Chem 273(43):27765–27767
Chasseigneaux S, Allinquant B (2012) Functions of Abeta, sAPPalpha and sAPPbeta : similarities and differences. J Neurochem 120(Suppl 1):99–108. https://doi.org/10.1111/j.1471-4159.2011.07584.x
Hick M, Herrmann U, Weyer SW, Mallm JP, Tschape JA, Borgers M, Mercken M, Roth FC, Draguhn A, Slomianka L, Wolfer DP, Korte M, Muller UC (2015) Acute function of secreted amyloid precursor protein fragment APPsalpha in synaptic plasticity. Acta Neuropathol 129(1):21–37. https://doi.org/10.1007/s00401-014-1368-x
Rose C, Dorard E, Audrain M, Gorisse-Hussonnois L, Cartier N, Braudeau J, Allinquant B (2018) Transient increase in sAPPalpha secretion in response to Abeta1-42 oligomers: an attempt of neuronal self-defense? Neurobiol Aging 61:23–35. https://doi.org/10.1016/j.neurobiolaging.2017.09.008
Soscia SJ, Kirby JE, Washicosky KJ, Tucker SM, Ingelsson M, Hyman B, Burton MA, Goldstein LE, Duong S, Tanzi RE, Moir RD (2010) The Alzheimer’s disease-associated amyloid beta-protein is an antimicrobial peptide. PLoS One 5(3):e9505. https://doi.org/10.1371/journal.pone.0009505
Kumar DK, Choi SH, Washicosky KJ, Eimer WA, Tucker S, Ghofrani J, Lefkowitz A, McColl G, Goldstein LE, Tanzi RE, Moir RD (2016) Amyloid-beta peptide protects against microbial infection in mouse and worm models of Alzheimer’s disease. Sci Transl Med 8(340):340ra372. https://doi.org/10.1126/scitranslmed.aaf1059
Eimer WA, Vijaya Kumar DK, Navalpur Shanmugam NK, Rodriguez AS, Mitchell T, Washicosky KJ, Gyorgy B, Breakefield XO, Tanzi RE, Moir RD (2018) Alzheimer’s disease-associated beta-amyloid is rapidly seeded by herpesviridae to protect against brain infection. Neuron 100(6):1527–1532. https://doi.org/10.1016/j.neuron.2018.11.043
Dominy SS, Lynch C, Ermini F, Benedyk M, Marczyk A, Konradi A, Nguyen M, Haditsch U, Raha D, Griffin C, Holsinger LJ, Arastu-Kapur S, Kaba S, Lee A, Ryder MI, Potempa B, Mydel P, Hellvard A, Adamowicz K, Hasturk H, Walker GD, Reynolds EC, Faull RLM, Curtis MA, Dragunow M, Potempa J (2019) Porphyromonas gingivalis in Alzheimer’s disease brains: Evidence for disease causation and treatment with small-molecule inhibitors. Sci Adv 5(1):33. https://doi.org/10.1126/sciadv.aau3333
Abramov E, Dolev I, Fogel H, Ciccotosto GD, Ruff E, Slutsky I (2009) Amyloid-beta as a positive endogenous regulator of release probability at hippocampal synapses. Nat Neurosci 12(12):1567–1576. https://doi.org/10.1038/nn.2433
Puzzo D, Privitera L, Leznik E, Fa M, Staniszewski A, Palmeri A, Arancio O (2008) Picomolar amyloid-beta positively modulates synaptic plasticity and memory in hippocampus. J Neurosci 28(53):14537–14545. https://doi.org/10.1523/JNEUROSCI.2692-08.2008
Morley JE, Farr SA, Banks WA, Johnson SN, Yamada KA, Xu L (2010) A physiological role for amyloid-beta protein:enhancement of learning and memory. J Alzheimers Dis 19(2):441–449. https://doi.org/10.3233/JAD-2009-1230
Puzzo D, Privitera L, Palmeri A (2012) Hormetic effect of amyloid-beta peptide in synaptic plasticity and memory. Neurobiol Aging 33(7):1484. https://doi.org/10.1016/j.neurobiolaging.2011.12.020
Lawrence JL, Tong M, Alfulaij N, Sherrin T, Contarino M, White MM, Bellinger FP, Todorovic C, Nichols RA (2014) Regulation of presynaptic Ca2+, synaptic plasticity and contextual fear conditioning by a N-terminal beta-amyloid fragment. J Neurosci 34(43):14210–14218. https://doi.org/10.1523/JNEUROSCI.0326-14.2014
Palmeri A, Ricciarelli R, Gulisano W, Rivera D, Rebosio C, Calcagno E, Tropea MR, Conti S, Das U, Roy S, Pronzato MA, Arancio O, Fedele E, Puzzo D (2017) Amyloid-beta peptide is needed for cGMP-induced long-term potentiation and memory. J Neurosci 37(29):6926–6937. https://doi.org/10.1523/JNEUROSCI.3607-16.2017
Backstrom JR, Lim GP, Cullen MJ, Tokes ZA (1996) Matrix metalloproteinase-9 (MMP-9) is synthesized in neurons of the human hippocampus and is capable of degrading the amyloid-beta peptide (1-40). J Neurosci 16(24):7910–7919
Fragkouli A, Tsilibary EC, Tzinia AK (2014) Neuroprotective role of MMP-9 overexpression in the brain of Alzheimer’s 5xFAD mice. Neurobiol Dis 70:179–189. https://doi.org/10.1016/j.nbd.2014.06.021
Yan P, Hu X, Song H, Yin K, Bateman RJ, Cirrito JR, Xiao Q, Hsu FF, Turk JW, Xu J, Hsu CY, Holtzman DM, Lee JM (2006) Matrix metalloproteinase-9 degrades amyloid-beta fibrils in vitro and compact plaques in situ. J Biol Chem 281(34):24566–24574. https://doi.org/10.1074/jbc.M602440200
Hernandez-Guillamon M, Mawhirt S, Blais S, Montaner J, Neubert TA, Rostagno A, Ghiso J (2015) Sequential amyloid-beta degradation by the matrix metalloproteases MMP-2 and MMP-9. J Biol Chem 290(24):15078–15091. https://doi.org/10.1074/jbc.M114.610931
Yin KJ, Cirrito JR, Yan P, Hu X, Xiao Q, Pan X, Bateman R, Song H, Hsu FF, Turk J, Xu J, Hsu CY, Mills JC, Holtzman DM, Lee JM (2006) Matrix metalloproteinases expressed by astrocytes mediate extracellular amyloid-beta peptide catabolism. J Neurosci 26(43):10939–10948. https://doi.org/10.1523/JNEUROSCI.2085-06.2006
Moore KM, Girens RE, Larson SK, Jones MR, Restivo JL, Holtzman DM, Cirrito JR, Yuede CM, Zimmerman SD, Timson BF (2016) A spectrum of exercise training reduces soluble Abeta in a dose-dependent manner in a mouse model of Alzheimer’s disease. Neurobiol Dis 85:218–224. https://doi.org/10.1016/j.nbd.2015.11.004
White AR, Du T, Laughton KM, Volitakis I, Sharples RA, Xilinas ME, Hoke DE, Holsinger RM, Evin G, Cherny RA, Hill AF, Barnham KJ, Li QX, Bush AI, Masters CL (2006) Degradation of the Alzheimer disease amyloid beta-peptide by metal-dependent up-regulation of metalloprotease activity. J Biol Chem 281(26):17670–17680. https://doi.org/10.1074/jbc.M602487200
Taniguchi M, Matsuura K, Nakamura R, Kojima A, Konishi M, Akizawa T (2017) MMP-7 cleaves amyloid beta fragment peptides and copper ion inhibits the degradation. Biometals 30(5):797–807. https://doi.org/10.1007/s10534-017-0048-4
Liao MC, Van Nostrand WE (2010) Degradation of soluble and fibrillar amyloid beta-protein by matrix metalloproteinase (MT1-MMP) in vitro. Biochemistry 49(6):1127–1136. https://doi.org/10.1021/bi901994d
Montaner J, Ramiro L, Simats A, Hernández-Guillamon M, Delgado P, Bustamante A, Rosell A (2019) Matrix metalloproteinases and ADAMs in stroke. Cell Mol Life Sci. https://doi.org/10.1007/s00018-019-03175-5
Sweeney MD, Sagare AP, Zlokovic BV (2018) Blood-brain barrier breakdown in Alzheimer disease and other neurodegenerative disorders. Nat Rev Neurol 14(3):133–150. https://doi.org/10.1038/nrneurol.2017.188
Giannoni P, Arango-Lievano M, Neves ID, Rousset MC, Baranger K, Rivera S, Jeanneteau F, Claeysen S, Marchi N (2016) Cerebrovascular pathology during the progression of experimental Alzheimer’s disease. Neurobiol Dis 88:107–117. https://doi.org/10.1016/j.nbd.2016.01.001
Spampinato SF, Merlo S, Sano Y, Kanda T, Sortino MA (2017) Astrocytes contribute to Abeta-induced blood-brain barrier damage through activation of endothelial MMP9. J Neurochem 142(3):464–477. https://doi.org/10.1111/jnc.14068
Mazzitelli S, Filipello F, Rasile M, Lauranzano E, Starvaggi-Cucuzza C, Tamborini M, Pozzi D, Barajon I, Giorgino T, Natalello A, Matteoli M (2016) Amyloid-beta 1-24 C-terminal truncated fragment promotes amyloid-beta 1-42 aggregate formation in the healthy brain. Acta Neuropathol Comm 4(1):110. https://doi.org/10.1186/s40478-016-0381-9
Brkic M, Balusu S, Van Wonterghem E, Gorle N, Benilova I, Kremer A, Van Hove I, Moons L, De Strooper B, Kanazir S, Libert C, Vandenbroucke RE (2015) Amyloid beta oligomers disrupt blood-CSF barrier integrity by activating matrix metalloproteinases. J Neurosci 35(37):12766–12778. https://doi.org/10.1523/JNEUROSCI.0006-15.2015
Garcia-Alloza M, Prada C, Lattarulo C, Fine S, Borrelli LA, Betensky R, Greenberg SM, Frosch MP, Bacskai BJ (2009) Matrix metalloproteinase inhibition reduces oxidative stress associated with cerebral amyloid angiopathy in vivo in transgenic mice. J Neurochem 109(6):1636–1647. https://doi.org/10.1111/j.1471-4159.2009.06096.x
Prinz M, Priller J (2017) The role of peripheral immune cells in the CNS in steady state and disease. Nat Neurosci 20(2):136–144. https://doi.org/10.1038/nn.4475
Jhang KA, Lee EO, Kim HS, Chang KA, Suh YH, Chong YH (2016) S100A9 exacerbates the Abeta1-42-mediated innate immunity in human THP-1 monocytes. CNS Neurol Disord-DR 15(8):910–917
Achilli C, Ciana A, Minetti G (2014) Amyloid-beta (25-35) peptide induces the release of pro-matrix metalloprotease 9 (pro-MMP-9) from human neutrophils. Mol Cell Biochem 397(1–2):117–123. https://doi.org/10.1007/s11010-014-2178-0
Zenaro E, Pietronigro E, Della Bianca V, Piacentino G, Marongiu L, Budui S, Turano E, Rossi B, Angiari S, Dusi S, Montresor A, Carlucci T, Nani S, Tosadori G, Calciano L, Catalucci D, Berton G, Bonetti B, Constantin G (2015) Neutrophils promote Alzheimer’s disease-like pathology and cognitive decline via LFA-1 integrin. Nat Med 21(8):880–886. https://doi.org/10.1038/nm.3913
Deb S, Gottschall PE (1996) Increased production of matrix metalloproteinases in enriched astrocyte and mixed hippocampal cultures treated with beta-amyloid peptides. J Neurochem 66(4):1641–1647
Py NA, Bonnet AE, Bernard A, Marchalant Y, Charrat E, Checler F, Khrestchatisky M, Baranger K, Rivera S (2014) Differential spatio-temporal regulation of MMPs in the 5xFAD mouse model of Alzheimer’s disease: evidence for a pro-amyloidogenic role of MT1-MMP. Front Aging Neurosci 6:247. https://doi.org/10.3389/fnagi.2014.00247
Girard SD, Jacquet M, Baranger K, Migliorati M, Escoffier G, Bernard A, Khrestchatisky M, Feron F, Rivera S, Roman FS, Marchetti E (2014) Onset of hippocampus-dependent memory impairments in 5XFAD transgenic mouse model of Alzheimer’s disease. Hippocampus 24(7):762–772. https://doi.org/10.1002/hipo.22267
Seo JH, Guo S, Lok J, Navaratna D, Whalen MJ, Kim KW, Lo EH (2012) Neurovascular matrix metalloproteinases and the blood–brain barrier. Curr Pharm Design 18(25):3645–3648
Jourquin J, Tremblay E, Decanis N, Charton G, Hanessian S, Chollet AM, Le Diguardher T, Khrestchatisky M, Rivera S (2003) Neuronal activity-dependent increase of net matrix metalloproteinase activity is associated with MMP-9 neurotoxicity after kainate. Eur J Neurosci 18(6):1507–1517
Hernandez-Guillamon M, Mawhirt S, Fossati S, Blais S, Pares M, Penalba A, Boada M, Couraud PO, Neubert TA, Montaner J, Ghiso J, Rostagno A (2010) Matrix metalloproteinase 2 (MMP-2) degrades soluble vasculotropic amyloid-beta E22Q and L34V mutants, delaying their toxicity for human brain microvascular endothelial cells. J Biol Chem 285(35):27144–27158. https://doi.org/10.1074/jbc.M110.135228
Mizoguchi H, Takuma K, Fukuzaki E, Ibi D, Someya E, Akazawa KH, Alkam T, Tsunekawa H, Mouri A, Noda Y, Nabeshima T, Yamada K (2009) Matrix metalloprotease-9 inhibition improves amyloid beta-mediated cognitive impairment and neurotoxicity in mice. J Pharmacol Exp Ther 331(1):14–22. https://doi.org/10.1124/jpet.109.154724
Langenfurth A, Rinnenthal JL, Vinnakota K, Prinz V, Carlo AS, Stadelmann C, Siffrin V, Peaschke S, Endres M, Heppner F, Glass R, Wolf SA, Kettenmann H (2014) Membrane-type 1 metalloproteinase is upregulated in microglia/brain macrophages in neurodegenerative and neuroinflammatory diseases. J Neurosci Res 92(3):275–286. https://doi.org/10.1002/jnr.23288
Ito S, Koshikawa N, Mochizuki S, Takenaga K (2007) 3-Methyladenine suppresses cell migration and invasion of HT1080 fibrosarcoma cells through inhibiting phosphoinositide 3-kinases independently of autophagy inhibition. Int J Oncol 31(2):261–268
Ierusalimsky VN, Kuleshova EP, Balaban PM (2013) Expression of the type 1 metalloproteinase in the rat hippocampus after the intracerebroventricular injection of beta-amyloid peptide (25-35). Acta Neurobiol Exp 73(4):571–578
Jung SS, Zhang W, Van Nostrand WE (2003) Pathogenic A beta induces the expression and activation of matrix metalloproteinase-2 in human cerebrovascular smooth muscle cells. J Neurochem 85(5):1208–1215
Walker DG, Link J, Lue LF, Dalsing-Hernandez JE, Boyes BE (2006) Gene expression changes by amyloid beta peptide-stimulated human postmortem brain microglia identify activation of multiple inflammatory processes. J Leuk Biol 79(3):596–610. https://doi.org/10.1189/jlb.0705377
Leake A, Morris CM, Whateley J (2000) Brain matrix metalloproteinase 1 levels are elevated in Alzheimer’s disease. Neurosci Lett 291(3):201–203
Sekine-Aizawa Y, Hama E, Watanabe K, Tsubuki S, Kanai-Azuma M, Kanai Y, Arai H, Aizawa H, Iwata N, Saido TC (2001) Matrix metalloproteinase (MMP) system in brain: identification and characterization of brain-specific MMP highly expressed in cerebellum. Eur J Neurosci 13(5):935–948
Yoshiyama Y, Asahina M, Hattori T (2000) Selective distribution of matrix metalloproteinase-3 (MMP-3) in Alzheimer’s disease brain. Acta Neuropathol 99(2):91–95
Mroczko B, Groblewska M, Zboch M, Kulczynska A, Koper OM, Szmitkowski M, Kornhuber J, Lewczuk P (2014) Concentrations of matrix metalloproteinases and their tissue inhibitors in the cerebrospinal fluid of patients with Alzheimer’s disease. J Alzheimers Dis 40(2):351–357. https://doi.org/10.3233/JAD-131634
Horstmann S, Budig L, Gardner H, Koziol J, Deuschle M, Schilling C, Wagner S (2010) Matrix metalloproteinases in peripheral blood and cerebrospinal fluid in patients with Alzheimer’s disease. Int Psychogeriatr 22(6):966–972. https://doi.org/10.1017/S1041610210000827
Lorenzl S, Albers DS, Relkin N, Ngyuen T, Hilgenberg SL, Chirichigno J, Cudkowicz ME, Beal MF (2003) Increased plasma levels of matrix metalloproteinase-9 in patients with Alzheimer’s disease. Neurochem Int 43(3):191–196
Lorenzl S, Buerger K, Hampel H, Beal MF (2008) Profiles of matrix metalloproteinases and their inhibitors in plasma of patients with dementia. Int Psychogeriatr 20(1):67–76. https://doi.org/10.1017/S1041610207005790
Stomrud E, Bjorkqvist M, Janciauskiene S, Minthon L, Hansson O (2010) Alterations of matrix metalloproteinases in the healthy elderly with increased risk of prodromal Alzheimer’s disease. Alz Res Ther 2(3):20. https://doi.org/10.1186/alzrt44
Hanzel CE, Iulita MF, Eyjolfsdottir H, Hjorth E, Schultzberg M, Eriksdotter M, Cuello AC (2014) Analysis of matrix metallo-proteases and the plasminogen system in mild cognitive impairment and Alzheimer’s disease cerebrospinal fluid. J Alzheimers Dis 40(3):667–678. https://doi.org/10.3233/JAD-132282
Peng M, Jia J, Qin W (2015) Plasma gelsolin and matrix metalloproteinase 3 as potential biomarkers for Alzheimer disease. Neurosci Lett 595:116–121. https://doi.org/10.1016/j.neulet.2015.04.014
Selvais C, D’Auria L, Tyteca D, Perrot G, Lemoine P, Troeberg L, Dedieu S, Noel A, Nagase H, Henriet P, Courtoy PJ, Marbaix E, Emonard H (2011) Cell cholesterol modulates metalloproteinase-dependent shedding of low-density lipoprotein receptor-related protein-1 (LRP-1) and clearance function. FASEB J 25(8):2770–2781. https://doi.org/10.1096/fj.10-169508
Liu Q, Zhang J, Tran H, Verbeek MM, Reiss K, Estus S, Bu G (2009) LRP1 shedding in human brain: roles of ADAM10 and ADAM17. Mol Neurodegener 4:17. https://doi.org/10.1186/1750-1326-4-17
Raucci A, Cugusi S, Antonelli A, Barabino SM, Monti L, Bierhaus A, Reiss K, Saftig P, Bianchi ME (2008) A soluble form of the receptor for advanced glycation endproducts (RAGE) is produced by proteolytic cleavage of the membrane-bound form by the sheddase a disintegrin and metalloprotease 10 (ADAM10). FASEB J 22(10):3716–3727. https://doi.org/10.1096/fj.08-109033
Zhang L, Bukulin M, Kojro E, Roth A, Metz VV, Fahrenholz F, Nawroth PP, Bierhaus A, Postina R (2008) Receptor for advanced glycation end products is subjected to protein ectodomain shedding by metalloproteinases. J Biol Chem 283(51):35507–35516. https://doi.org/10.1074/jbc.M806948200
Metz VV, Kojro E, Rat D, Postina R (2012) Induction of RAGE shedding by activation of G protein-coupled receptors. PLoS One 7(7):e41823. https://doi.org/10.1371/journal.pone.0041823
Sagare A, Deane R, Bell RD, Johnson B, Hamm K, Pendu R, Marky A, Lenting PJ, Wu Z, Zarcone T, Goate A, Mayo K, Perlmutter D, Coma M, Zhong Z, Zlokovic BV (2007) Clearance of amyloid-beta by circulating lipoprotein receptors. Nat Med 13(9):1029–1031. https://doi.org/10.1038/nm1635
Terni B, Ferrer I (2015) Abnormal expression and distribution of MMP2 at initial stages of Alzheimer’s disease-related pathology. J Alzheimers Dis 46(2):461–469. https://doi.org/10.3233/JAD-142460
Nubling G, Levin J, Bader B, Israel L, Botzel K, Lorenzl S, Giese A (2012) Limited cleavage of tau with matrix-metalloproteinase MMP-9, but not MMP-3, enhances tau oligomer formation. Exp Neurol 237(2):470–476. https://doi.org/10.1016/j.expneurol.2012.07.018
Bjerke M, Zetterberg H, Edman A, Blennow K, Wallin A, Andreasson U (2011) Cerebrospinal fluid matrix metalloproteinases and tissue inhibitor of metalloproteinases in combination with subcortical and cortical biomarkers in vascular dementia and Alzheimer’s disease. J Alzheimers Dis 27(3):665–676. https://doi.org/10.3233/JAD-2011-110566
Higashi S, Miyazaki K (2003) Novel processing of beta-amyloid precursor protein catalyzed by membrane type 1 matrix metalloproteinase releases a fragment lacking the inhibitor domain against gelatinase A. Biochemistry 42(21):6514–6526. https://doi.org/10.1021/bi020643m
Miyazaki K, Hasegawa M, Funahashi K, Umeda M (1993) A metalloproteinase inhibitor domain in Alzheimer amyloid protein precursor. Nature 362(6423):839–841. https://doi.org/10.1038/362839a0
Ahmad M, Takino T, Miyamori H, Yoshizaki T, Furukawa M, Sato H (2006) Cleavage of amyloid-beta precursor protein (APP) by membrane-type matrix metalloproteinases. J Biochem 139(3):517–526. https://doi.org/10.1093/jb/mvj054
Willem M, Tahirovic S, Busche MA, Ovsepian SV, Chafai M, Kootar S, Hornburg D, Evans LD, Moore S, Daria A, Hampel H, Muller V, Giudici C, Nuscher B, Wenninger-Weinzierl A, Kremmer E, Heneka MT, Thal DR, Giedraitis V, Lannfelt L, Muller U, Livesey FJ, Meissner F, Herms J, Konnerth A, Marie H, Haass C (2015) eta-Secretase processing of APP inhibits neuronal activity in the hippocampus. Nature 526(7573):443–447. https://doi.org/10.1038/nature14864
Oakley H, Cole SL, Logan S, Maus E, Shao P, Craft J, Guillozet-Bongaarts A, Ohno M, Disterhoft J, Van Eldik L, Berry R, Vassar R (2006) Intraneuronal beta-amyloid aggregates, neurodegeneration, and neuron loss in transgenic mice with five familial Alzheimer’s disease mutations: potential factors in amyloid plaque formation. J Neurosci 26(40):10129–10140. https://doi.org/10.1523/JNEUROSCI.1202-06.2006
Komori K, Nonaka T, Okada A, Kinoh H, Hayashita-Kinoh H, Yoshida N, Yana I, Seiki M (2004) Absence of mechanical allodynia and Abeta-fiber sprouting after sciatic nerve injury in mice lacking membrane-type 5 matrix metalloproteinase. FEBS Lett 557(1–3):125–128
Baranger K, Marchalant Y, Bonnet AE, Crouzin N, Carrete A, Paumier JM, Py NA, Bernard A, Bauer C, Charrat E, Moschke K, Seiki M, Vignes M, Lichtenthaler SF, Checler F, Khrestchatisky M, Rivera S (2016) MT5-MMP is a new pro-amyloidogenic proteinase that promotes amyloid pathology and cognitive decline in a transgenic mouse model of Alzheimer’s disease. Cell Mol Life Sci 73(1):217–236. https://doi.org/10.1007/s00018-015-1992-1
Baranger K, Bonnet AE, Girard SD, Paumier JM, Garcia-Gonzalez L, Elmanaa W, Bernard A, Charrat E, Stephan D, Bauer C, Moschke K, Lichtenthaler SF, Roman FS, Checler F, Khrestchatisky M, Rivera S (2017) MT5-MMP Promotes Alzheimer’s Pathogenesis in the Frontal Cortex of 5xFAD Mice and APP Trafficking in vitro. Front Mol Neurosci 9:163. https://doi.org/10.3389/fnmol.2016.00163
Kimura R, Ohno M (2009) Impairments in remote memory stabilization precede hippocampal synaptic and cognitive failures in 5XFAD Alzheimer mouse model. Neurobiol Dis 33(2):229–235. https://doi.org/10.1016/j.nbd.2008.10.006
Crouzin N, Baranger K, Cavalier M, Marchalant Y, Cohen-Solal C, Roman FS, Khrestchatisky M, Rivera S, Feron F, Vignes M (2013) Area-specific alterations of synaptic plasticity in the 5XFAD mouse model of Alzheimer’s disease: dissociation between somatosensory cortex and hippocampus. PLoS One 8(9):e74667. https://doi.org/10.1371/journal.pone.0074667
Jawhar S, Trawicka A, Jenneckens C, Bayer TA, Wirths O (2012) Motor deficits, neuron loss, and reduced anxiety coinciding with axonal degeneration and intraneuronal Abeta aggregation in the 5XFAD mouse model of Alzheimer’s disease. Neurobiol Aging 33(1):196. https://doi.org/10.1016/j.neurobiolaging.2010.05.027
Girard SD, Baranger K, Gauthier C, Jacquet M, Bernard A, Escoffier G, Marchetti E, Khrestchatisky M, Rivera S, Roman FS (2013) Evidence for early cognitive impairment related to frontal cortex in the 5XFAD mouse model of Alzheimer’s disease. J Alzheimers Dis 33(3):781–796. https://doi.org/10.3233/JAD-2012-120982
Baranger K, Giannoni P, Girard SD, Girot S, Gaven F, Stephan D, Migliorati M, Khrestchatisky M, Bockaert J, Marchetti-Gauthier E, Rivera S, Claeysen S, Roman FS (2017) Chronic treatments with a 5-HT4 receptor agonist decrease amyloid pathology in the entorhinal cortex and learning and memory deficits in the 5xFAD mouse model of Alzheimer’s disease. Neuropharmacology 126:128–141. https://doi.org/10.1016/j.neuropharm.2017.08.031
Wang P, Wang X, Pei D (2004) Mint-3 regulates the retrieval of the internalized membrane-type matrix metalloproteinase, MT5-MMP, to the plasma membrane by binding to its carboxyl end motif EWV. J Biol Chem 279(19):20461–20470. https://doi.org/10.1074/jbc.M400264200
Laulagnier K, Javalet C, Hemming FJ, Chivet M, Lachenal G, Blot B, Chatellard C, Sadoul R (2018) Amyloid precursor protein products concentrate in a subset of exosomes specifically endocytosed by neurons. Cell Mol Life Sci 75(4):757–773. https://doi.org/10.1007/s00018-017-2664-0
Zhang Z, Song M, Liu X, Su Kang S, Duong DM, Seyfried NT, Cao X, Cheng L, Sun YE, Ping YuS, Jia J, Levey AI, Ye K (2015) Delta-secretase cleaves amyloid precursor protein and regulates the pathogenesis in Alzheimer’s disease. Nat Comm 6:8762. https://doi.org/10.1038/ncomms9762
Paumier JM, Py NA, Garcia-Gonzalez L, Bernard A, Stephan D, Louis L, Checler F, Khrestchatisky M, Baranger K, Rivera S (2018) Proamyloidogenic effects of membrane type 1 matrix metalloproteinase involve MMP-2 and BACE-1 activities, and the modulation of APP trafficking. FASEB J. https://doi.org/10.1096/fj.201801076r
Uekita T, Itoh Y, Yana I, Ohno H, Seiki M (2001) Cytoplasmic tail-dependent internalization of membrane-type 1 matrix metalloproteinase is important for its invasion-promoting activity. J Cell Biol 155(7):1345–1356. https://doi.org/10.1083/jcb.200108112
Perez RG, Soriano S, Hayes JD, Ostaszewski B, Xia W, Selkoe DJ, Chen X, Stokin GB, Koo EH (1999) Mutagenesis identifies new signals for beta-amyloid precursor protein endocytosis, turnover, and the generation of secreted fragments, including Abeta42. J Biol Chem 274(27):18851–18856
Caster AH, Kahn RA (2013) Recruitment of the Mint3 adaptor is necessary for export of the amyloid precursor protein (APP) from the Golgi complex. J Biol Chem 288(40):28567–28580. https://doi.org/10.1074/jbc.M113.481101
Vincent B, Checler F (2012) alpha-Secretase in Alzheimer’s disease and beyond: mechanistic, regulation and function in the shedding of membrane proteins. Curr Alz Res 9(2):140–156
Saftig P, Lichtenthaler SF (2015) The alpha secretase ADAM10: a metalloprotease with multiple functions in the brain. Prog Neurobiol 135:1–20. https://doi.org/10.1016/j.pneurobio.2015.10.003
Letronne F, Laumet G, Ayral AM, Chapuis J, Demiautte F, Laga M, Vandenberghe ME, Malmanche N, Leroux F, Eysert F, Sottejeau Y, Chami L, Flaig A, Bauer C, Dourlen P, Lesaffre M, Delay C, Huot L, Dumont J, Werkmeister E, Lafont F, Mendes T, Hansmannel F, Dermaut B, Deprez B, Herard AS, Dhenain M, Souedet N, Pasquier F, Tulasne D, Berr C, Hauw JJ, Lemoine Y, Amouyel P, Mann D, Deprez R, Checler F, Hot D, Delzescaux T, Gevaert K, Lambert JC (2016) ADAM30 Downregulates APP-Linked defects through cathepsin D activation in Alzheimer’s disease. EBioMedicine 9:278–292. https://doi.org/10.1016/j.ebiom.2016.06.002
Kleinberger G, Yamanishi Y, Suarez-Calvet M, Czirr E, Lohmann E, Cuyvers E, Struyfs H, Pettkus N, Wenninger-Weinzierl A, Mazaheri F, Tahirovic S, Lleo A, Alcolea D, Fortea J, Willem M, Lammich S, Molinuevo JL, Sanchez-Valle R, Antonell A, Ramirez A, Heneka MT, Sleegers K, van der Zee J, Martin JJ, Engelborghs S, Demirtas-Tatlidede A, Zetterberg H, Van Broeckhoven C, Gurvit H, Wyss-Coray T, Hardy J, Colonna M, Haass C (2014) TREM2 mutations implicated in neurodegeneration impair cell surface transport and phagocytosis. Sci Transl Med 6(243):243ra286. https://doi.org/10.1126/scitranslmed.3009093
Thornton P, Sevalle J, Deery MJ, Fraser G, Zhou Y, Stahl S, Franssen EH, Dodd RB, Qamar S, Gomez Perez-Nievas B, Nicol LS, Eketjall S, Revell J, Jones C, Billinton A, St George-Hyslop PH, Chessell I, Crowther DC (2017) TREM2 shedding by cleavage at the H157-S158 bond is accelerated for the Alzheimer’s disease-associated H157Y variant. EMBO Mol Med 9(10):1366–1378. https://doi.org/10.15252/emmm.201707673
Feuerbach D, Schindler P, Barske C, Joller S, Beng-Louka E, Worringer KA, Kommineni S, Kaykas A, Ho DJ, Ye C, Welzenbach K, Elain G, Klein L, Brzak I, Mir AK, Farady CJ, Aichholz R, Popp S, George N, Neumann U (2017) ADAM17 is the main sheddase for the generation of human triggering receptor expressed in myeloid cells (hTREM2) ectodomain and cleaves TREM2 after Histidine 157. Neurosci Lett 660:109–114. https://doi.org/10.1016/j.neulet.2017.09.034
Carmona S, Zahs K, Wu E, Dakin K, Bras J, Guerreiro R (2018) The role of TREM2 in Alzheimer’s disease and other neurodegenerative disorders. Lancet Neurol 17(8):721–730. https://doi.org/10.1016/S1474-4422(18)30232-1
Black RA, Rauch CT, Kozlosky CJ, Peschon JJ, Slack JL, Wolfson MF, Castner BJ, Stocking KL, Reddy P, Srinivasan S, Nelson N, Boiani N, Schooley KA, Gerhart M, Davis R, Fitzner JN, Johnson RS, Paxton RJ, March CJ, Cerretti DP (1997) A metalloproteinase disintegrin that releases tumour-necrosis factor-alpha from cells. Nature 385(6618):729–733. https://doi.org/10.1038/385729a0
Decourt B, Lahiri DK, Sabbagh MN (2017) Targeting tumor necrosis factor alpha for Alzheimer’s disease. Curr Alz Res 14(4):412–425. https://doi.org/10.2174/1567205013666160930110551
Peress N, Perillo E, Zucker S (1995) Localization of tissue inhibitor of matrix metalloproteinases in Alzheimer’s disease and normal brain. J Neuropathol Exp Neurol 54(1):16–22
Lorenzl S, Albers DS, LeWitt PA, Chirichigno JW, Hilgenberg SL, Cudkowicz ME, Beal MF (2003) Tissue inhibitors of matrix metalloproteinases are elevated in cerebrospinal fluid of neurodegenerative diseases. J Neurol Sci 207(1–2):71–76
Marksteiner J, Imarhiagbe D, Defrancesco M, Deisenhammer EA, Kemmler G, Humpel C (2014) Analysis of 27 vascular-related proteins reveals that NT-proBNP is a potential biomarker for Alzheimer’s disease and mild cognitive impairment: a pilot-study. Exp Gerontol 50:114–121. https://doi.org/10.1016/j.exger.2013.12.001
Ridnour LA, Dhanapal S, Hoos M, Wilson J, Lee J, Cheng RY, Brueggemann EE, Hines HB, Wilcock DM, Vitek MP, Wink DA, Colton CA (2012) Nitric oxide-mediated regulation of beta-amyloid clearance via alterations of MMP-9/TIMP-1. J Neurochem 123(5):736–749. https://doi.org/10.1111/jnc.12028
Duits FH, Hernandez-Guillamon M, Montaner J, Goos JD, Montanola A, Wattjes MP, Barkhof F, Scheltens P, Teunissen CE, van der Flier WM (2015) Matrix metalloproteinases in Alzheimer’s disease and concurrent cerebral microbleeds. J Alzheimers Dis 48(3):711–720. https://doi.org/10.3233/JAD-143186
Hernandez-Guillamon M, Delgado P, Ortega L, Pares M, Rosell A, Garcia-Bonilla L, Fernandez-Cadenas I, Borrell-Pages M, Boada M, Montaner J (2009) Neuronal TIMP-1 release accompanies astrocytic MMP-9 secretion and enhances astrocyte proliferation induced by beta-amyloid 25-35 fragment. J Neurosci Res 87(9):2115–2125. https://doi.org/10.1002/jnr.22034
Ogier C, Creidy R, Boucraut J, Soloway PD, Khrestchatisky M, Rivera S (2005) Astrocyte reactivity to Fas activation is attenuated in TIMP-1 deficient mice, an in vitro study. BMC Neurosci 6:68. https://doi.org/10.1186/1471-2202-6-68
Thirumangalakudi L, Samany PG, Owoso A, Wiskar B, Grammas P (2006) Angiogenic proteins are expressed by brain blood vessels in Alzheimer’s disease. J Alzheimers Dis 10(1):111–118
Park SK, Hwang YS, Park KK, Park HJ, Seo JY, Chung WY (2009) Kalopanaxsaponin A inhibits PMA-induced invasion by reducing matrix metalloproteinase-9 via PI3K/Akt- and PKCdelta-mediated signaling in MCF-7 human breast cancer cells. Carcinogenesis 30(7):1225–1233. https://doi.org/10.1093/carcin/bgp111
Castellano JM, Mosher KI, Abbey RJ, McBride AA, James ML, Berdnik D, Shen JC, Zou B, Xie XS, Tingle M, Hinkson IV, Angst MS, Wyss-Coray T (2017) Human umbilical cord plasma proteins revitalize hippocampal function in aged mice. Nature 544(7651):488–492. https://doi.org/10.1038/nature22067
Hoe HS, Cooper MJ, Burns MP, Lewis PA, van der Brug M, Chakraborty G, Cartagena CM, Pak DT, Cookson MR, Rebeck GW (2007) The metalloprotease inhibitor TIMP-3 regulates amyloid precursor protein and apolipoprotein E receptor proteolysis. J Neurosci 27(40):10895–10905. https://doi.org/10.1523/JNEUROSCI.3135-07.2007
Dunckley T, Beach TG, Ramsey KE, Grover A, Mastroeni D, Walker DG, LaFleur BJ, Coon KD, Brown KM, Caselli R, Kukull W, Higdon R, McKeel D, Morris JC, Hulette C, Schmechel D, Reiman EM, Rogers J, Stephan DA (2006) Gene expression correlates of neurofibrillary tangles in Alzheimer’s disease. Neurobiol Aging 27(10):1359–1371. https://doi.org/10.1016/j.neurobiolaging.2005.08.013
Qin W, Jia X, Wang F, Zuo X, Wu L, Zhou A, Li D, Min B, Wei C, Tang Y, Xing Y, Dong X, Wang Q, Gao Y, Li Y, Jia J (2015) Elevated plasma angiogenesis factors in Alzheimer’s disease. J Alzheimers Dis 45(1):245–252. https://doi.org/10.3233/JAD-142409
Polymeropoulos MH, Lavedan C, Leroy E, Ide SE, Dehejia A, Dutra A, Pike B, Root H, Rubenstein J, Boyer R, Stenroos ES, Chandrasekharappa S, Athanassiadou A, Papapetropoulos T, Johnson WG, Lazzarini AM, Duvoisin RC, Di Iorio G, Golbe LI, Nussbaum RL (1997) Mutation in the alpha-synuclein gene identified in families with Parkinson’s disease. Science 276(5321):2045–2047
Kruger R, Kuhn W, Muller T, Woitalla D, Graeber M, Kosel S, Przuntek H, Epplen JT, Schols L, Riess O (1998) Ala30Pro mutation in the gene encoding alpha-synuclein in Parkinson’s disease. Nat Genet 18(2):106–108. https://doi.org/10.1038/ng0298-106
Singleton AB, Farrer M, Johnson J, Singleton A, Hague S, Kachergus J, Hulihan M, Peuralinna T, Dutra A, Nussbaum R, Lincoln S, Crawley A, Hanson M, Maraganore D, Adler C, Cookson MR, Muenter M, Baptista M, Miller D, Blancato J, Hardy J, Gwinn-Hardy K (2003) alpha-Synuclein locus triplication causes Parkinson’s disease. Science 302(5646):841. https://doi.org/10.1126/science.1090278
Chartier-Harlin MC, Kachergus J, Roumier C, Mouroux V, Douay X, Lincoln S, Levecque C, Larvor L, Andrieux J, Hulihan M, Waucquier N, Defebvre L, Amouyel P, Farrer M, Destee A (2004) Alpha-synuclein locus duplication as a cause of familial Parkinson’s disease. Lancet 364(9440):1167–1169. https://doi.org/10.1016/S0140-6736(04)17103-1
Zarranz JJ, Alegre J, Gomez-Esteban JC, Lezcano E, Ros R, Ampuero I, Vidal L, Hoenicka J, Rodriguez O, Atares B, Llorens V, Gomez Tortosa E, del Ser T, Munoz DG, de Yebenes JG (2004) The new mutation, E46K, of alpha-synuclein causes Parkinson and Lewy body dementia. Ann Neurol 55(2):164–173. https://doi.org/10.1002/ana.10795
Ghosh D, Mehra S, Sahay S, Singh PK, Maji SK (2017) alpha-synuclein aggregation and its modulation. Int J Biol Macromol 100:37–54. https://doi.org/10.1016/j.ijbiomac.2016.10.021
Longhena F, Faustini G, Missale C, Pizzi M, Spano P, Bellucci A (2017) The contribution of alpha-synuclein spreading to Parkinson’s disease synaptopathy. Neural Plast 2017:5012129. https://doi.org/10.1155/2017/5012129
Olanow CW, Brundin P (2013) Parkinson’s disease and alpha synuclein: is Parkinson’s disease a prion-like disorder? Mov Dis 28(1):31–40. https://doi.org/10.1002/mds.25373
Wakabayashi K, Tanji K, Odagiri S, Miki Y, Mori F, Takahashi H (2013) The Lewy body in Parkinson’s disease and related neurodegenerative disorders. Mol Neurobiol 47(2):495–508. https://doi.org/10.1007/s12035-012-8280-y
Milber JM, Noorigian JV, Morley JF, Petrovitch H, White L, Ross GW, Duda JE (2012) Lewy pathology is not the first sign of degeneration in vulnerable neurons in Parkinson disease. Neurology 79(24):2307–2314. https://doi.org/10.1212/WNL.0b013e318278fe32
Ding TT, Lee SJ, Rochet JC, Lansbury PT Jr (2002) Annular alpha-synuclein protofibrils are produced when spherical protofibrils are incubated in solution or bound to brain-derived membranes. Biochemistry 41(32):10209–10217
Lashuel HA, Hartley D, Petre BM, Walz T, Lansbury PT Jr (2002) Neurodegenerative disease: amyloid pores from pathogenic mutations. Nature 418(6895):291. https://doi.org/10.1038/418291a
Lashuel HA, Petre BM, Wall J, Simon M, Nowak RJ, Walz T, Lansbury PT Jr (2002) Alpha-synuclein, especially the Parkinson’s disease-associated mutants, forms pore-like annular and tubular protofibrils. J Mol Biol 322(5):1089–1102
Baba M, Nakajo S, Tu PH, Tomita T, Nakaya K, Lee VM, Trojanowski JQ, Iwatsubo T (1998) Aggregation of alpha-synuclein in Lewy bodies of sporadic Parkinson’s disease and dementia with Lewy bodies. Am J Pathol 152(4):879–884
Lee MK, Stirling W, Xu Y, Xu X, Qui D, Mandir AS, Dawson TM, Copeland NG, Jenkins NA, Price DL (2002) Human alpha-synuclein-harboring familial Parkinson’s disease-linked Ala-53 –> Thr mutation causes neurodegenerative disease with alpha-synuclein aggregation in transgenic mice. Proc Natl Acad Sci USA 99(13):8968–8973. https://doi.org/10.1073/pnas.132197599
Choi DH, Kim YJ, Kim YG, Joh TH, Beal MF, Kim YS (2011) Role of matrix metalloproteinase 3-mediated alpha-synuclein cleavage in dopaminergic cell death. J Biol Chem 286(16):14168–14177. https://doi.org/10.1074/jbc.M111.222430
Crowther RA, Jakes R, Spillantini MG, Goedert M (1998) Synthetic filaments assembled from C-terminally truncated alpha-synuclein. FEBS Lett 436(3):309–312
Kanda S, Bishop JF, Eglitis MA, Yang Y, Mouradian MM (2000) Enhanced vulnerability to oxidative stress by alpha-synuclein mutations and C-terminal truncation. Neuroscience 97(2):279–284
Sung JY, Park SM, Lee CH, Um JW, Lee HJ, Kim J, Oh YJ, Lee ST, Paik SR, Chung KC (2005) Proteolytic cleavage of extracellular secreted {alpha}-synuclein via matrix metalloproteinases. J Biol Chem 280(26):25216–25224. https://doi.org/10.1074/jbc.M503341200
Levin J, Giese A, Boetzel K, Israel L, Hogen T, Nubling G, Kretzschmar H, Lorenzl S (2009) Increased alpha-synuclein aggregation following limited cleavage by certain matrix metalloproteinases. Exp Neurol 215(1):201–208. https://doi.org/10.1016/j.expneurol.2008.10.010
Kim YS, Choi DH, Block ML, Lorenzl S, Yang L, Kim YJ, Sugama S, Cho BP, Hwang O, Browne SE, Kim SY, Hong JS, Beal MF, Joh TH (2007) A pivotal role of matrix metalloproteinase-3 activity in dopaminergic neuronal degeneration via microglial activation. FASEB J 21(1):179–187. https://doi.org/10.1096/fj.06-5865com
Chung YC, Kim YS, Bok E, Yune TY, Maeng S, Jin BK (2013) MMP-3 contributes to nigrostriatal dopaminergic neuronal loss, BBB damage, and neuroinflammation in an MPTP mouse model of Parkinson’s disease. Mediat Inflamm 2013:370526. https://doi.org/10.1155/2013/370526
Choi DH, Kim EM, Son HJ, Joh TH, Kim YS, Kim D, Flint Beal M, Hwang O (2008) A novel intracellular role of matrix metalloproteinase-3 during apoptosis of dopaminergic cells. J Neurochem 106(1):405–415. https://doi.org/10.1111/j.1471-4159.2008.05399.x
Kim YS, Kim SS, Cho JJ, Choi DH, Hwang O, Shin DH, Chun HS, Beal MF, Joh TH (2005) Matrix metalloproteinase-3: a novel signaling proteinase from apoptotic neuronal cells that activates microglia. J Neurosci 25(14):3701–3711. https://doi.org/10.1523/JNEUROSCI.4346-04.2005
Lee EJ, Woo MS, Moon PG, Baek MC, Choi IY, Kim WK, Junn E, Kim HS (2010) Alpha-synuclein activates microglia by inducing the expressions of matrix metalloproteinases and the subsequent activation of protease-activated receptor-1. J Immunol 185(1):615–623. https://doi.org/10.4049/jimmunol.0903480
Bonifati V, Rizzu P, van Baren MJ, Schaap O, Breedveld GJ, Krieger E, Dekker MC, Squitieri F, Ibanez P, Joosse M, van Dongen JW, Vanacore N, van Swieten JC, Brice A, Meco G, van Duijn CM, Oostra BA, Heutink P (2003) Mutations in the DJ-1 gene associated with autosomal recessive early-onset parkinsonism. Science 299(5604):256–259. https://doi.org/10.1126/science.1077209
Choi DH, Hwang O, Lee KH, Lee J, Beal MF, Kim YS (2011) DJ-1 cleavage by matrix metalloproteinase 3 mediates oxidative stress-induced dopaminergic cell death. Antiox Redox Sign 14(11):2137–2150. https://doi.org/10.1089/ars.2009.3059
Miller DW, Ahmad R, Hague S, Baptista MJ, Canet-Aviles R, McLendon C, Carter DM, Zhu PP, Stadler J, Chandran J, Klinefelter GR, Blackstone C, Cookson MR (2003) L166P mutant DJ-1, causative for recessive Parkinson’s disease, is degraded through the ubiquitin-proteasome system. J Biol Chem 278(38):36588–36595. https://doi.org/10.1074/jbc.M304272200
Kim YS, Joh TH (2012) Matrix metalloproteinases, new insights into the understanding of neurodegenerative disorders. Biomol Ther 20(2):133–143. https://doi.org/10.4062/biomolther.2012.20.2.133
Shendelman S, Jonason A, Martinat C, Leete T, Abeliovich A (2004) DJ-1 is a redox-dependent molecular chaperone that inhibits alpha-synuclein aggregate formation. PLoS Biol 2(11):e362. https://doi.org/10.1371/journal.pbio.0020362
Butler GS, Dean RA, Tam EM, Overall CM (2008) Pharmacoproteomics of a metalloproteinase hydroxamate inhibitor in breast cancer cells: dynamics of membrane type 1 matrix metalloproteinase-mediated membrane protein shedding. Mol Cell Biol 28(15):4896–4914. https://doi.org/10.1128/MCB.01775-07
Joo SH, Kwon KJ, Kim JW, Kim JW, Hasan MR, Lee HJ, Han SH, Shin CY (2010) Regulation of matrix metalloproteinase-9 and tissue plasminogen activator activity by alpha-synuclein in rat primary glial cells. Neurosci Lett 469(3):352–356. https://doi.org/10.1016/j.neulet.2009.12.026
Kim S, Cho SH, Kim KY, Shin KY, Kim HS, Park CH, Chang KA, Lee SH, Cho D, Suh YH (2009) Alpha-synuclein induces migration of BV-2 microglial cells by up-regulation of CD44 and MT1-MMP. J Neurochem 109(5):1483–1496. https://doi.org/10.1111/j.1471-4159.2009.06075.x
Paisan-Ruiz C, Jain S, Evans EW, Gilks WP, Simon J, van der Brug M, Lopez de Munain A, Aparicio S, Gil AM, Khan N, Johnson J, Martinez JR, Nicholl D, Carrera IM, Pena AS, de Silva R, Lees A, Marti-Masso JF, Perez-Tur J, Wood NW, Singleton AB (2004) Cloning of the gene containing mutations that cause PARK8-linked Parkinson’s disease. Neuron 44(4):595–600. https://doi.org/10.1016/j.neuron.2004.10.023
Cookson MR (2010) The role of leucine-rich repeat kinase 2 (LRRK2) in Parkinson’s disease. Nat Rev Neurosci 11(12):791–797. https://doi.org/10.1038/nrn2935
Caesar M, Felk S, Zach S, Bronstad G, Aasly JO, Gasser T, Gillardon F (2014) Changes in matrix metalloprotease activity and progranulin levels may contribute to the pathophysiological function of mutant leucine-rich repeat kinase 2. Glia 62(7):1075–1092. https://doi.org/10.1002/glia.22663
Suh HS, Choi N, Tarassishin L, Lee SC (2012) Regulation of progranulin expression in human microglia and proteolysis of progranulin by matrix metalloproteinase-12 (MMP-12). PLoS One 7(4):e35115. https://doi.org/10.1371/journal.pone.0035115
Bachiller S, Jimenez-Ferrer I, Paulus A, Yang Y, Swanberg M, Deierborg T, Boza-Serrano A (2018) Microglia in neurological diseases: a road map to brain-disease dependent-inflammatory response. Front Cell Neurosci 12:488. https://doi.org/10.3389/fncel.2018.00488
Oh SH, Kim HN, Park HJ, Shin JY, Kim DY, Lee PH (2017) The cleavage effect of mesenchymal stem cell and its derived matrix metalloproteinase-2 on extracellular alpha-synuclein aggregates in Parkinsonian models. Stem Cells Translat Med 6(3):949–961. https://doi.org/10.5966/sctm.2016-0111
Lorenzl S, Albers DS, Narr S, Chirichigno J, Beal MF (2002) Expression of MMP-2, MMP-9, and MMP-1 and their endogenous counterregulators TIMP-1 and TIMP-2 in postmortem brain tissue of Parkinson’s disease. Exp Neurol 178(1):13–20
Kim SY, Woo MS, Park JS, Hyun JW, Kim YS, Kim HS (2010) The neuroprotective role of tissue inhibitor of metalloproteinase-2 in MPP+- or 6-OHDA-treated SK-N-BE(2)C and SH-SY5Y human neuroblastoma cells. Neurosci Lett 468(2):136–140. https://doi.org/10.1016/j.neulet.2009.10.084
Kim J, Jeong YH, Lee EJ, Park JS, Seo H, Kim HS (2017) Suppression of neuroinflammation by matrix metalloproteinase-8 inhibitor in aged normal and LRRK2 G2019S Parkinson’s disease model mice challenged with lipopolysaccharide. Biochem Biophys Res Comm 493(2):879–886. https://doi.org/10.1016/j.bbrc.2017.09.129
Lorenzl S, Calingasan N, Yang L, Albers DS, Shugama S, Gregorio J, Krell HW, Chirichigno J, Joh T, Beal MF (2004) Matrix metalloproteinase-9 is elevated in 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine-induced parkinsonism in mice. Neuromol Med 5(2):119–132. https://doi.org/10.1385/nmm:5:2:119
Logroscino G, Tortelli R, Rizzo G, Marin B, Preux P, Malaspina A (2015) Amyotrophic lateral sclerosis: an aging-related disease. Curr Geri Rep 4:142. https://doi.org/10.1007/s13670-015-0127-8
Lukaszewicz-Zajac M, Mroczko B, Slowik A (2014) Matrix metalloproteinases (MMPs) and their tissue inhibitors (TIMPs) in amyotrophic lateral sclerosis (ALS). J Neural Trans 121(11):1387–1397. https://doi.org/10.1007/s00702-014-1205-3
Dewil M, Schurmans C, Starckx S, Opdenakker G, Van Den Bosch L, Robberecht W (2005) Role of matrix metalloproteinase-9 in a mouse model for amyotrophic lateral sclerosis. NeuroReport 16(4):321–324
Kiaei M, Kipiani K, Calingasan NY, Wille E, Chen J, Heissig B, Rafii S, Lorenzl S, Beal MF (2007) Matrix metalloproteinase-9 regulates TNF-alpha and FasL expression in neuronal, glial cells and its absence extends life in a transgenic mouse model of amyotrophic lateral sclerosis. Exp Neurol 205(1):74–81. https://doi.org/10.1016/j.expneurol.2007.01.036
Kaplan A, Spiller KJ, Towne C, Kanning KC, Choe GT, Geber A, Akay T, Aebischer P, Henderson CE (2014) Neuronal matrix metalloproteinase-9 is a determinant of selective neurodegeneration. Neuron 81(2):333–348. https://doi.org/10.1016/j.neuron.2013.12.009
Morisaki Y, Niikura M, Watanabe M, Onishi K, Tanabe S, Moriwaki Y, Okuda T, Ohara S, Murayama S, Takao M, Uchida S, Yamanaka K, Misawa H (2016) Selective expression of osteopontin in ALS-resistant motor neurons is a critical determinant of late phase neurodegeneration mediated by matrix metalloproteinase-9. Sci Rep 6:27354. https://doi.org/10.1038/srep27354
Lorenzl S, Narr S, Angele B, Krell HW, Gregorio J, Kiaei M, Pfister HW, Beal MF (2006) The matrix metalloproteinases inhibitor Ro 28-2653 [correction of Ro 26-2853] extends survival in transgenic ALS mice. Exp Neurol 200(1):166–171. https://doi.org/10.1016/j.expneurol.2006.01.026
Vaz AR, Cunha C, Gomes C, Schmucki N, Barbosa M, Brites D (2015) Glycoursodeoxycholic acid reduces matrix metalloproteinase-9 and caspase-9 activation in a cellular model of superoxide dismutase-1 neurodegeneration. Mol Neurobiol 51(3):864–877. https://doi.org/10.1007/s12035-014-8731-8
Spiller KJ, Khan T, Dominique MA, Restrepo CR, Cotton-Samuel D, Levitan M, Jafar-Nejad P, Zhang B, Soriano A, Rigo F, Trojanowski JQ, Lee VM (2019) Reduction of matrix metalloproteinase 9 (MMP-9) protects motor neurons from TDP-43-triggered death in rNLS8 mice. Neurobiol Dis 124:133–140. https://doi.org/10.1016/j.nbd.2018.11.013
Soon CP, Crouch PJ, Turner BJ, McLean CA, Laughton KM, Atkin JD, Masters CL, White AR, Li QX (2010) Serum matrix metalloproteinase-9 activity is dysregulated with disease progression in the mutant SOD1 transgenic mice. Neuromusc Disord 20(4):260–266. https://doi.org/10.1016/j.nmd.2009.11.015
Izrael M, Slutsky SG, Admoni T, Cohen L, Granit A, Hasson A, Itskovitz-Eldor J, Krush Paker L, Kuperstein G, Lavon N, Yehezkel Ionescu S, Solmesky LJ, Zaguri R, Zhuravlev A, Volman E, Chebath J, Revel M (2018) Safety and efficacy of human embryonic stem cell-derived astrocytes following intrathecal transplantation in SOD1(G93A) and NSG animal models. Stem Cell Res Ther 9(1):152. https://doi.org/10.1186/s13287-018-0890-5
Lee JK, Shin JH, Suh J, Choi IS, Ryu KS, Gwag BJ (2008) Tissue inhibitor of metalloproteinases-3 (TIMP-3) expression is increased during serum deprivation-induced neuronal apoptosis in vitro and in the G93A mouse model of amyotrophic lateral sclerosis: a potential modulator of Fas-mediated apoptosis. Neurobiol Dis 30(2):174–185. https://doi.org/10.1016/j.nbd.2008.01.004
Lim GP, Backstrom JR, Cullen MJ, Miller CA, Atkinson RD, Tokes ZA (1996) Matrix metalloproteinases in the neocortex and spinal cord of amyotrophic lateral sclerosis patients. J Neurochem 67(1):251–259
Beuche W, Yushchenko M, Mader M, Maliszewska M, Felgenhauer K, Weber F (2000) Matrix metalloproteinase-9 is elevated in serum of patients with amyotrophic lateral sclerosis. NeuroReport 11(16):3419–3422
Fang L, Huber-Abel F, Teuchert M, Hendrich C, Dorst J, Schattauer D, Zettlmeissel H, Wlaschek M, Scharffetter-Kochanek K, Tumani H, Ludolph AC, Brettschneider J (2009) Linking neuron and skin: matrix metalloproteinases in amyotrophic lateral sclerosis (ALS). J Neurol Sci 285(1–2):62–66. https://doi.org/10.1016/j.jns.2009.05.025
Niebroj-Dobosz I, Janik P, Sokolowska B, Kwiecinski H (2010) Matrix metalloproteinases and their tissue inhibitors in serum and cerebrospinal fluid of patients with amyotrophic lateral sclerosis. Eur J Neurol 17(2):226–231. https://doi.org/10.1111/j.1468-1331.2009.02775.x
Liu Y, Hao W, Dawson A, Liu S, Fassbender K (2009) Expression of amyotrophic lateral sclerosis-linked SOD1 mutant increases the neurotoxic potential of microglia via TLR2. J Biol Chem 284(6):3691–3699. https://doi.org/10.1074/jbc.M804446200
Lee JK, Shin JH, Gwag BJ, Choi EJ (2015) Iron accumulation promotes TACE-mediated TNF-alpha secretion and neurodegeneration in a mouse model of ALS. Neurobiol Dis 80:63–69. https://doi.org/10.1016/j.nbd.2015.05.009
Lemarchant S, Pomeshchik Y, Kidin I, Karkkainen V, Valonen P, Lehtonen S, Goldsteins G, Malm T, Kanninen K, Koistinaho J (2016) ADAMTS-4 promotes neurodegeneration in a mouse model of amyotrophic lateral sclerosis. Mol Neurodegener 11:10. https://doi.org/10.1186/s13024-016-0078-3
DiFiglia M, Sapp E, Chase KO, Davies SW, Bates GP, Vonsattel JP, Aronin N (1997) Aggregation of huntingtin in neuronal intranuclear inclusions and dystrophic neurites in brain. Science 277(5334):1990–1993
Sapp E, Schwarz C, Chase K, Bhide PG, Young AB, Penney J, Vonsattel JP, Aronin N, DiFiglia M (1997) Huntingtin localization in brains of normal and Huntington’s disease patients. Ann Neurol 42(4):604–612. https://doi.org/10.1002/ana.410420411
Wheeler VC, White JK, Gutekunst CA, Vrbanac V, Weaver M, Li XJ, Li SH, Yi H, Vonsattel JP, Gusella JF, Hersch S, Auerbach W, Joyner AL, MacDonald ME (2000) Long glutamine tracts cause nuclear localization of a novel form of huntingtin in medium spiny striatal neurons in HdhQ92 and HdhQ111 knock-in mice. Hum Mol Genet 9(4):503–513
Wellington CL, Singaraja R, Ellerby L, Savill J, Roy S, Leavitt B, Cattaneo E, Hackam A, Sharp A, Thornberry N, Nicholson DW, Bredesen DE, Hayden MR (2000) Inhibiting caspase cleavage of huntingtin reduces toxicity and aggregate formation in neuronal and nonneuronal cells. J Biol Chem 275(26):19831–19838. https://doi.org/10.1074/jbc.M001475200
Hermel E, Gafni J, Propp SS, Leavitt BR, Wellington CL, Young JE, Hackam AS, Logvinova AV, Peel AL, Chen SF, Hook V, Singaraja R, Krajewski S, Goldsmith PC, Ellerby HM, Hayden MR, Bredesen DE, Ellerby LM (2004) Specific caspase interactions and amplification are involved in selective neuronal vulnerability in Huntington’s disease. Cell Death Diff 11(4):424–438. https://doi.org/10.1038/sj.cdd.4401358
Gafni J, Hermel E, Young JE, Wellington CL, Hayden MR, Ellerby LM (2004) Inhibition of calpain cleavage of huntingtin reduces toxicity: accumulation of calpain/caspase fragments in the nucleus. J Biol Chem 279(19):20211–20220. https://doi.org/10.1074/jbc.M401267200
Miller JP, Holcomb J, Al-Ramahi I, de Haro M, Gafni J, Zhang N, Kim E, Sanhueza M, Torcassi C, Kwak S, Botas J, Hughes RE, Ellerby LM (2010) Matrix metalloproteinases are modifiers of huntingtin proteolysis and toxicity in Huntington’s disease. Neuron 67(2):199–212. https://doi.org/10.1016/j.neuron.2010.06.021
Naphade S, Embusch A, Madushani KL, Ring KL, Ellerby LM (2017) Altered expression of matrix metalloproteinases and their endogenous inhibitors in a human isogenic stem cell model of Huntington’s disease. Front Neurosci 11:736. https://doi.org/10.3389/fnins.2017.00736
Silvestroni A, Faull RL, Strand AD, Moller T (2009) Distinct neuroinflammatory profile in post-mortem human Huntington’s disease. NeuroReport 20(12):1098–1103. https://doi.org/10.1097/WNR.0b013e32832e34ee
Chang KH, Wu YR, Chen YC, Chen CM (2015) Plasma inflammatory biomarkers for Huntington’s disease patients and mouse model. Brain Behav Immun 44:121–127. https://doi.org/10.1016/j.bbi.2014.09.011
Connolly C, Magnusson-Lind A, Lu G, Wagner PK, Southwell AL, Hayden MR, Bjorkqvist M, Leavitt BR (2016) Enhanced immune response to MMP3 stimulation in microglia expressing mutant huntingtin. Neuroscience 325:74–88. https://doi.org/10.1016/j.neuroscience.2016.03.031
Duran-Vilaregut J, del Valle J, Manich G, Camins A, Pallas M, Vilaplana J, Pelegri C (2011) Role of matrix metalloproteinase-9 (MMP-9) in striatal blood-brain barrier disruption in a 3-nitropropionic acid model of Huntington’s disease. Neuropathol Appl Neuro 37(5):525–537. https://doi.org/10.1111/j.1365-2990.2010.01157.x
Vinther-Jensen T, Bornsen L, Budtz-Jorgensen E, Ammitzboll C, Larsen IU, Hjermind LE, Sellebjerg F, Nielsen JE (2016) Selected CSF biomarkers indicate no evidence of early neuroinflammation in Huntington disease. Neurol Neuroimmun Neuroinfln 3(6):e287. https://doi.org/10.1212/NXI.0000000000000287
Lo Sardo V, Zuccato C, Gaudenzi G, Vitali B, Ramos C, Tartari M, Myre MA, Walker JA, Pistocchi A, Conti L, Valenza M, Drung B, Schmidt B, Gusella J, Zeitlin S, Cotelli F, Cattaneo E (2012) An evolutionary recent neuroepithelial cell adhesion function of huntingtin implicates ADAM10-Ncadherin. Nat Neurosci 15(5):713–721. https://doi.org/10.1038/nn.3080
Acknowledgements
This work was supported by funding from the CNRS and Aix-Marseille Université and by public grants overseen by the French National Research Agency (ANR), MAD5 to SR, and PREVENTAD to MK, as part of the second “Investissements d’Avernir” program. The work was also supported by the DHUNE Centre of Excellence and grants from CoEN, “Fondation Plan Alzheimer”, France Alzheimer and Vaincre l’Alzheimer to SR. KB was granted a research associate fellowship (Management of Talents) by the Initiative d’Excellence of Aix-Marseille University - A*MIDEX, a French “Investissements d’Avenir” programme.
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Rivera, S., García-González, L., Khrestchatisky, M. et al. Metalloproteinases and their tissue inhibitors in Alzheimer’s disease and other neurodegenerative disorders. Cell. Mol. Life Sci. 76, 3167–3191 (2019). https://doi.org/10.1007/s00018-019-03178-2
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DOI: https://doi.org/10.1007/s00018-019-03178-2