Abstract
Plasmin is the key enzyme involved in the dissolution of fibrin. It is produced from plasminogen, which is activated by a plasminogen activator – the two primary activators are tissue-type plasminogen activator (tPA) and urinary-type plasminogen activator (uPA), also called urokinase. The process is regulated by inhibitors, principally plasminogen activator inhibitor 1 (PAI-1), α2-antiplasmin (α2AP) and thrombin-activatable fibrinolysis inhibitor (TAFI). Crucial control is exerted by surfaces, such as fibrin or cells, with plasminogen activation not normally occurring in the circulation. Here we will consider the individual players of the fibrinolytic cascade and their specific locations and potential interactions. Key questions considered are the initiation of fibrinolysis and the most appropriate ways to measure abnormalities in disease situations.
Access provided by Autonomous University of Puebla. Download chapter PDF
Similar content being viewed by others
Keywords
Fibrin as a Substrate
Plasmin is a potent trypsin-like serine protease that cleaves any substrate after lysyl or arginyl bonds. It activates growth factors and prohormones, actions that are outside the scope of this review, but its main substrate in vivo is fibrin. Many of the cleavage sites in fibrin have been revealed by the study of fibrinogen, which, as a soluble protein, is easier to analyse (reviewed by [1]). The ordered degradation pattern (Fig. 5.1) is detailed here as it is essential to our understanding of what is measured in assays of D-dimer and other fibrin degradation products (FDP). The first cut is to the α-chain of fibrinogen, releasing the αC fragments; the remainder of the molecule is called fragment X (~260 kDa). Fragment X is then cut in the α-, β- and γ-chains across the coiled coil that connects the central E and terminal D domains of fragment X. The cleavage occurs in two steps, first splitting the molecule asymmetrically to generate fragment Y (~160 kDa) and fragment D (~100 kDa) and then cleaving fragment Y into a second fragment D and fragment E (~60 kDa), which contains the amino terminal portion of all six polypeptide chains.
Newly formed fibrin is degraded by plasmin with the same cleavage pattern as fibrinogen, indicating that no major structural reorganization occurs during fibrin polymerization [2, 3]. In contrast, when fibrin is cross-linked by the transglutaminase factor XIIIa (Fig. 5.1, right), it is cleaved at a slower rate and different degradation products arise. D-dimer , which consists of two fragments D from adjacent fibrin monomers, cross-linked via their γ-chains remnants, is generated. This covalent dimer, bound non-covalently to fragment E, is the DD/E complex. This fragment also occurs in long arrays held together by uncleaved coiled coils [4]. Larger FDP have the capacity to reassociate with one another and with fibrin [5], so the substrate for fibrinolysis is not a single entity but a complex and dynamic one, in which both formation and degradation occur simultaneously. The clearance of FDP from the circulation is via the kidney and also liver, depending on the actual fragment [6, 7].
Fibrin as a Vital Surface for Plasmin Generation and Activity
Fibrin is at the heart of the lytic cascade and plays a vital role in “orchestrating its own destruction” [1]. This behaviour will be explained by considering the proteases and inhibitors that regulate the system, stressing throughout the governing role of fibrin.
Plasminogen
Plasminogen is a 92-kDa glycoprotein, abundant in plasma (Table 5.1). It is a classic zymogen, a single-chain molecule, activated by cleavage of one peptide bond to produce plasmin, in which the two chains are held together by two disulphide bonds. It is composed of several discretely folded domains. From the N-terminus, these are the activation peptide, a pan apple domain, kringles 1–5 and the protease domain (Fig. 5.2). The crystal structure of plasminogen indicates that two chloride ions in association with the pan apple and serine protease domain hold the zymogen in an inactive closed conformation [8]. The kringles, particularly kringle 1 [8], endow plasminogen with the capacity to bind to cells and other proteins; the most relevant to this chapter are fibrin, α2AP and TAFI. Such binding has profound effects on plasminogen activation. Plasminogen is primarily produced by the liver and is classified as an acute-phase protein [9]. Cells other than hepatocytes can produce plasminogen, for example, eosinophils, kidney, cornea, brain and adrenal medulla; such plasminogen is more likely to have local effects acting on substrates other than fibrin [10,11,12,13]. Human deficiency of plasminogen is uncommon, but when it occurs, it is often in association with fibrin deposition, for instance, in ligneous conjunctivitis [14].
Native plasminogen has several variants, in terms of limited proteolysis, degree of glycosylation and genetic polymorphism. For the purposes of this review, we will consider only the two main variants, Glu-plasminogen, the full-length form, and Lys-plasminogen, which has been processed to a variable extent at the N-terminus by trace plasmin. These two forms differ markedly in how efficiently they are activated (Fig. 5.2). Glu-plasminogen is a relatively closed structure [15], whereas Lys-plasminogen is more flexible and open; it binds to the plasminogen activator approximately tenfold more effectively [16,17,18]. Lys-plasminogen also binds to fibrin with higher affinity than Glu-plasminogen. The same is true of binding to plasminogen receptors, a group of proteins that are exposed on cell surfaces and bind to plasminogen via lysine residues [19]. Thus, through several mechanisms, Lys-plasminogen is activated more readily, especially on the fibrin or cell surface [20].
Plasminogen Activators
The principal plasminogen activators are tPA and uPA, while the contact pathway plays a role in some contexts. Activation of plasminogen is always by cleavage of Arg561-Val562 bond, yielding the two-chain active form, plasmin. It may be helpful to consider the life cycle of a plasminogen activator in terms of synthesis and release into the circulation, neutralization by inhibitors and clearance from the circulation by receptor-mediated mechanisms.
tPA is produced by endothelial and other cells as a single chain but is exceptional in that it is an active serine protease and not a true zymogen [21]. It circulates at low concentrations, mostly in complex with its primary inhibitor, PAI-1 [22, 23]. The plasma half-life is very short (Table 5.1) and shows a circadian rhythm, with lowest levels at night. Plasma tPA can be increased approximately fourfold under experimental conditions by venous occlusion or by drugs that induce acute endothelial release, such as bradykinin, histamine and β-adrenergic agents [24, 25]. Exercise also augments adrenalin-mediated tPA release, but also decreases clearance from the circulation [26]. Both tPA and tPA-PAI-1 complex are cleared by the low-density lipoprotein-related protein receptor (LRP) system [27].
tPA contains a finger domain and two kringle domains; the finger domain is the basis for its affinity to fibrin [28, 29]. This characteristic is crucial because tPA is a poor plasminogen activator in solution and requires fibrin to function as a cofactor in the reaction. Fibrinogen is not able to accelerate plasminogen activation by tPA, as the sites are encrypted in the precursor form [30]. Single-chain and two-chain tPA bind to fibrin in a comparable way [31] with plasminogen increasing the affinity of tPA for fibrin some 20-fold [32], as a result of ternary complex formation. In the absence of fibrin, the KM values range from 9 to 100 μM plasminogen [33,34,35]. In most studies, this KM value is three- to fourfold lower with two-chain tPA than with the single-chain form, a difference that essentially disappears in the presence of fibrin, when both forms of tPA yield KM values ranging from 0.16 to 1.1 μM plasminogen [33, 35]. These concentrations are readily achieved in blood (Table 5.1). One clear reason for the experimental range in these data is that the kinetics are non-linear [34, 36, 37], with a dual-phase activation. Starting with Glu-plasminogen and tPA in the presence of fibrin, the initial KM of 1.05 μM plasminogen was observed. Following plasmin formation and generation of partially digested fibrin, binding of both plasminogen and tPA increased [38,39,40,41,42], so that the KM was decreased to 0.07 μM plasminogen, with no change in kcat [37].
uPA is synthesized by several cell types, particularly those with a fibroblast-like morphology, but also by epithelial cells [43], monocytes and macrophages [44, 45]. uPA can activate solution-phase plasminogen; it does not require fibrin as a cofactor. This behaviour, which is in marked contrast with tPA, is sometimes interpreted to suggest that uPA is unimportant in fibrinolysis and certainly it has roles in other processes, such as extracellular matrix degradation, cell migration, wound healing, inflammation, embryogenesis and invasion of tumour cells and metastasis [46, 47].
uPA has three domains: an epidermal growth factor (EGF) domain, a kringle and a protease domain. The uPA kringle has no affinity for fibrin. Its main binding, via the EGF domain located in the amino-terminal fragment, is with a specific uPA receptor, uPAR, described later in this chapter. uPA is expressed in its single-chain (sc) form, which has trace proteolytic activity; full activity requires cleavage of Lys158-Ile159 [48]. This can be achieved by several enzymes, the most relevant being plasmin [49, 50], factor XIIa and kallikrein [51]. Normal plasma contains scuPA at relatively stable concentrations of 2–4 ng per mL [52, 53] with little circadian fluctuation [54]. While endothelium is not a major source of uPA, there are reports of increased uPA following venous stasis [53], DDAVP infusion [55] and strenuous physical exercise [56], probably explained by decreased clearance from the circulation by receptor-mediated mechanisms. Under normal circumstances ,uPA activity is not detected in plasma, but both leukocyte-associated and free scuPA are elevated in leukaemia [57] and other disorders, including liver disease [58]. If generated, uPA is rapidly cleared from plasma, in a manner that depends on hepatic blood flow [59]. The LRP system binds and internalizes scuPA and uPA-PAI-1 complexes [27, 60, 61]. The asialoglycoprotein receptor, on parenchymal liver cells, also removes nonsialated uPA from the circulation [59].
Contact activation is a distinct process resulting from the interactions of four proteins, factor XII (FXII), prekallikrein (PK), factor XI (FXI) and high-molecular-weight kininogen (HK). Negatively charged surfaces such as polyphosphate [62, 63], RNA [64], misfolded proteins [65] and collagen [66] stimulate reciprocal activation of FXII to FXIIa and of PK to kallikrein (PKa) in association with its non-enzymatic cofactor, HK. The process is accelerated by zinc ions which induce a conformational change in FXII [67,68,69,70,71] and HK [72,73,74], thereby augmenting surface interactions. The downstream targets of these proteases have been debated as this pathway is associated with coagulation via cleavage of FXI to yield FXIa, inflammation by generation of bradykinin from HK and fibrinolysis.
Of note, while FXII is classified as a coagulation factor, it is structurally related to tPA, uPA and plasminogen [75, 76] and can function in plasminogen activation by different mechanisms. FXIIa directly activates plasminogen (Fig. 5.3) albeit relatively poorly compared to tPA and uPA [77,78,79]. However, the reaction is markedly enhanced by negatively charged surfaces such as dextran sulphate [80] and importantly by platelet-derived polyphosphate [81]. Circulating plasma concentrations of FXII are four orders of magnitude higher than tPA and uPA and, combined with the increase in plasma half-life, suggest that in certain environments or conditions, in vivo FXIIa could be a relevant plasminogen activator [82].
PKa generated by FXII-dependent [51, 83] and FXII-independent [84] pathways is a kinetically favourable activator of scuPA (Fig. 5.3) which in turn activates plasminogen. Finally, the vasoactive peptide bradykinin, described above in the inflammatory arm of the contact pathway, also indirectly impacts fibrinolysis by stimulating tPA release from endothelial cells [85, 86]. These three functionally distinct mechanisms implicate the contact pathway as a modulator of plasminogen activation, but further studies are necessary to unravel its contribution in different milieu.
Inhibitors of Plasmin Generation and Activity
The proteases of the system are controlled by inhibitors, most of which act directly on the proteases and form inactive complexes with them. PAI-1 and α2AP are members of the serpin family, which inhibit plasminogen activators and plasmin, respectively, via a reactive centre loop that mimics the protease substrate (reviewed by [87]). A second mode of action, exemplified by TAFIa, is modulation of the generation of fibrinolytic activity.
PAI-1 is the principal inhibitor of tPA and uPA and inhibits both with second-order rate constants greater than 107 M−1 S−1, close to the diffusion limit [88]. It does not inhibit scuPA, which is largely inactive, but it does associate with scuPA non-covalently [89]. It is an unusual serpin in that it spontaneously loses activity by insertion of its reactive centre loop into the core of the molecule [90]. This inactive form was originally termed “latent”, which unfortunately gives an impression that the latent material is physiologically activated. Reactivation is indeed possible, but only by chemical denaturation and refolding [91]. It was characterized originally as a product of endothelial cells but it is synthesized by most cells in culture, including megakaryocytes [92], endothelial cells [93], hepatocytes [94] and adipocytes [95,96,97]. PAI-1 is synthesized in its active form and circulates in plasma in complex with vitronectin, which stabilizes the active form substantially lengthening its plasma half-life [98].
PAI-1 plasma concentrations are approximately 20 ng per mL [99,100,101] but reported values range, even in normal individuals, from barely detectable to 40 ng per mL. The variations may be circadian; PAI-1 plasma concentration peaks in the morning [102,103,104], and in addition, PAI-1 is an acute-phase protein [105]. Understanding its behaviour in response to stress is complicated by the fact that it is synthesized by a wider range of cells than the classic acute-phase proteins and that it is responsive to many stimuli. Some variations in PAI-1 measurements may be methodological. It is necessary to exclude platelets and their release products in analysis of plasma PAI-1, since platelets are the major pool (more than 95%) of circulating PAI-1 antigen [106]. PAI-1 in plasma is in excess over tPA (Table 5.1); therefore, most of the tPA is in complex with PAI-1. Immunological assays of either protein generally measure both free and complexed forms, requiring care in interpretation. Gram-negative septicaemic patients have dramatically elevated plasma PAI-1 concentrations, as much as 50-fold over normal, and are associated with high mortality [107]. High circulating PAI-1 is associated with a range of disease, including cardiovascular disease [108, 109] and cancer [110]. The causal significance remains unclear, and it seems that high PAI-1 does not independently predict disease when factors like obesity, diabetes and elevated triglycerides are taken into account [111]. There is a guanine insertion/deletion polymorphism at position 675 in the PAI-1 promoter [112], which is associated with differences in circulating PAI-l [113], but the predictive power of this polymorphism appears to be low [111, 114]. Deficiency of PAI-1 in humans is rare but it causes a lifelong bleeding disorder, characteristically after a delay, consistent with normal clotting but premature lysis of haemostatic plugs at sites of vascular trauma [115,116,117,118]. Fibrinolytic inhibitors such as tranexamic acid decrease plasminogen activation and therefore are effective in normalizing haemostatic function in such patients [117, 118].
α2AP is the principal inhibitor of plasmin, the term fast-acting being used to stress the rapid inhibition, with a second-order rate constant of 4 × 107 per M per second [119]. Its plasma concentration is 1 μM, about half the molar concentration of plasminogen; it has to be remembered that plasma plasminogen is seldom, if ever, entirely converted to plasmin, so the inhibitor is usually in excess. It is synthesized in the liver and consequently decreased in patients with advanced impairment of hepatic function. The t1/2 of the native inhibitor is approximately 3 days, whereas the covalent plasmin/α2AP (PAP) complex is cleared with a t1/2 of approximately 0.5 days [120].
α2AP circulates in several forms, depending on limited proteolysis at N- and C-termini. The processing of the inhibitor has little impact on the inhibitory capacity of α2AP which depends on the reactive centre loop. Newly produced α2AP (Met form) has 12 residues at the N-terminus that can be cleaved to yield N-terminal Asn [121] by an antiplasmin cleaving enzyme (APCE) [122]. Both forms are equally represented in plasma [123]. The N-terminal cleavage is important because it reveals Gln2, in the processed, Asn form, the Gln2 being cross-linked to Lys 303 of the fibrin(ogen) Aα-chain by FXIIIa [124, 125]. In contrast, in the Met form, Gln2 is blocked [126]. Fibrin to which α2AP is cross-linked resists lysis by plasmin, and this observation was central to the discovery of the first human deficiency of α2AP [124]. Consistent with this, antibodies that react specifically with cross-linked α2AP stimulate lysis of fibrin [127].
Comparison of α2AP with other members of the serpin family reveals that it has a C-terminal extension of some 50 residues [121]. This full-length form and a shortened form are both detectable in normal human plasma [128]. The full-length form binds plasminogen but the processed form, which is still a potent inhibitor of plasmin, cannot bind plasminogen [129]. The enzyme responsible for this C-terminal cleavage has not yet been characterized. The ratio of two forms, plasminogen binding to non-binding, is approximately 2:1 in plasma. This was still true even in advanced liver cirrhosis [58], despite the impaired synthesis of α2AP in these patients.
Binding of α2AP to plasminogen competes with the plasminogen-fibrin interaction, as it occurs via the same lysine binding site (Fig. 5.4). Plasmin formed on fibrin is therefore relatively protected from the action of α2AP [130], a key finding in the control of fibrinolysis [130]. The experimental basis for this concept used lysine analogues, in the presence of which α2AP was about 100 times less effective in inhibiting plasmin [119]. The exact Lys residues responsible for binding the C-terminal region of α2AP to plasminogen are not conclusively defined. Studies have shown a major effect of Lys452, but that other internal Lys residues “tether” the kringles [131, 132]. A different study, in which Lys residues were systematically mutated, suggested that Lys436 had the greatest effect [133].
Thrombin-activatable fibrinolysis inhibitor (TAFIa; also known as carboxypeptidase B, U, R [134] and CPB2 gene product [135]) removes C-terminal lysyl residues from fibrin, which, as previously stressed, are important in the binding of plasminogen [136]. TAFI is produced as a zymogen (or procarboxypeptidase) and is activated by the thrombin/thrombomodulin complex [137] or by plasmin in the presence of glycosaminoglycans [138]. Its activation by thrombin makes it an important molecular link between fibrinolysis and coagulation [139]. TAFI is produced in the liver but there is considerable variation in normal circulating concentrations [136, 140] and only a fraction need be activated for full physiological impact [137]. Its activity is controlled by its instability, with an effective plasma half-life of only about 10 min [141]. The function of TAFIa was shown in clot lysis assays; potato tuber carboxypeptidase inhibitor relieves the inhibition [139, 142]. This approach and more sensitive and specific assays for TAFIa have shown that the carboxypeptidase must be maintained at a threshold level to be effective in modulating fibrinolysis; this level fluctuates in relation to plasmin concentration [143]. Several polymorphisms in the TAFI gene have been reported, resulting in four isoforms [144, 145]. These isoforms explain the normal wide range in concentration, but do not correlate strongly with disease [145, 146]. Thr325Ile polymorphism has been shown to be an independent risk factor for ST acute myocardial infarction in a Mexican population [147]. Elevated TAFI appears to be a mild risk factor for venous thrombosis [148], and it also increases in inflammation, correlating with other acute-phase markers [149]. Contrary to this, patients recently suffering a myocardial infarction have been shown to have lower levels of TAFI [150].
Increased fibrinolytic activity in haemophilia patients is explained by defective TAFI activation. Most thrombin is formed after clot formation, mainly by back activation of FXI by thrombin, with deficiencies in FXI resulting in a mild to moderate tissue-specific bleeding disorder (haemophilia C). In the absence of FXI, clots lyse more readily [151], which is associated with the loss in feedback activation of FXI by thrombin [152]. The enhanced generation of thrombin augments TAFI activation stabilizing clots against premature lysis [153, 154]. In line with this, defective TAFI activation in congenital haemophilia A is associated with uPA-mediated joint bleeding [155]. Addition of TAFI, thrombomodulin or factor VIII to haemophilia A plasma restores normal fibrinolysis [156]. Consistent with this, incorporation of anti-factor XI antibodies or inhibition of TAFIa in a rabbit model resulted in an almost twofold increase in endogenous thrombolytic activity [157].
We described earlier the potential contribution of the contact pathway in facilitating plasminogen activation. The role of FXIa in sustaining thrombin generation and therefore TAFI activation implicates the contact pathway in antifibrinolytic as well as profibrinolytic mechanisms. Indeed, abnormal clot structure and sensitivity to fibrinolysis have been described to help predict the risk of bleeding tendency in severe and partial FXI deficiency [158, 159].
Other Inhibitors
In most situations, α2AP, PAI-1 and TAFI are the major gatekeepers in the regulation of plasmin generation and activity, but there are other inhibitors that may function in specific circumstances, which will now be introduced briefly.
PAI-2 is an inhibitor of uPA purified from human placenta and the cell line U-937 [160, 161]. The role of PAI-2 as a PA inhibitor has been questioned [162], as mice deficient in PAI-2 do not present any major haemostatic abnormalities [163]. The intracellular location of this serpin and the fact that it is a much poorer inhibitor of uPA and tPA [161] have led researchers to believe that its functions may lie outside the haemostatic cascade. In the circulation, monocytes are the main reservoir of PAI-2 [164] and may increase fibrin stability on migration into thrombi, particularly as PAI-2 is cross-linked to fibrin [165]. Interestingly, deficiency of PAI-2 is found to interfere with venous thrombus resolution in mice [166], most likely due to the instigated inflammatory response. PAI-2 is not normally detected in normal plasma, except in pregnancy, where it rises steadily to reach approximately 250 ng/mL by the third trimester [167]. In placental dysfunction413,414 and intrauterine growth retardation [168,169,170], the rise in plasma PAI-2 is much smaller, highlighting its importance in normal foetal development. PAI-2 also occurs in plasma of patients with acute myeloblastic leukaemia (M4 and M5, [171]) and in patients with sepsis [172]. Local PAI-2 activity appears to be relevant to a number of cancers, and studies on the function of this serpin in these settings may provide further clues to its true biological role [173, 174].
α2-Macroglobulin (α2M) is a non-serpin inhibitor of wide specificity. This breadth of targets and its relatively high plasma concentration (2.5 g per L, 3 μM) make it an effective stand-in inhibitor that contains the activity of many proteases, including plasmin, tPA and uPA [57]. α2M is a tetramer made up of a pair of dimers containing two reactive sites. When proteases are inhibited by α2M, they generally retain activity towards small peptide substrates, but are unable to cleave larger targets.
C1-inhibitor is a highly glycosylated serpin that directly modulates the activity of C1r and C1s proteases of complement C1. It also inhibits the contact proteases, FXIIa, FXIa and PKa, as well as tPA, plasmin and uPA. It circulates in plasma at a relatively high concentration (1.7 μM). When tPA is in excess over PAI-1, complex formation with C1-inhibitor is observed [23, 58, 175]. Its diverse targets suggest that it would function in regulating contact phase–dependent fibrinolysis and the conversion of scuPA to uPA (Fig. 5.3). Indeed, peripheral blood mononuclear cells from patients with hereditary angioedema (HAE), arising from a deficiency in C1-inhibitor, express elevated levels of uPAR [176]. HAE is also associated with aberrant fibrinolytic activity as a result of dysregulated plasmin generation and inhibition. Indeed, during activation of fibrinolysis, approximately 15% of plasmin inhibition is reportedly accounted for by C1-inhibitor [177]. The increase in bradykinin generation in HAE patients will also augment tPA release from the endothelium.
Regulation of Plasmin Generation and Activity
So far, we have highlighted three important concepts: zymogen activation, protease inhibition and, crucially, the role of fibrin in promoting activation of plasminogen and protecting plasmin from inhibition. Further discussion requires consideration of particular situations, so we will now examine the balance of the various proteases and inhibitors in plasma, on platelets, cell surfaces and thrombi.
Plasma Balance
Plasminogen , the central player of the fibrinolytic system, circulates at approximately 5 orders of magnitude higher than tPA and scuPA (Table 5.1). Plasminogen is turned over relatively slowly, with a half-life of 2.2 days for Glu-plasminogen and 0.8 days for Lys-plasminogen, while tPA and scuPA have plasma half-lives of only minutes. From this we can infer that the rates of synthesis, release and clearance are low for plasminogen and much higher for the PA, illustrating the more dynamic part of the system. Similar considerations apply to the main inhibitors. PAI-1 is present in plasma at only 400 nM, while α2AP circulates at 1 μM, and again the plasma half-lives are in marked contrast.
Fibrinolytic activity is not normally detectable in plasma because plasminogen is a true zymogen, and therefore inactive, while the one active PA in plasma, tPA, is normally controlled by an excess of PAI-1. Even if the concentration of PAI-1 were insufficient for full neutralization, then α2AP, C1-inhibitor and α2M would act as backup inhibitors. The other potential activator, scuPA, is not sufficiently active to initiate the process of plasminogen activation, as prior activation by plasmin or kallikrein is necessary. Any trace of plasmin generated in plasma would be quickly neutralized by α2AP, again endorsed as necessary by other inhibitors, especially α2M. So the quiescence of the system, in plasma, is maintained by tight control of protease activity, both at the level of existence of plasminogen as a zymogen and at the level of control by inhibitors, primarily PAI-1 and α2AP.
Cellular and Platelet Contributions
While the central role of fibrin in controlling activation of plasminogen and protection of plasmin has been appreciated for several years [130], we are now aware that many of the same general characteristics apply to cell-based or platelet-based fibrinolysis. That is, more efficient activation of plasminogen occurs on the surface of cells, while cell-bound plasmin is protected from inhibition by α2AP [178]. Plasminogen binding to circulating cells, including monocytes, neutrophils and platelets, was first reported in 1985 [179]. Binding to platelets is now known to occur in distinct locations, dependent on the specific subpopulation [180]. The proteins responsible for binding vary from cell to cell but include PlgRKT, α-enolase, S100A10 (functioning with annexin A2), actin, cytokeratin 8 and integrins αIIbβ3 and αMβ2 (reviewed by [181]). The binding of plasminogen to these receptors tends to be low affinity but high capacity, with some cell-surface proteins only found on cells undergoing apoptosis. Not all these proteins express the C-terminal Lys that is expected of a plasminogen-binding protein. PlgRKT is a true membrane protein and is synthesized with a C-terminal Lys residue. tPA binding to cells occurs via annexin II and also directly to PlgRKT [181]. Other reports on tPA receptors, which have been characterized in less detail [182, 183], may be of the same or similar molecules.
uPA and scuPA bind to a well-characterized receptor, uPAR (CD87), with high affinity (KD 10−9 to 10−11 M) depending on the cell type [184]. uPAR is not a transmembrane protein but is attached to membranes via a glycosylphosphatidylinositol (GPI) anchor. Binding of uPA to uPAR elicits signalling [185], via other intracellular proteins. Other proteins also bind uPAR, including vitronectin and integrins in complex with caveolin [186]. The uPA/uPAR complex on some cells is associated with Endo 180, also known as uPAR-associated protein (uPARAP) [187], and has a role in collagen IV internalization [188]. uPA bound to uPAR is still inactivated by PAI-1 but not as fast as in solution [189]. The uPA/PAI-1 complex is then internalized, while uPAR is recycled to the surface, a process that also involves LRP [61, 190]. uPAR has clear roles in migration and metastasis. In terms of fibrin degradation, we must distinguish between activation by scuPA and uPA. In the case of uPA, which can freely activate plasminogen in solution, binding to uPAR seems not to affect plasminogen activation, but the activity of scuPA is increased by two orders of magnitude when it is bound to uPAR on the surface of monocytes [191, 192]. An elegant experiment in which a uPA variant was directly anchored to the cell surface showed a stimulation of plasminogen activation similar to that achieved by binding to uPAR [193]. This is consistent with the principal function of uPAR being one of localization of uPA to the cell surface rather than enhancement of catalytic activity. The same co-localization and reciprocal activation of scuPA and plasminogen occurs on platelets [50], which do not express uPAR, indicating there are additional receptors yet to be discovered. Other studies show that cellular binding of plasminogen and (sc)uPA does not have to be on the same cells or surface to facilitate fibrinolysis [194].
Platelets make several contributions to clot stability and lysis. On the profibrinolytic side, activated platelets exhibit endogenous plasmin activity [180] and surface-bound plasmin, formed from local plasminogen, is afforded protection from inhibition by α2AP. On the antifibrinolytic side, there is the physical barrier to lysis that results from clot retraction, added to which platelets have a pool of FXIII [195] that stabilizes fibrin. Further, platelets are a source of the three main inhibitors of fibrinolysis, PAI-1, α2AP and TAFI (Fig. 5.5). These platelet-derived pools result from synthesis and packaging of the inhibitors at the megakaryocyte stage. Indeed, it has been reported that while platelets are devoid of a nucleus, they are capable of synthesizing large quantities of PAI-1 [196]. Recent work has illustrated that despite our traditional view that PAI-1 is released from platelets, a considerable amount of active PAI-1 is retained on the activated platelet membrane [197]. In terms of activity, platelet PAI-1 is less active than plasma PAI-1, but platelets still account for some 50% of the total circulating active PAI-1. The platelet pools of α2AP and TAFI are not as substantial, accounting for less than 1% of the total blood pool [198, 199] and may have functional significance in particular niches. The interaction of platelets and fibrin is regulated by the integrin αIIbβ3 and is key to the process of clot retraction. A recent elegant study has illustrated that the processes of clot retraction and fibrinolysis are mechanistically coupled indicating their intrinsic interaction in vivo to modulate thrombus size [200].
Studies on human thrombi reveal that the inhibitors of fibrinolysis, especially PAI-1, accumulate in great excess over proteases [201, 202], providing an explanation as to why established thrombi are often resistant to lysis. Observations on human thrombi also show they retain substantial amounts of coagulant and fibrinolytic activity [203, 204]. Of course, such diverse material is taxing to work on in a quantitative way and there are obviously differences in venous and arterial thrombi and between mural and luminal thrombi. Our studies in Chandler model thrombi showed that these thrombi lyse spontaneously, with fibrinolytic activity that could be ascribed primarily to uPA but to a lesser extent to tPA, elastase and cathepsin G [205]. This spontaneous generation of fibrinolytic activity [204] was dependent on polymorphonuclear cells, primarily neutrophils, generating local uPA activity on uPAR [205]. Plasma α1-antitrypsin was crucial in protecting the activity from neutrophil elastase [206]. The integrin αMβ2 is important in the generation of such local activity [207]. Discovery of a role for local uPA in thrombus lysis ran counter to the usual proposition that tPA’s role is fibrin degradation and uPA mediates other cellular events. There is, however, compelling support for it from a number of other studies, including failure of thrombi from uPA gene knockout mice to resolve [208]. In that model, the uPA activity was associated primarily with monocytes, which migrate into thrombi [209] and express fibrinolytic activity [44]. Indeed, monocyte-bound uPA has been shown to reduce thrombus size in a model of venous thrombosis [210].
Questions That Remain
What Initiates Fibrinolysis?
The available evidence suggests that the Glu-plasminogen to Lys-plasminogen conversion is the initiating event. It has the required features of leading to large-scale amplification as the plasminogen binding sites on fibrin are revealed by partial lysis, and formed plasmin is protected from α2AP. Part of the same question is which PA is responsible for the first molecules of plasmin that allow Glu-plasminogen to be converted to Lys-plasminogen? In the context of fibrin, with no cells or platelets, it may be tPA, a few molecules of which may be free of PAI-1, that provides initiation, especially since its single-chain form is active and not as readily inactivated by PAI-1 . This has been suggested by Thorsen (1992) in his well-established biphasic lysis [211], where a small amount of plasminogen on fibrin fibres is activated and then degrades fibrin to generate C-terminal lysine residues that bind additional plasminogen and perhaps tPA, leading to the second faster phase of tPA-mediated fibrinolysis [212]. The molecular interactions and specific binding sites involved have been extensively reviewed [30]. Experiments using tPA variants show that the finger domain of tPA plays a more dominant role in the interaction with fibrin than the kringle 2 interaction with C-terminal lysine residues [213]. This suggests that it is the binding of plasminogen to partially degraded fibrin, and thus subsequently the opening of the closed to open confirmation, that is the crucial step in the rapid second phase of fibrinolysis. This central role of plasminogen may suggest that the PA responsible for activation is less crucial than previously assumed. Our experiments with TAFI demonstrated a similar delay in lysis regardless of the PA used [214] and we interpreted this as plasminogen primarily controlling fibrin-bound plasmin generation.
If a cell membrane is present, then it may be scuPA , bound to cellular uPAR or on platelets, that yields the initial protease activity. This is suggested on the basis of several experimental systems, including data showing that the ordered addition of scuPA and then tPA [215] is potentially more effective than either agent alone. Our own work on Chandler model thrombi underlines the importance of the scuPA/uPA system in spontaneous lysis [205] but affirms the involvement of other proteases, especially tPA [204]. When in association with cellular uPAR, scuPA binds PAI-1 and other serpins reversibly [89]. This has been interpreted in terms of receptor-bound scuPA initiating proteolytic activity, with conversion to uPA achieving inhibition thereby regulating the activity [216].
How Best to Measure Fibrinolysis?
Fibrinolysis, like other cascade systems, coagulation and complement, can be studied by various means. Individual components can be quantified, either as antigen or activity, and under defined situations can provide clear answers. However, the complexities of the system mean that a change in one factor can influence measurements of another and therefore it is important to interpret results with caution. As an example, tPA activity is challenging to measure in plasma, as it is at the limit of detection of most assays. Elevated PAI-1 may depress the activity that is measured. Frequently, a manipulation of plasma is necessary to reveal tPA activity, including acidification of plasma or preparation of a euglobulin fraction, where tPA, plasminogen and fibrinogen are retained. Most inhibitors are removed but about 50% of PAI-1 is retained [100], and these facts must be borne in mind for valid interpretation. As mentioned previously, circulating tPA is variable, whether at the level of synthesis or release; therefore, it is vital to consider the time course as each sample represents a snapshot. Rapid hepatic clearance of tPA and of tPA-PAI-1 complex from the circulation rapidly restores the system to normality, allowing key events to be overlooked.
It is often essential to measure more than one analyte for a fuller appreciation of the system. Ideally, the aim is to know how much enzyme is free and/or active and how much has been converted to a complex, such as tPA-PAI-1. A combination of ELISA and activity assays may provide a clear picture, but only if the specificity of the ELISA is known in some detail. Ideally, measurement of PA would be complemented by examining a consequence of the elevation, for instance, the fibrin degradation products produced, which of course reflects the presence of the fibrin substrate, or generation of the plasmin-α2AP complex. The essential feature of ELISA for a complex is the use of antibody to one of the proteins, e.g. α2AP, as a capture system and an antibody to the second moiety, e.g. plasmin, in the detection system . The capture antibody in this example will bind free α2AP and α2AP in complex, giving rise to potential competition and misrepresentation of the results. This element limits the use of these assays to situations where the free protein is decreased, for instance, in liver disease, where α2AP is lower than normal. Other approaches to measuring overall fibrinolytic activity in plasma include measurement of a zone of lysis on a fibrin plate, clot lysis assays and zymography. Recently, a method which combines magnetic immunocapture of leukocyte-derived microvesicles and chromogenic measurement of plasmin generation has been described [217]. These can all be useful but there are limitations associated with most individual assays. For instance, in plasma clot lysis assays, the effects of FXIIIa cannot be reproducibly observed [218]. In addition, the overwhelming effects of α2AP make it difficult to see inhibition by PAI-1. Failure to be alert to such considerations gives rise, in the literature, to many inappropriate interpretations about the relative importance of particular proteases or inhibitors. In all assays, the balance of enzyme to inhibitor ought to be as close to physiological as possible. When tPA is added, it should be at a low concentration, always remembering that it is a catalyst, not a reagent that is consumed. The literature abounds with examples where PA are added at high concentrations, simply to speed up the assay. This distorts a system that is designed to be delicately poised and generates artefacts of the experimental system rather than a true reflection of what goes on in vivo.
Detailed analysis of the fibrinolytic system is only practical for small numbers of samples, but, for large clinical cohorts, the aim is to obtain an insight from a limited number of assays. Not surprisingly this has promoted the use of overall measures of activity, such as global assays of fibrinolysis, which have inherent advantages and some limitations. Thromboelastography is rapid, widely available and easily applicable to large sample sizes. However, most studies add tPA as a stimulus. In this situation, added enzyme should be kept to a minimum, to avoid generating results that are far from physiological. Another global assay quantified fibrin degradation products after collection of blood samples onto thrombin [219]. Comparison of samples with and without aprotinin gives a measure of global fibrinolytic capacity, an approach that has proved useful clinically [220]. It should be noted that thrombin greatly enhances endogenous fibrinolytic activity, probably by inactivation of PAI-1 among other mechanisms. This consideration serves as a useful aide-mémoire that fibrinolysis is not an independent system. As Ratnoff reminds us, “The coagulation, fibrinolysis, complement and kinin pathways are studied separately by scientists for their convenience. In life, they form a seamless web” [221]. Undoubtedly, we choose our approaches and molecules of interest to us, and may well ignore other players, by virtue of the experimental system used. These choices may be convenient, but we must bear in mind the selection bias introduced into the system.
References
Gaffney PJ. Fibrin degradation products. A review of structures found in vitro and in vivo. Ann N Y Acad Sci. 2001;936:594–610.
Dudek GA, Kloczewiak M, Budzynski AZ, Latallo ZS, Kopec M. Characterisation and comparison of macromolecular end products of fibrinogen and fibrin proteolysis by plasmin. Biochim Biophys Acta. 1970;214(1):44–51.
Pizzo SV, Schwartz ML, Hill RL, McKee PA. The effect of plasmin on the subunit structure of human fibrin. J Biol Chem. 1973;248(13):4574–83.
Francis CW, Marder VJ, Barlow GH. Plasmic degradation of crosslinked fibrin. Characterization of new macromolecular soluble complexes and a model of their structure. J Clin Invest. 1980;66(5):1033–43.
Walker JB, Nesheim ME. The molecular weights, mass distribution, chain composition, and structure of soluble fibrin degradation products released from a fibrin clot perfused with plasmin. J Biol Chem. 1999;274(8):5201–12.
Hedner U. Urinary fibrin/fibrinogen derivatives. Thromb Diath Haemorrh. 1975;34(3):693–708.
Dardik BN, Shainoff JR. Kinetic characterization of a saturable pathway for rapid clearance of circulating fibrin monomer. Blood. 1985;65(3):680–8.
Law RH, Caradoc-Davies T, Cowieson N, Horvath AJ, Quek AJ, Encarnacao JA, et al. The X-ray crystal structure of full-length human plasminogen. Cell Rep. 2012;1(3):185–90.
Bannach FG, Gutierrez A, Fowler BJ, Bugge TH, Degen JL, Parmer RJ, et al. Localization of regulatory elements mediating constitutive and cytokine-stimulated plasminogen gene expression. J Biol Chem. 2002;277(41):38579–88.
Raum D, Marcus D, Alper CA, Levey R, Taylor PD, Starzl TE. Synthesis of human plasminogen by the liver. Science. 1980;208(4447):1036–7.
Highsmith RF, Kline DL. Kidney: primary source of plasminogen after acute depletion in the cat. Science. 1971;174(5):141–2.
Twining SS, Wilson PM, Ngamkitidechakul C. Extrahepatic synthesis of plasminogen in the human cornea is up-regulated by interleukins-1alpha and -1beta. Biochem J. 1999;339(Pt 3):705–12.
Zhang L, Seiffert D, Fowler BJ, Jenkins GR, Thinnes TC, Loskutoff DJ, et al. Plasminogen has a broad extrahepatic distribution. Thromb Haemost. 2002;87(3):493–501.
Schuster V, Mingers AM, Seidenspinner S, Nussgens Z, Pukrop T, Kreth HW. Homozygous mutations in the plasminogen gene of two unrelated girls with ligneous conjunctivitis. Blood. 1997;90(3):958–66.
Mangel WF, Lin BH, Ramakrishnan V. Characterization of an extremely large, ligand-induced conformational change in plasminogen. Science. 1990;248(4951):69–73.
Urano T, Chibber BA, Castellino FJ. The reciprocal effects of epsilon-aminohexanoic acid and chloride ion on the activation of human [Glu1]plasminogen by human urokinase. Proc Natl Acad Sci U S A. 1987;84(12):4031–4.
Sjoholm I. Studies on the conformational changes of plasminogen induced during activation to plasmin and by 6-aminohexanoic acid. Eur J Biochem. 1973;39(2):471–9.
Castellino FJ. Biochemistry of human plasminogen. Semin Thromb Hemost. 1984;10(1):18–23.
Plow EF, Doeuvre L, Das R. So many plasminogen receptors: why? J Biomed Biotechnol. 2012;2012:141806.
Miles LA, Castellino FJ, Gong Y. Critical role for conversion of glu-plasminogen to Lys-plasminogen for optimal stimulation of plasminogen activation on cell surfaces. Trends Cardiovasc Med. 2003;13(1):21–30.
Madison EL. Probing structure-function relationships of tissue-type plasminogen activator by site-specific mutagenesis. Fibrinolysis. 1994;8(Suppl. 1):221–6.
Stalder M, Hauert J, Kruithof EK, Bachmann F. Release of vascular plasminogen activator (v-PA) after venous stasis: electrophoretic-zymographic analysis of free and complexed v-PA. Br J Haematol. 1985;61(1):169–76.
Booth NA, Walker E, Maughan R, Bennett B. Plasminogen activator in normal subjects after exercise and venous occlusion: t-PA circulates as complexes with C1-inhibitor and PAI-1. Blood. 1987;69(6):1600–4.
Tappy L, Hauert J, Bachmann F. Effects of hypoxia and acidosis on vascular plasminogen activator release in the pig ear perfusion system. Thromb Res. 1984;33(2):117–24.
Vaughan DE. The renin-angiotensin system and fibrinolysis. Am J Cardiol. 1997;79(5A):12–6.
Chandler WL, Levy WC, Stratton JR. The circulatory regulation of TPA and UPA secretion, clearance, and inhibition during exercise and during the infusion of isoproterenol and phenylephrine. Circulation. 1995;92(10):2984–94.
Strickland DK, Ranganathan S. Diverse role of LDL receptor-related protein in the clearance of proteases and in signaling. J Thromb Haemost. 2003;1(7):1663–70.
van Zonneveld AJ, Veerman H, Pannekoek H. On the interaction of the finger and the kringle-2 domain of tissue-type plasminogen activator with fibrin. Inhibition of kringle-2 binding to fibrin by epsilon-amino caproic acid. J Biol Chem. 1986;261(30):14214–8.
Longstaff C, Thelwell C, Williams SC, Silva MM, Szabo L, Kolev K. The interplay between tissue plasminogen activator domains and fibrin structures in the regulation of fibrinolysis: kinetic and microscopic studies. Blood. 2011;117(2):661–8.
Medved L, Nieuwenhuizen W. Molecular mechanisms of initiation of fibrinolysis by fibrin. Thromb Haemost. 2003;89(3):409–19.
Higgins DL, Vehar GA. Interaction of one-chain and two-chain tissue plasminogen activator with intact and plasmin-degraded fibrin. Biochemistry. 1987;26(24):7786–91.
Ranby M, Bergsdorf N, Nilsson T. Enzymatic properties of the one- and two-chain form of tissue plasminogen activator. Thromb Res. 1982;27(2):175–83.
Rijken DC, Hoylaerts M, Collen D. Fibrinolytic properties of one-chain and two-chain human extrinsic (tissue-type) plasminogen activator. J Biol Chem. 1982;257(6):2920–5.
Ranby M. Studies on the kinetics of plasminogen activation by tissue plasminogen activator. Biochim Biophys Acta. 1982;704(3):461–9.
Hoylaerts M, Rijken DC, Lijnen HR, Collen D. Kinetics of the activation of plasminogen by human tissue plasminogen activator. Role of fibrin. J Biol Chem. 1982;257(6):2912–9.
Geppert AG, Binder BR. Allosteric regulation of tPA-mediated plasminogen activation by a modifier mechanism: evidence for a binding site for plasminogen on the tPA A-chain. Arch Biochem Biophys. 1992;297(2):205–12.
Norrman B, Wallen P, Ranby M. Fibrinolysis mediated by tissue plasminogen activator. Disclosure of a kinetic transition. Eur J Biochem. 1985;149(1):193–200.
Suenson E, Lutzen O, Thorsen S. Initial plasmin-degradation of fibrin as the basis of a positive feed-back mechanism in fibrinolysis. Eur J Biochem. 1984;140(3):513–22.
Harpel PC, Chang TS, Verderber E. Tissue plasminogen activator and urokinase mediate the binding of Glu-plasminogen to plasma fibrin I. Evidence for new binding sites in plasmin-degraded fibrin I. J Biol Chem. 1985;260(7):4432–40.
Tran-Thang C, Kruithof EK, Atkinson J, Bachmann F. High-affinity binding sites for human Glu-plasminogen unveiled by limited plasmic degradation of human fibrin. Eur J Biochem. 1986;160(3):599–604.
Rijken DC, Wijngaards G, Zaal-de Jong M, Welbergen J. Purification and partial characterization of plasminogen activator from human uterine tissue. Biochim Biophys Acta. 1979;580(1):140–53.
de Vries C, Veerman H, Koornneef E, Pannekoek H. Tissue-type plasminogen activator and its substrate Glu-plasminogen share common binding sites in limited plasmin-digested fibrin. J Biol Chem. 1990;265(23):13547–52.
Larsson LI, Skriver L, Nielsen LS, Grondahl-Hansen J, Kristensen P, Dano K. Distribution of urokinase-type plasminogen activator immunoreactivity in the mouse. J Cell Biol. 1984;98(3):894–903.
Grau E, Moroz LA. Fibrinolytic activity of normal human blood monocytes. Thromb Res. 1989;53(2):145–62.
Manchanda N, Schwartz BS. Lipopolysaccharide-induced modulation of human monocyte urokinase production and activity. J Immunol. 1990;145(12):4174–80.
Dano K, Andreasen PA, Grondahl-Hansen J, Kristensen P, Nielsen LS, Skriver L. Plasminogen activators, tissue degradation, and cancer. Adv Cancer Res. 1985;44:139–266.
Duffy MJ. The urokinase plasminogen activator system: role in malignancy. Curr Pharm Des. 2004;10(1):39–49.
Lijnen HR, Van Hoef B, Collen D. Activation with plasmin of two-chain urokinase-type plasminogen activator derived from single-chain urokinase-type plasminogen activator by treatment with thrombin. Eur J Biochem. 1987;169(2):359–64.
Bernik MB. Increased plasminogen activator (urokinase) in tissue culture after fibrin deposition. J Clin Invest. 1973;52(4):823–34.
Baeten KM, Richard MC, Kanse SM, Mutch NJ, Degen JL, Booth NA. Activation of single-chain urokinase-type plasminogen activator by platelet-associated plasminogen: a mechanism for stimulation of fibrinolysis by platelets. J Thromb Haemost. 2010;8(6):1313–22.
Ichinose A, Fujikawa K, Suyama T. The activation of pro-urokinase by plasma kallikrein and its inactivation by thrombin. J Biol Chem. 1986;261(8):3486–9.
Wun TC, Schleuning WD, Reich E. Isolation and characterization of urokinase from human plasma. J Biol Chem. 1982;257(6):3276–83.
Darras V, Thienpont M, Stump DC, Collen D. Measurement of urokinase-type plasminogen activator (u-PA) with an enzyme-linked immunosorbent assay (ELISA) based on three murine monoclonal antibodies. Thromb Haemost. 1986;56(3):411–4.
Andreotti F, Kluft C. Circadian variation of fibrinolytic activity in blood. Chronobiol Int. 1991;8(5):336–51.
Levi M, ten Cate JW, Dooijewaard G, Sturk A, Brommer EJ, Agnelli G. DDAVP induces systemic release of urokinase-type plasminogen activator. Thromb Haemost. 1989;62(2):686–9.
Dooijewaard G, de Boer A, Turion PN, Cohen AF, Breimer DD, Kluft C. Physical exercise induces enhancement of urokinase-type plasminogen activator (u-PA) levels in plasma. Thromb Haemost. 1991;65(1):82–6.
Bennett B, Booth NA, Croll A, Dawson AA. The bleeding disorder in acute promyelocytic leukaemia: fibrinolysis due to u-PA rather than defibrination. Br J Haematol. 1989;71(4):511–7.
Booth NA, Anderson JA, Bennett B. Plasminogen activators in alcoholic cirrhosis: demonstration of increased tissue type and urokinase type activator. J Clin Pathol. 1984;37(7):772–7.
van der Kaaden MERD, Van Berkel TJC, et al. Plasma clearance of urokinase-type plasminogen activator. Fibrinolysis Proteolysis. 1998;12:251–8.
Kounnas MZ, Henkin J, Argraves WS, Strickland DK. Low density lipoprotein receptor-related protein/alpha 2-macroglobulin receptor mediates cellular uptake of pro-urokinase. J Biol Chem. 1993;268(29):21862–7.
Nykjaer A, Kjoller L, Cohen RL, Lawrence DA, Garni-Wagner BA, Todd RF 3rd, et al. Regions involved in binding of urokinase-type-1 inhibitor complex and pro-urokinase to the endocytic alpha 2-macroglobulin receptor/low density lipoprotein receptor-related protein. Evidence that the urokinase receptor protects pro-urokinase against binding to the endocytic receptor. J Biol Chem. 1994;269(41):25668–76.
Smith SA, Mutch NJ, Baskar D, Rohloff P, Docampo R, Morrissey JH. Polyphosphate modulates blood coagulation and fibrinolysis. Proc Natl Acad Sci U S A. 2006;103(4):903–8.
Muller F, Mutch NJ, Schenk WA, Smith SA, Esterl L, Spronk HM, et al. Platelet polyphosphates are proinflammatory and procoagulant mediators in vivo. Cell. 2009;139(6):1143–56.
Kannemeier C, Shibamiya A, Nakazawa F, Trusheim H, Ruppert C, Markart P, et al. Extracellular RNA constitutes a natural procoagulant cofactor in blood coagulation. Proc Natl Acad Sci U S A. 2007;104(15):6388–93.
Maas C, Govers-Riemslag JW, Bouma B, Schiks B, Hazenberg BP, Lokhorst HM, et al. Misfolded proteins activate factor XII in humans, leading to kallikrein formation without initiating coagulation. J Clin Invest. 2008;118(9):3208–18.
van der Meijden PE, Munnix IC, Auger JM, Govers-Riemslag JW, Cosemans JM, Kuijpers MJ, et al. Dual role of collagen in factor XII-dependent thrombus formation. Blood. 2009;114(4):881–90.
Shore JD, Day DE, Bock PE, Olson ST. Acceleration of surface-dependent autocatalytic activation of blood coagulation factor XII by divalent metal ions. Biochemistry. 1987;26(8):2250–8.
Schousboe I. The inositol-phospholipid-accelerated activation of prekallikrein by activated factor XII at physiological ionic strength requires zinc ions and high-Mr kininogen. Eur J Biochem. 1990;193(2):495–9.
Bernardo MM, Day DE, Halvorson HR, Olson ST, Shore JD. Surface-independent acceleration of factor XII activation by zinc ions. II. Direct binding and fluorescence studies. J Biol Chem. 1993;268(17):12477–83.
Bernardo MM, Day DE, Olson ST, Shore JD. Surface-independent acceleration of factor XII activation by zinc ions. I. Kinetic characterization of the metal ion rate enhancement. J Biol Chem. 1993;268(17):12468–76.
Shimada T, Kato H, Iwanaga S. Accelerating effect of zinc ions on the surface-mediated activation of factor XII and prekallikrein. J Biochem (Tokyo). 1987;102(4):913–21.
Greengard JS, Griffin JH. Receptors for high molecular weight kininogen on stimulated washed human platelets. Biochemistry. 1984;23(26):6863–9.
Zini JM, Schmaier AH, Cines DB. Bradykinin regulates the expression of kininogen binding sites on endothelial cells. Blood. 1993;81(11):2936–46.
Herwald H, Morgelin M, Svensson HG, Sjobring U. Zinc-dependent conformational changes in domain D5 of high molecular mass kininogen modulate contact activation. Eur J Biochem. 2001;268(2):396–404.
McMullen BA, Fujikawa K. Amino acid sequence of the heavy chain of human alpha-factor XIIa (activated Hageman factor). J Biol Chem. 1985;260(9):5328–41.
Tans G, Rosing J. Structural and functional characterization of factor XII. Semin Thromb Hemost. 1987;13(1):1–14.
Goldsmith GH Jr, Saito H, Ratnoff OS. The activation of plasminogen by Hageman factor (Factor XII) and Hageman factor fragments. J Clin Invest. 1978;62(1):54–60.
Miles LA, Greengard JS, Griffin JH. A comparison of the abilities of plasma kallikrein, beta-Factor XIIa, Factor XIa and urokinase to activate plasminogen. Thromb Res. 1983;29(4):407–17.
Schousboe I. Factor XIIa activation of plasminogen is enhanced by contact activating surfaces and Zn2+. Blood Coagul Fibrinolysis. 1997;8(2):97–104.
Schousboe I, Feddersen K, Rojkjaer R. Factor XIIa is a kinetically favorable plasminogen activator. Thromb Haemost. 1999;82(3):1041–6.
Mitchell JL, Lionikiene AS, Georgiev G, Klemmer A, Brain C, Kim PY, et al. Polyphosphate colocalizes with factor XII on platelet-bound fibrin and augments its plasminogen activator activity. Blood. 2016;128(24):2834–45.
Levi M, Hack CE, de Boer JP, Brandjes DP, Buller HR, ten Cate JW. Reduction of contact activation related fibrinolytic activity in factor XII deficient patients. Further evidence for the role of the contact system in fibrinolysis in vivo. J Clin Invest. 1991;88(4):1155–60.
Binnema DJ, Dooijewaard G, Turion PN. An analysis of the activators of single-chain urokinase-type plasminogen activator (scu-PA) in the dextran sulphate euglobulin fraction of normal plasma and of plasmas deficient in factor XII and prekallikrein. Thromb Haemost. 1991;65(2):144–8.
Motta G, Rojkjaer R, Hasan AA, Cines DB, Schmaier AH. High molecular weight kininogen regulates prekallikrein assembly and activation on endothelial cells: a novel mechanism for contact activation. Blood. 1998;91(2):516–28.
Smith D, Gilbert M, Owen WG. Tissue plasminogen activator release in vivo in response to vasoactive agents. Blood. 1985;66(4):835–9.
Brown NJ, Nadeau JH, Vaughan DE. Selective stimulation of tissue-type plasminogen activator (t-PA) in vivo by infusion of bradykinin. Thromb Haemost. 1997;77(3):522–5.
Huntington JA. Serpin structure, function and dysfunction. J Thromb Haemost. 2011;9(Suppl 1):26–34.
Madison EL, Goldsmith EJ, Gerard RD, Gething MJ, Sambrook JF. Serpin-resistant mutants of human tissue-type plasminogen activator. Nature. 1989;339(6227):721–4.
Manchanda N, Schwartz BS. Interaction of single-chain urokinase and plasminogen activator inhibitor type 1. J Biol Chem. 1995;270(34):20032–5.
Goldsmith EJ, Sheng-Cheng C, Danley DE, Gerard RD, Geoghegan KF, Mottonen J, et al. Preliminary X-ray analysis of crystals of plasminogen activator inhibitor-1. Proteins. 1991;9(3):225–7.
Hekman CM, Loskutoff DJ. Endothelial cells produce a latent inhibitor of plasminogen activators that can be activated by denaturants. J Biol Chem. 1985;260(21):11581–7.
Konkle BA, Schick PK, He X, Liu RJ, Mazur EM. Plasminogen activator inhibitor-1 mRNA is expressed in platelets and megakaryocytes and the megakaryoblastic cell line CHRF-288. Arterioscler Thromb. 1993;13(5):669–74.
van Mourik JA, Lawrence DA, Loskutoff DJ. Purification of an inhibitor of plasminogen activator (antiactivator) synthesized by endothelial cells. J Biol Chem. 1984;259(23):14914–21.
Cwikel BJ, Barouski-Miller PA, Coleman PL, Gelehrter TD. Dexamethasone induction of an inhibitor of plasminogen activator in HTC hepatoma cells. J Biol Chem. 1984;259(11):6847–51.
Morange PE, Alessi MC, Verdier M, Casanova D, Magalon G, Juhan-Vague I. PAI-1 produced ex vivo by human adipose tissue is relevant to PAI-1 blood level. Arterioscler Thromb Vasc Biol. 1999;19(5):1361–5.
Loskutoff DJ, Samad F. The adipocyte and hemostatic balance in obesity: studies of PAI-1. Arterioscler Thromb Vasc Biol. 1998;18(1):1–6.
Crandall DL, Quinet EM, Morgan GA, Busler DE, McHendry-Rinde B, Kral JG. Synthesis and secretion of plasminogen activator inhibitor-1 by human preadipocytes. J Clin Endocrinol Metab. 1999;84(9):3222–7.
Declerck PJ, De Mol M, Alessi MC, Baudner S, Paques EP, Preissner KT, et al. Purification and characterization of a plasminogen activator inhibitor 1 binding protein from human plasma. Identification as a multimeric form of S protein (vitronectin). J Biol Chem. 1988;263(30):15454–61.
Kruithof EK, Gudinchet A, Bachmann F. Plasminogen activator inhibitor 1 and plasminogen activator inhibitor 2 in various disease states. Thromb Haemost. 1988;59(1):7–12.
Booth NA, Simpson AJ, Croll A, Bennett B, MacGregor IR. Plasminogen activator inhibitor (PAI-1) in plasma and platelets. Br J Haematol. 1988;70(3):327–33.
Declerck PJ, Alessi MC, Verstreken M, Kruithof EK, Juhan-Vague I, Collen D. Measurement of plasminogen activator inhibitor 1 in biologic fluids with a murine monoclonal antibody-based enzyme-linked immunosorbent assay. Blood. 1988;71(1):220–5.
Andreotti F, Davies GJ, Hackett DR, Khan MI, De Bart AC, Aber VR, et al. Major circadian fluctuations in fibrinolytic factors and possible relevance to time of onset of myocardial infarction, sudden cardiac death and stroke. Am J Cardiol. 1988;62(9):635–7.
Angleton P, Chandler WL, Schmer G. Diurnal variation of tissue-type plasminogen activator and its rapid inhibitor (PAI-1). Circulation. 1989;79(1):101–6.
Kluft C, Jie AF, Rijken DC, Verheijen JH. Daytime fluctuations in blood of tissue-type plasminogen activator (t-PA) and its fast-acting inhibitor (PAI-1). Thromb Haemost. 1988;59(2):329–32.
Booth NA. The natural inhibitors of fibrinolysis. In: Bloom AL, Forbes CD, Thomas DP, et al., editors. Haemostasis and thrombosis. 3rd ed. Edinburgh: Churchill Livingstone; 1994. p. 699–717.
Johnson SA, Schneider CL. The existence of antifibrinolysin activity in platelets. Science. 1953;117(3035):229–30.
Pralong G, Calandra T, Glauser MP, Schellekens J, Verhoef J, Bachmann F, et al. Plasminogen activator inhibitor 1: a new prognostic marker in septic shock. Thromb Haemost. 1989;61(3):459–62.
Vaughan DE. Plasminogen activator inhibitor-1: a common denominator in cardiovascular disease. J Investig Med. 1998;46(8):370–6.
Juhan-Vague I, Pyke SD, Alessi MC, Jespersen J, Haverkate F, Thompson SG. Fibrinolytic factors and the risk of myocardial infarction or sudden death in patients with angina pectoris. ECAT Study Group. European Concerted Action on Thrombosis and Disabilities. Circulation. 1996;94(9):2057–63.
Carroll VA, Binder BR. The role of the plasminogen activation system in cancer. Semin Thromb Hemost. 1999;25(2):183–97.
Scarabin PY, Aillaud MF, Amouyel P, Evans A, Luc G, Ferrieres J, et al. Associations of fibrinogen, factor VII and PAI-1 with baseline findings among 10,500 male participants in a prospective study of myocardial infarction–the PRIME Study. Prospective Epidemiological Study of Myocardial Infarction. Thromb Haemost. 1998;80(5):749–56.
Dawson S, Hamsten A, Wiman B, Henney A, Humphries S. Genetic variation at the plasminogen activator inhibitor-1 locus is associated with altered levels of plasma plasminogen activator inhibitor-1 activity. Arterioscler Thromb. 1991;11(1):183–90.
Eriksson P, Kallin B, van ‘t Hooft FM, Bavenholm P, Hamsten A. Allele-specific increase in basal transcription of the plasminogen-activator inhibitor 1 gene is associated with myocardial infarction. Proc Natl Acad Sci U S A. 1995;92(6):1851–5.
Lowe GD, Yarnell JW, Sweetnam PM, Rumley A, Thomas HF, Elwood PC. Fibrin D-dimer, tissue plasminogen activator, plasminogen activator inhibitor, and the risk of major ischaemic heart disease in the Caerphilly Study. Thromb Haemost. 1998;79(1):129–33.
Dieval J, Nguyen G, Gross S, Delobel J, Kruithof EK. A lifelong bleeding disorder associated with a deficiency of plasminogen activator inhibitor type 1. Blood. 1991;77(3):528–32.
Fay WP, Shapiro AD, Shih JL, Schleef RR, Ginsburg D. Brief report: complete deficiency of plasminogen-activator inhibitor type 1 due to a frame-shift mutation. N Engl J Med. 1992;327(24):1729–33.
Lee MH, Vosburgh E, Anderson K, McDonagh J. Deficiency of plasma plasminogen activator inhibitor 1 results in hyperfibrinolytic bleeding. Blood. 1993;81(9):2357–62.
Fay WP, Parker AC, Condrey LR, Shapiro AD. Human plasminogen activator inhibitor-1 (PAI-1) deficiency: characterization of a large kindred with a null mutation in the PAI-1 gene. Blood. 1997;90(1):204–8.
Wiman B, Collen D. On the kinetics of the reaction between human antiplasmin and plasmin. Eur J Biochem. 1978;84(2):573–8.
Mast AE, Enghild JJ, Pizzo SV, Salvesen G. Analysis of the plasma elimination kinetics and conformational stabilities of native, proteinase-complexed, and reactive site cleaved serpins: comparison of alpha 1-proteinase inhibitor, alpha 1-antichymotrypsin, antithrombin III, alpha 2-antiplasmin, angiotensinogen, and ovalbumin. Biochemistry. 1991;30(6):1723–30.
Holmes WE, Nelles L, Lijnen HR, Collen D. Primary structure of human alpha 2-antiplasmin, a serine protease inhibitor (serpin). J Biol Chem. 1987;262(4):1659–64.
Lee KN, Jackson KW, Christiansen VJ, Chung KH, McKee PA. A novel plasma proteinase potentiates alpha2-antiplasmin inhibition of fibrin digestion. Blood. 2004;103(10):3783–8.
Bangert K, Johnsen AH, Christensen U, Thorsen S. Different N-terminal forms of alpha 2-plasmin inhibitor in human plasma. Biochem J. 1993;291(Pt 2):623–5.
Kimura S, Aoki N. Cross-linking site in fibrinogen for alpha 2-plasmin inhibitor. J Biol Chem. 1986;261(33):15591–5.
Booth NA. Regulation of fibrinolytic activity by localization of inhibitors to fibrin(ogen). Fibrinolysis Proteolysis. 2000;14(2–3):206–13.
Sumi Y, Ichikawa Y, Nakamura Y, Miura O, Aoki N. Expression and characterization of pro alpha 2-plasmin inhibitor. J Biochem. 1989;106(4):703–7.
Reed GL 3rd, Matsueda GR, Haber E. Synergistic fibrinolysis: combined effects of plasminogen activators and an antibody that inhibits alpha 2-antiplasmin. Proc Natl Acad Sci U S A. 1990;87(3):1114–8.
Clemmensen I, Thorsen S, Mullertz S, Petersen LC. Properties of three different molecular forms of the alpha 2 plasmin inhibitor. Eur J Biochem. 1981;120(1):105–12.
Sasaki T, Morita T, Iwanaga S. Identification of the plasminogen-binding site of human alpha 2-plasmin inhibitor. J Biochem. 1986;99(6):1699–705.
Collen D. On the regulation and control of fibrinolysis. Edward Kowalski Memorial Lecture. Thromb Haemost. 1980;43(2):77–89.
Frank PS, Douglas JT, Locher M, Llinas M, Schaller J. Structural/functional characterization of the alpha 2-plasmin inhibitor C-terminal peptide. Biochemistry. 2003;42(4):1078–85.
Lu BG, Sofian T, Law RH, Coughlin PB, Horvath AJ. Contribution of conserved lysine residues in the alpha2-antiplasmin C terminus to plasmin binding and inhibition. J Biol Chem. 2011;286(28):24544–52.
Wang H, Yu A, Wiman B, Pap S. Identification of amino acids in antiplasmin involved in its noncovalent ‘lysine-binding-site’-dependent interaction with plasmin. Eur J Biochem. 2003;270(9):2023–9.
Foley JH, Kim PY, Mutch NJ, Gils A. Insights into thrombin activatable fibrinolysis inhibitor function and regulation. J Thromb Haemost. 2013;11(Suppl 1):306–15.
Foley JH, Kim PY, Hendriks D, Morser J, Gils A, Mutch NJ, et al. Evaluation of and recommendation for the nomenclature of the CPB2 gene product (also known as TAFI and proCPU): communication from the SSC of the ISTH. J Thromb Haemost. 2015;13(12):2277–8.
Nesheim M. Fibrinolysis and the plasma carboxypeptidase. Curr Opin Hematol. 1998;5(5):309–13.
Bajzar L, Morser J, Nesheim M. TAFI, or plasma procarboxypeptidase B, couples the coagulation and fibrinolytic cascades through the thrombin-thrombomodulin complex. J Biol Chem. 1996;271(28):16603–8.
Mao SS, Cooper CM, Wood T, Shafer JA, Gardell SJ. Characterization of plasmin-mediated activation of plasma procarboxypeptidase B. Modulation by glycosaminoglycans. J Biol Chem. 1999;274(49):35046–52.
Bajzar L, Nesheim M, Morser J, Tracy PB. Both cellular and soluble forms of thrombomodulin inhibit fibrinolysis by potentiating the activation of thrombin-activable fibrinolysis inhibitor. J Biol Chem. 1998;273(5):2792–8.
Bouma BN, Marx PF, Mosnier LO, Meijers JC. Thrombin-activatable fibrinolysis inhibitor (TAFI, plasma procarboxypeptidase B, procarboxypeptidase R, procarboxypeptidase U). Thromb Res. 2001;101(5):329–54.
Boffa MB, Wang W, Bajzar L, Nesheim ME. Plasma and recombinant thrombin-activable fibrinolysis inhibitor (TAFI) and activated TAFI compared with respect to glycosylation, thrombin/thrombomodulin-dependent activation, thermal stability, and enzymatic properties. J Biol Chem. 1998;273(4):2127–35.
Leurs J, Wissing BM, Nerme V, Schatteman K, Bjorquist P, Hendriks D. Different mechanisms contribute to the biphasic pattern of carboxypeptidase U (TAFIa) generation during in vitro clot lysis in human plasma. Thromb Haemost. 2003;89(2):264–71.
Leurs J, Nerme V, Sim Y, Hendriks D. Carboxypeptidase U (TAFIa) prevents lysis from proceeding into the propagation phase through a threshold-dependent mechanism. J Thromb Haemost. 2004;2(3):416–23.
Zhao L, Morser J, Bajzar L, Nesheim M, Nagashima M. Identification and characterization of two thrombin-activatable fibrinolysis inhibitor isoforms. Thromb Haemost. 1998;80(6):949–55.
Brouwers GJ, Vos HL, Leebeek FW, Bulk S, Schneider M, Boffa M, et al. A novel, possibly functional, single nucleotide polymorphism in the coding region of the thrombin-activatable fibrinolysis inhibitor (TAFI) gene is also associated with TAFI levels. Blood. 2001;98(6):1992–3.
Morange PE, Aillaud MF, Nicaud V, Henry M, Juhan-Vague I. Ala147Thr and C+1542G polymorphisms in the TAFI gene are not associated with a higher risk of venous thrombosis in FV Leiden carriers. Thromb Haemost. 2001;86(6):1583–4.
Isordia-Salas I, Martinez-Marino M, Alberti-Minutti P, Ricardo-Moreno MT, Castro-Calvo R, Santiago-German D, et al. Genetic polymorphisms associated with thrombotic disease comparison of two territories: myocardial infarction and ischemic stroke. Dis Markers. 2019;2019:3745735.
Meltzer ME, Lisman T, de Groot PG, Meijers JC, le Cessie S, Doggen CJ, et al. Venous thrombosis risk associated with plasma hypofibrinolysis is explained by elevated plasma levels of TAFI and PAI-1. Blood. 2010;116(1):113–21.
Silveira A, Schatteman K, Goossens F, Moor E, Scharpe S, Stromqvist M, et al. Plasma procarboxypeptidase U in men with symptomatic coronary artery disease. Thromb Haemost. 2000;84(3):364–8.
Juhan-Vague I, Morange PE, Aubert H, Henry M, Aillaud MF, Alessi MC, et al. Plasma thrombin-activatable fibrinolysis inhibitor antigen concentration and genotype in relation to myocardial infarction in the north and south of Europe. Arterioscler Thromb Vasc Biol. 2002;22(5):867–73.
von dem Borne PA, Meijers JC, Bouma BN. Feedback activation of factor XI by thrombin in plasma results in additional formation of thrombin that protects fibrin clots from fibrinolysis. Blood. 1995;86(8):3035–42.
Kravtsov DV, Matafonov A, Tucker EI, Sun MF, Walsh PN, Gruber A, et al. Factor XI contributes to thrombin generation in the absence of factor XII. Blood. 2009;114(2):452–8.
Bouma BN, Meijers JC. Fibrinolysis and the contact system: a role for factor XI in the down-regulation of fibrinolysis. Thromb Haemost. 1999;82(2):243–50.
Broze GJ Jr, Higuchi DA. Coagulation-dependent inhibition of fibrinolysis: role of carboxypeptidase-U and the premature lysis of clots from hemophilic plasma. Blood. 1996;88(10):3815–23.
Wyseure T, Cooke EJ, Declerck PJ, Behrendt N, Meijers JCM, von Drygalski A, et al. Defective TAFI activation in hemophilia A mice is a major contributor to joint bleeding. Blood. 2018;132(15):1593–603.
Mosnier LO, Lisman T, van den Berg HM, Nieuwenhuis HK, Meijers JC, Bouma BN. The defective down regulation of fibrinolysis in haemophilia A can be restored by increasing the TAFI plasma concentration. Thromb Haemost. 2001;86(4):1035–9.
Minnema MC, Friederich PW, Levi M, von dem Borne PA, Mosnier LO, Meijers JC, et al. Enhancement of rabbit jugular vein thrombolysis by neutralization of factor XI. In vivo evidence for a role of factor XI as an anti-fibrinolytic factor. J Clin Invest. 1998;101(1):10–4.
Zucker M, Seligsohn U, Salomon O, Wolberg AS. Abnormal plasma clot structure and stability distinguish bleeding risk in patients with severe factor XI deficiency. J Thromb Haemost. 2014;12(7):1121–30.
Gidley GN, Holle LA, Burthem J, Bolton-Maggs PHB, Lin FC, Wolberg AS. Abnormal plasma clot formation and fibrinolysis reveal bleeding tendency in patients with partial factor XI deficiency. Blood Adv. 2018;2(10):1076–88.
Astedt B, Lecander I, Brodin T, Lundblad A, Low K. Purification of a specific placental plasminogen activator inhibitor by monoclonal antibody and its complex formation with plasminogen activator. Thromb Haemost. 1985;53(1):122–5.
Kruithof EK, Vassalli JD, Schleuning WD, Mattaliano RJ, Bachmann F. Purification and characterization of a plasminogen activator inhibitor from the histiocytic lymphoma cell line U-937. J Biol Chem. 1986;261(24):11207–13.
Risse BC, Brown H, Lavker RM, Pearson JM, Baker MS, Ginsburg D, et al. Differentiating cells of murine stratified squamous epithelia constitutively express plasminogen activator inhibitor type 2 (PAI-2). Histochem Cell Biol. 1998;110(6):559–69.
Dougherty KM, Pearson JM, Yang AY, Westrick RJ, Baker MS, Ginsburg D. The plasminogen activator inhibitor-2 gene is not required for normal murine development or survival. Proc Natl Acad Sci U S A. 1999;96(2):686–91.
Schwartz BS, Bradshaw JD. Differential regulation of tissue factor and plasminogen activator inhibitor by human mononuclear cells. Blood. 1989;74(5):1644–50.
Ritchie H, Robbie LA, Kinghorn S, Exley R, Booth NA. Monocyte plasminogen activator inhibitor 2 (PAI-2) inhibits u-PA-mediated fibrin clot lysis and is cross-linked to fibrin. Thromb Haemost. 1999;81(1):96–103.
Siefert SA, Chabasse C, Mukhopadhyay S, Hoofnagle MH, Strickland DK, Sarkar R, et al. Enhanced venous thrombus resolution in plasminogen activator inhibitor type-2 deficient mice. J Thromb Haemost. 2014;12(10):1706–16.
Kruithof EK, Tran-Thang C, Gudinchet A, Hauert J, Nicoloso G, Genton C, et al. Fibrinolysis in pregnancy: a study of plasminogen activator inhibitors. Blood. 1987;69(2):460–6.
Bonnar J, Daly L, Sheppard BL. Changes in the fibrinolytic system during pregnancy. Semin Thromb Hemost. 1990;16(3):221–9.
Reith A, Booth NA, Moore NR, Cruickshank DJ, Bennett B. Plasminogen activator inhibitors (PAI-1 and PAI-2) in normal pregnancies, pre-eclampsia and hydatidiform mole. Br J Obstet Gynaecol. 1993;100(4):370–4.
Grancha S, Estelles A, Gilabert J, Chirivella M, Espana F, Aznar J. Decreased expression of PAI-2 mRNA and protein in pregnancies complicated with intrauterine fetal growth retardation. Thromb Haemost. 1996;76(5):761–7.
Scherrer A, Kruithof EK, Grob JP. Plasminogen activator inhibitor-2 in patients with monocytic leukemia. Leukemia. 1991;5(6):479–86.
Robbie LA, Dummer S, Booth NA, Adey GD, Bennett B. Plasminogen activator inhibitor 2 and urokinase-type plasminogen activator in plasma and leucocytes in patients with severe sepsis. Br J Haematol. 2000;109(2):342–8.
Mueller BM, Yu YB, Laug WE. Overexpression of plasminogen activator inhibitor 2 in human melanoma cells inhibits spontaneous metastasis in scid/scid mice. Proc Natl Acad Sci U S A. 1995;92(1):205–9.
Varro A, Noble PJ, Pritchard DM, Kennedy S, Hart CA, Dimaline R, et al. Helicobacter pylori induces plasminogen activator inhibitor 2 in gastric epithelial cells through nuclear factor-kappaB and RhoA: implications for invasion and apoptosis. Cancer Res. 2004;64(5):1695–702.
Huisman LG, van Griensven JM, Kluft C. On the role of C1-inhibitor as inhibitor of tissue-type plasminogen activator in human plasma. Thromb Haemost. 1995;73(3):466–71.
Castellano G, Divella C, Sallustio F, Montinaro V, Curci C, Zanichelli A, et al. A transcriptomics study of hereditary angioedema attacks. J Allergy Clin Immunol. 2018;142(3):883–91.
Levi M, Roem D, Kamp AM, de Boer JP, Hack CE, ten Cate JW. Assessment of the relative contribution of different protease inhibitors to the inhibition of plasmin in vivo. Thromb Haemost. 1993;69(2):141–6.
Miles LA, Hawley SB, Baik N, Andronicos NM, Castellino FJ, Parmer RJ. Plasminogen receptors: the sine qua non of cell surface plasminogen activation. Front Biosci. 2005;10:1754–62.
Miles LA, Plow EF. Binding and activation of plasminogen on the platelet surface. J Biol Chem. 1985;260(7):4303–11.
Whyte CS, Swieringa F, Mastenbroek TG, Lionikiene AS, Lance MD, van der Meijden PE, et al. Plasminogen associates with phosphatidylserine-exposing platelets and contributes to thrombus lysis under flow. Blood. 2015;125(16):2568–78.
Miles LA, Parmer RJ. Plasminogen receptors: the first quarter century. Semin Thromb Hemost. 2013;39(4):329–37.
Cheng XF, Brohlin M, Pohl G, Back O, Wallen P. Binding of tissue plasminogen activator to endothelial cells. The effect on functional properties. Localization of a ligand in the B-chain of tPA. Thromb Res. 1995;77(2):149–64.
Razzaq TM, Bass R, Vines DJ, Werner F, Whawell SA, Ellis V. Functional regulation of tissue plasminogen activator on the surface of vascular smooth muscle cells by the type-II transmembrane protein p63 (CKAP4). J Biol Chem. 2003;278(43):42679–85.
Behrendt N, Ronne E, Dano K. The structure and function of the urokinase receptor, a membrane protein governing plasminogen activation on the cell surface. Biol Chem Hoppe Seyler. 1995;376(5):269–79.
Webb DJ, Nguyen DH, Gonias SL. Extracellular signal-regulated kinase functions in the urokinase receptor-dependent pathway by which neutralization of low density lipoprotein receptor-related protein promotes fibrosarcoma cell migration and matrigel invasion. J Cell Sci. 2000;113(Pt 1):123–34.
Wei Y, Yang X, Liu Q, Wilkins JA, Chapman HA. A role for caveolin and the urokinase receptor in integrin-mediated adhesion and signaling. J Cell Biol. 1999;144(6):1285–94.
Wienke D, MacFadyen JR, Isacke CM. Identification and characterization of the endocytic transmembrane glycoprotein Endo180 as a novel collagen receptor. Mol Biol Cell. 2003;14(9):3592–604.
Kjoller L, Engelholm LH, Hoyer-Hansen M, Dano K, Bugge TH, Behrendt N. uPARAP/endo180 directs lysosomal delivery and degradation of collagen IV. Exp Cell Res. 2004;293(1):106–16.
Ellis V. Functional analysis of the cellular receptor for urokinase in plasminogen activation. Receptor binding has no influence on the zymogenic nature of pro-urokinase. J Biol Chem. 1996;271(25):14779–84.
Nykjaer A, Conese M, Christensen EI, Olson D, Cremona O, Gliemann J, et al. Recycling of the urokinase receptor upon internalization of the uPA:serpin complexes. EMBO J. 1997;16(10):2610–20.
Ellis V, Scully MF, Kakkar VV. Plasminogen activation initiated by single-chain urokinase-type plasminogen activator. Potentiation by U937 monocytes. J Biol Chem. 1989;264(4):2185–8.
Manchanda N, Schwartz BS. Single chain urokinase. Augmentation of enzymatic activity upon binding to monocytes. J Biol Chem. 1991;266(22):14580–4.
Lee SW, Ellis V, Dichek DA. Characterization of plasminogen activation by glycosylphosphatidylinositol-anchored urokinase. J Biol Chem. 1994;269(4):2411–8.
Dejouvencel T, Doeuvre L, Lacroix R, Plawinski L, Dignat-George F, Lijnen HR, et al. Fibrinolytic cross-talk: a new mechanism for plasmin formation. Blood. 2010;115(10):2048–56.
Mitchell JL, Lionikiene AS, Fraser SR. Whyte CS. Mutch NJ. Functional factor XIII-A is exposed on the stimulated platelet surface. Blood: Booth NA; 2014.
Brogren H, Karlsson L, Andersson M, Wang L, Erlinge D, Jern S. Platelets synthesize large amounts of active plasminogen activator inhibitor 1. Blood. 2004;104(13):3943–8.
Morrow GB, Whyte CS, Mutch NJ. Functional plasminogen activator inhibitor 1 is retained on the activated platelet membrane following platelet activation. Haematologica. 2020.
Plow EF, Collen D. The presence and release of alpha 2-antiplasmin from human platelets. Blood. 1981;58(6):1069–74.
Schadinger SL, Lin JH, Garand M, Boffa MB. Secretion and antifibrinolytic function of thrombin-activatable fibrinolysis inhibitor from human platelets. J Thromb Haemost. 2010;8(11):2523–9.
Samson AL, Alwis I, Maclean JAA, Priyananda P, Hawkett B, Schoenwaelder SM, et al. Endogenous fibrinolysis facilitates clot retraction in vivo. Blood. 2017;130(23):2453–62.
Robbie LA, Bennett B, Croll AM, Brown PA, Booth NA. Proteins of the fibrinolytic system in human thrombi. Thromb Haemost. 1996;75(1):127–33.
Potter van Loon BJ, Rijken DC, Brommer EJ, van der Maas AP. The amount of plasminogen, tissue-type plasminogen activator and plasminogen activator inhibitor type 1 in human thrombi and the relation to ex-vivo lysibility. Thromb Haemost. 1992;67(1):101–5.
Mutch NJ, Robbie LA, Booth NA. Human thrombi contain an abundance of active thrombin. Thromb Haemost. 2001;86(4):1028–34.
Mutch NJ, Moir E, Robbie LA, Berry SH, Bennett B, Booth NA. Localization and identification of thrombin and plasminogen activator activities in model human thrombi by in situ zymography. Thromb Haemost. 2002;88(6):996–1002.
Moir E, Booth NA, Bennett B, Robbie LA. Polymorphonuclear leucocytes mediate endogenous thrombus lysis via a u-PA-dependent mechanism. Br J Haematol. 2001;113(1):72–80.
Moir E, Robbie LA, Bennett B, Booth NA. Polymorphonuclear leucocytes have two opposing roles in fibrinolysis. Thromb Haemost. 2002;87(6):1006–10.
Pluskota E, Soloviev DA, Bdeir K, Cines DB, Plow EF. Integrin alphaMbeta2 orchestrates and accelerates plasminogen activation and fibrinolysis by neutrophils. J Biol Chem. 2004;279(17):18063–72.
Singh I, Burnand KG, Collins M, Luttun A, Collen D, Boelhouwer B, et al. Failure of thrombus to resolve in urokinase-type plasminogen activator gene-knockout mice: rescue by normal bone marrow-derived cells. Circulation. 2003;107(6):869–75.
McGuinness CL, Humphries J, Waltham M, Burnand KG, Collins M, Smith A. Recruitment of labelled monocytes by experimental venous thrombi. Thromb Haemost. 2001;85(6):1018–24.
Humphries J, Gossage JA, Modarai B, Burnand KG, Sisson TH, Murdoch C, et al. Monocyte urokinase-type plasminogen activator up-regulation reduces thrombus size in a model of venous thrombosis. J Vasc Surg. 2009;50(5):1127–34.
Thorsen S. The mechanism of plasminogen activation and the variability of the fibrin effector during tissue-type plasminogen activator-mediated fibrinolysis. Ann N Y Acad Sci. 1992;667:52–63.
Rijken DC, Sakharov DV. Basic principles in thrombolysis: regulatory role of plasminogen. Thromb Res. 2001;103(Suppl 1):S41–9.
Longstaff C, Thelwell C, Williams SC, Silva MM, Szabo L, Kolev K. The interplay between tissue plasminogen activator domains and fibrin structures in the regulation of fibrinolysis: kinetic and microscopic studies. Blood. 2020.
Mutch NJ, Moore NR, Wang E, Booth NA. Thrombus lysis by uPA, scuPA and tPA is regulated by plasma TAFI. J Thromb Haemost. 2003;1(9):2000–7.
Gurewich V, Pannell R, Louie S, Kelley P, Suddith RL, Greenlee R. Effective and fibrin-specific clot lysis by a zymogen precursor form of urokinase (pro-urokinase). A study in vitro and in two animal species. J Clin Invest. 1984;73(6):1731–9.
Schwartz BS, Espana F. Two distinct urokinase-serpin interactions regulate the initiation of cell surface-associated plasminogen activation. J Biol Chem. 1999;274(21):15278–83.
Cointe S, Harti Souab K, Bouriche T, Vallier L, Bonifay A, Judicone C, et al. A new assay to evaluate microvesicle plasmin generation capacity: validation in disease with fibrinolysis imbalance. J Extracell Vesicles. 2018;7(1):1494482.
Mutch NJ, Koikkalainen JS, Fraser SR, Duthie KM, Griffin M, Mitchell J, et al. Model thrombi formed under flow reveal the role of factor XIII-mediated cross-linking in resistance to fibrinolysis. J Thromb Haemost. 2010;8(9):2017–24.
Rijken DC, Hoegee-de Nobel E, Jie AF, Atsma DE, Schalij MJ, Nieuwenhuizen W. Development of a new test for the global fibrinolytic capacity in whole blood. J Thromb Haemost. 2008;6(1):151–7.
Rijken DC, Kock EL, Guimaraes AH, Talens S, Darwish Murad S, Janssen HL, et al. Evidence for an enhanced fibrinolytic capacity in cirrhosis as measured with two different global fibrinolysis tests. J Thromb Haemost. 2012;10(10):2116–22.
Ratnoff OD. Some relationships among hemostasis, fibrinolytic phenomena, immunity, and the inflammatory response. Adv Immunol. 1969;10:145–227.
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2021 Springer Nature Switzerland AG
About this chapter
Cite this chapter
Mutch, N.J., Whyte, C.S. (2021). Physiology of Haemostasis: Plasmin-Antiplasmin System. In: Moore, H.B., Neal, M.D., Moore, E.E. (eds) Trauma Induced Coagulopathy. Springer, Cham. https://doi.org/10.1007/978-3-030-53606-0_5
Download citation
DOI: https://doi.org/10.1007/978-3-030-53606-0_5
Published:
Publisher Name: Springer, Cham
Print ISBN: 978-3-030-53605-3
Online ISBN: 978-3-030-53606-0
eBook Packages: MedicineMedicine (R0)