Abstract
Purpose
Chronic low back pain causes structural remodelling and inflammation in the multifidus muscle. Collagen expression is increased in the multifidus of humans with lumbar disc degeneration. However, the extent and mechanisms underlying the increased fibrotic activity in the multifidus are unknown. Physical activity reduces local inflammation that precedes multifidus fibrosis during intervertebral disc degeneration (IDD), but its effect on amelioration of fibrosis is unknown. This study aimed to assess the development of fibrosis and its underlying genetic network during IDD and the impact of physical activity.
Methods
Wild-type and SPARC-null mice were either sedentary or housed with a running wheel, to allow voluntary physical activity. At 12 months of age, IDD was assessed with MRI, and multifidus muscle samples were harvested from L2 to L6. In SPARC-null mice, the L1/2 and L3/4 discs had low and high levels of IDD, respectively. Thus, multifidus samples from L2 and L4 were allocated to low- and high-IDD groups compared to assess the effects of IDD and physical activity on connective tissue and fibrotic genes.
Results
High IDD was associated with greater connective tissue thickness and dysregulation of collagen-III, fibronectin, CTGF, substance P, TIMP1 and TIMP2 in the multifidus muscle. Physical activity attenuated the IDD-dependent increased connective tissue thickness and reduced the expression of collagen-I, fibronectin, CTGF, substance P, MMP2 and TIMP2 in SPARC-null animals and wild-type mice. Collagen-III and TIMP1 were only reduced in wild-type animals.
Conclusions
These data reveal the fibrotic networks that promote fibrosis in the multifidus muscle during chronic IDD. Furthermore, physical activity is shown to reduce fibrosis and regulate the fibrotic gene network.
Graphical abstract
These slides can be retrieved under Electronic Supplementary Material.
Similar content being viewed by others
Avoid common mistakes on your manuscript.
Introduction
Low back pain (LBP) is the leading cause of disability internationally [1]. Treatment effects remain limited in part because the underlying mechanisms are multifactorial and vary in a time-dependant manner from the onset of injury to chronic stages [2,3,4]. Exercise is among the most efficacious treatments [5, 6], but incomplete understanding of the therapeutic mechanisms limits its targeted application.
LBP is accompanied by structural changes in the muscles that surround the spine, particularly the multifidus muscle [2, 7,8,9,10,11,12,13]. Localised acute atrophy [8] and then adipose accumulation (without atrophy) [14] in sub-acute LBP, followed by diffuse atrophy, fibrosis and adiposity in chronic LBP [15], have been identified in human studies. Ovine studies have shown increased cross-sectional area of connective tissue and expression of collagen-I (Col-I) in the multifidus during early chronic LBP [2]. These changes are characteristic of tissue fibrosis, which is a hallmark feature of various musculoskeletal conditions, and are associated with declines in sensory and motor function [16, 17], and once established, recovery is slow [18]. The extent and underlying mechanisms of fibrotic changes to the multifidus muscle during LBP are poorly characterised and require further investigation.
Connective tissue is highly adaptive and involves a delicate balance between extracellular matrix (ECM) synthesis and degradation [19, 20]. This balance is regulated by complex molecular networks (Fig. 1). Collagen synthesis is promoted by the upregulation of molecules such as transforming growth factor beta 1 (TGF-β1) [21, 22], connective tissue growth factor (CTGF) [23, 24], secreted protein acidic and rich in cysteine (SPARC) [25] and substance P (SP) [26, 27]. SP also has anti-fibrotic properties [28]. Collagen degradation is promoted by molecules including members of the matrix metalloproteinase (MMPs) family, which are in turn inhibited by tissue inhibitor of metalloproteinases (TIMPs) [29]. Although other molecules are involved, these networks are highly responsive to injury/pathology, and their dysregulation is a primary driver of fibrotic alterations in various tissues (e.g. skeletal muscle [29], liver [30], heart [31]).
Physical activity is a potent regulator of connective tissue in skeletal muscle [20, 32]. Short-term (acute) exercise stimulates both collagen synthesis and degradation to assist in its remodelling [33, 34], and long-term exercise prevents ageing-dependent fibrosis [35, 36]. The potential for exercise to reduce systemic and local inflammation [37,38,39,40,41] may partly explain its anti-fibrotic effect. In a model of LBP, physical activity attenuated increased pro-inflammatory cytokines and adipokines in multifidus associated with intervertebral disc degeneration (IDD) [42]. As inflammation precedes fibrosis, the anti-inflammatory effects of exercise highlight a possible pathway to prevent and/or reverse fibrotic changes.
This study addresses two issues. First, evidence for muscle fibrotic with IDD is derived from experimentally induced intervertebral disc (IVD) lesions. Whether similar processes accompany spontaneous IDD is unclear. Second, whether exercise ameliorates the fibrotic response is untested. These questions can be explored using a SPARC-null mouse model that develops spontaneous IDD, as we have previously described [42]. SPARC is required for ECM remodelling, and its absence results in spontaneous age-dependent IDD [43,44,45,46,47]. These animals provide an ideal model to explore: (1) whether fibrosis occurs during IDD, (2) whether the fibrotic gene network within multifidus are dysregulated in spontaneous IDD, (3) whether chronic physical activity ameliorates this dysregulation, and (4) the relationships between these genes.
Materials and methods
Experimental design
As SPARC has a pro-fibrotic role, we assessed the effects of IDD on fibrosis in the multifidus by comparison of a region of multifidus rostral to an IVD that consistently presented with IDD (adjacent to L4; 15 out of 16 had IDD in the L3/4 IVD) in SPARC mice against a region of multifidus rostral to an IVD with no/low levels of IDD (adjacent to L2; 3 of 16 had IDD in the L1/2 IVD) in the same mice, rather than use wild-type (WT) mice (Fig. 2a). The effect of physical activity on fibrotic networks in the multifidus were assessed in two ways: (1) using SPARC-null mice to examine the effect of physical activity on IDD-dependent alterations and (2) using WT mice (multifidus adjacent to L4 with no evidence of IDD.) to test the effects of physical activity in mice with a normal fibrotic network.
Animals and sample collection
All in vivo experiments were conducted with the approval of the faculty animal care committee at McGill University. Sixteen SPARC-null and 17 age-matched WT animals were used. The SPARC-null mice were developed on a mixed C57BL/6 × 129 SVJ background and backcrossed onto a standard C57BL/6 line for enough generations to be considered fully congenic [54]. Mice were housed with two-to-three littermates and separated into two groups: physical activity (PA) and sedentary (Sed). From 8 months of age, PA mice were housed with an Innowheel (Bio-serv, NJ, USA) that provided housing and a wheel for voluntary exercise. Voluntary exercise was selected to avoid stress-related problems and changes in circadian rhythm associated with forced exercise [48, 49]. Housing for the Sed animals was identical except the wheel was fixed in place with a screw preventing rotation and therefore unusable for voluntary exercise. At 12 months of age, IDD was assessed using MRI (see [42]). Multifidus muscle samples (L2–L6) were harvested adjacent to the spinous processes from the left and right sides and were stored in RNA later at − 20 °C or fixed overnight in 4% paraformaldehyde, then stored in 30% sucrose in phosphate-buffered saline. Fixed tissue was sectioned at 20 μm and mounted onto Superfrost Plus slides (Thermofisher) and stored at − 20 °C.
Van Gieson’s stain
Slides containing multifidus muscle from L2 (non-IDD) and L4 (IDD) were incubated in running water for 2 min, Weigert’s haematoxylin for 10 min and Van Gieson’s solution for 1 min before dehydration and mounting. Slides were imaged (ImageScope, Leica), and thickness of the connective tissue separating the multifidus and adjacent longissimus muscles was measured (Fig. 2b) (ImageJ software, NIH).
Immunofluorescence assay
Multifidus muscle sections on slides from L2 and L4 were immersed in acetone for 10 min, blocked in 5% bovine serum albumin (Sigma) and incubated overnight at 4 °C with anti-collagen 1 (1:400, AB6308, Abcam). Sections were incubated for 1 h at room temperature with goat anti-mouse IgG1 conjugated to FITC (1:1000, AB97239, Abcam) and mounted with Fluroshield mounting medium (AB104139, Abcam). The area positive for Col-I expression was measured and divided by the total muscle fibre area using ImageJ software (NIH) (Fig. 2c).
Quantitative polymerase chain reaction (qPCR) assay
RNA extraction, cDNA synthesis and qPCRs were performed as previously described [42]. Primer pairs are listed in Table 1. We quantified gene expression of the ECM components [Col-I, III, IV and fibronectin (Fn)], as well as molecules involved with collagen synthesis (SP, CTGF) and collagen degradation (MMP2, MMP9, TIMP1 and TIMP2). GAPDH was used as a housekeeping gene.
Statistical analysis
The role of IDD on fibrosis in the multifidus was tested by comparison of high- and low-IDD samples (low IDD vs. high IDD) and activity levels (Sed vs. PA) in SPARC-null animals using a two-way ANOVA and Duncan’s post hoc analyses. A one-way ANOVA tested the effect of exercise (PA vs. Sed) for WT mice. Pearson’s correlation was used to evaluate relationships between fibrotic and ECM gene expression in low-IDD and high-IDD groups from SPARC-null animals. Coefficients were interpreted as weak (0.3–0.5), moderate (0.5–0.7) or strong (0.7–1). Significance was set at P < 0.05. All data are presented as mean ± SEM. Statistica (StatSoft, USA) was used for all statistical analysis.
Results
Effect of IDD and physical activity on connective tissue
Connective tissue (CT) separating the multifidus and longissimus muscles (epimysium) was significantly thicker in L4 multifidus (high-IDD group) than at L2 (low-IDD group; Table 2, Fig. 3). Long-term exposure to physical activity reduced CT thickness in both SPARC-null and WT mice (Table 2, Fig. 3). Immunofluorescence staining for Col-I showed limited expression in the epimysium, and IDD or PA did not affect the area of Col-I as a percentage of the multifidus (Table 2, Fig. 3).
Effect of IDD and physical activity on ECM genes
Consistent with the impact of injury on fibrosis, Col-III gene expression was significantly higher in the multifidus at the high- than low-IDD levels (Table 3, Fig. 4). Dysregulation of ECM was also evidenced by lower Fn expression at the high-IDD level (Table 3, Fig. 4). Consistent with histological findings (above), IDD had no effect on Col-I or Col-IV expression (Table 3, Fig. 4). Physical activity had an opposite effect on Col-III in WT mice (lower in the PA than Sed group), but no effect in SPARC-null mice. Physical activity also lowered Col-I and Fn, but not Col-IV, in SPARC-null and WT mice (Table 3, Fig. 4).
Effect of IDD and physical activity on the fibrotic gene network
CTGF expression was significantly higher at the high- than at low-IDD levels in both Sed and PA groups (Table 4, Fig. 5). Physical activity attenuated the elevation of CTGF expression associated with high IDD in SPARC-null mice (Table 4, Fig. 5).
SP, TIMP1 and TIMP2 were significantly lower in the multifidus at high- than at low-IDD levels (Table 4, Fig. 5). In contrast, MMP2 and MMP9 expression were not altered by IDD (Table 4, Fig. 5). Physical activity reduced the expression of SP and MMP2 in WT and SPARC-null mice. TIMP1 and TIMP2 were reduced by physical activity in WT and SPARC-null mice, respectively (Table 4, Fig. 5).
Correlations between fibrotic and ECM gene expression in SPARC-null animals
CTGF, Col-I and Col-III, were moderately positively correlated in the SPARC-null animals (Table 5). SP, MMP2, TIMP1, TIMP2 and Fn displayed moderate or greater relationships with each other gene (Table 5). Col-IV was positively correlated with Col-III, SP, MMP2 and TIMP1 (Table 5). MMP9 was not significantly correlated with any gene (Table 5).
Discussion
These results provide several new insights into the role of IDD in multifidus muscle fibrosis and the impact of physical activity. First, fibrosis (i.e. increased thickness of the CT between the multifidus and longissimus muscles) was present in muscle that crossed a degenerated disc. Second, expression of Col-III was higher, but Fn was lower in the multifidus at the high-IDD level. Third, the fibrotic gene network (CTGF, SP, TIMP1 and TIMP2) was dysregulated in multifidus crossing a degenerated disc and correlated with changes in ECM gene expression. Fourth, physical activity attenuated IDD-dependent increases in CTGF expression but not Col-III, and reduced Col-1, Fn, SP and MMP2 expression in WT and SPARC-null mice.
IDD is associated with multifidus fibrosis
Fibrotic changes in the multifidus are reported in chronic LBP [15] and in sub-acute/early chronic LBP following surgically induced IVD injury [2]. This study shows similar processes after spontaneous IDD and identifies candidate mechanisms that drive it.
Increased CT thickness between the multifidus and longissimus muscles in our model is consistent with results from an Ovine model of IDD. Those data showed increased CT in the multifidus during the sub-acute/early chronic period [2]. Consistent with our findings, that increase appeared limited to the outer sheath surrounding the muscle (epimysium). Increased epimysium thickness might increase multifidus muscle stiffness and alter the distribution of forces after IVD injury [50]. Further research is required to understand the clinical implications of the altered multifidus muscle CT.
Although histological findings from studies of different species are somewhat similar, the ECM genes that are dysregulated with IDD appear to differ. Here, Col-III and Fn expression, but not Col-I, is affected with IDD (Fig. 6a). Conversely, in the aforementioned Ovine model, Col-I was upregulated, whereas Col-III expression was independent of IDD [2]. In humans with lumbar IVD herniation, Col-I, Col-III and Fn are upregulated in the multifidus compared to controls [51]. These differences highlight the variable nature of fibrosis associated with IDD and that treatments cannot be tailored until this is understood.
Reduced Fn expression with IDD could have an important impact on multifidus muscle health because it is required to maintain and regenerate muscle stem cells [52]. Fn expression and the regenerative capacity of muscle decline with age, but the reintroduction of Fn expression in aged muscle restores its regenerative ability to levels comparable to young animals [52]. Hence, loss of Fn expression might reduce the capacity of muscle stem cells to regenerate damaged tissue in the multifidus, contributing to its degeneration in chronic LBP.
IDD is associated with changes to the genetic networks that drive fibrosis
CTGF is a major driver of fibrosis in various tissues [23, 24, 53] and musculoskeletal conditions [24, 54]. Its increase during IDD and positive relationship with Col-I and Col-III support this role in the multifidus during chronic LBP (Fig. 6a). Although CTGF expression is reported to be regulated by TGF-β1 [55], SPARC [56] and/or SP [57], its upregulation here was not correlated with TGF-β1 or SP, and it remained elevated in the absence of SPARC. One explanation is that CTGF is regulated differently during IDD. CTGF is a highly stress-responsive gene and is markedly upregulated during mechanical stress without accompanying increases in TGF-β1 and SP [58, 59]. It is therefore possible that changes in the mechanical forces in local tissues as a result of IDD could upregulate CTGF independent of TGF-β1 or SP.
SP is a neuropeptide that traditionally produces a strong pro-fibrotic function [17, 26, 27, 57], has a key role in nociception [60] and is upregulated in painful diseases such as fibromyalgia [61]. There is also contrasting evidence that it has anti-fibrotic [28] and anti-nociceptive [62] functions in muscle. The relationships between SP, MMP2, TIMP1 and TIMP2 suggest that SP plays a role in regulation of collagen degradation during IDD. Reduced SP expression could lower collagen degradation leading to its accumulation and subsequent fibrosis. Conversely, its reported anti-fibrotic function involves inhibition of collagen synthesis [28]. The potential anti-fibrotic role of SP in promoting collagen degradation and subsequent turnover requires investigation.
Physical activity regulates fibrosis
Acute and long-term exercise alters the ECM [20, 32, 63]. Effects of physical activity on the ECM depend on the activity type and duration, and demographics of the study population, e.g. age [63]. Our model of long-term physical activity (3 months of voluntary aerobic exercise in middle-aged mice) sheds new light onto the role of physical activity in regulating CT in healthy and chronic IDD groups.
Physical activity attenuated IDD-dependent fibrosis by reducing epimysium thickness. However, physical activity had no effect on IDD-dependent increases in Col-III expression in SPARC-null animals, despite a decrease in Col-III expression in WT mice. This reveals that although physical activity is capable of regulating Col-III expression, it is unable to attenuate Col-III expression associated with IDD. This could indicate that although physical activity attenuates increased epimysium thickness after IDD, it does not prevent changes to the underlying ECM components. This may impact the mechanics of the CT, and subsequently the multifidus. More detailed examination of the collagen components of the epimysium, perimysium and endomysium during IDD and physical activity are required.
Reduced CTGF following long-term exercise is a likely mechanism to explain the effectiveness of physical activity in attenuating fibrosis (Fig. 6b). Inhibition of CTGF ameliorates fibrosis and inflammation in a mouse model of Duchenne muscular dystrophy [64]. Further investigation of treatments targeting CTGF during chronic LBP requires investigation.
Exercise prevents ageing-dependent fibrotic changes in skeletal muscle [65,66,67], but this is based on studies that compare young and old animals [35, 65]. Mice in this study are considered middle age (38–47 in human years [68]). We show that exercise reduced the quantity of CT and ECM genes in middle-aged WT mice (Fig. 6b). This is suggestive of age-dependent fibrosis attenuation and requires further investigation. Taken together, exercise appears to be a potent regulator of the ECM in the multifidus muscle and is a promising treatment option due to its ability to attenuate fibrotic changes.
Methodological considerations
As supported by our data, SPARC is a pro-fibrotic molecule [25] (Fig. 1). To control for the potential influence of SPARC on our findings, analyses with respect to fibrosis were performed by limiting comparisons to multifidus muscle within the same SPARC-null mice, but in muscle rostral to IVDs with high IDD versus low IDD. The influence of the absence of SPARC on interactions in the fibrosis network requires consideration.
Conclusions
This study has provided novel data on the extent and nature of the fibrosis in the multifidus muscle in association with IDD. Further, we identified a range of biomarkers, such as CTGF, that could be targeted to improve muscle health and outcomes in individuals with IDD and chronic LBP. Our data build on evidence for the positive impact of physical activity in the prevention/treatment of age- and IDD-dependent fibrosis of the multifidus muscle.
References
Hoy D, March L, Brooks P et al (2014) The global burden of low back pain: estimates from the Global Burden of Disease 2010 study. Ann Rheum Dis 73:968–974
Hodges PW, James G, Blomster L et al (2015) Multifidus muscle changes after back injury are characterized by structural remodeling of muscle, adipose and connective tissue, but not muscle atrophy: molecular and morphological evidence. Spine 40:1057–1071
Klyne DM, Barbe MF, Hodges PW (2017) Systemic inflammatory profiles and their relationships with demographic, behavioural and clinical features in acute low back pain. Brain Behav Immun 60:84–92
Klyne DM, Barbe MF, van den Hoorn W et al (2018) ISSLS PRIZE IN CLINICAL SCIENCE 2018: longitudinal analysis of inflammatory, psychological, and sleep-related factors following an acute low back pain episode-the good, the bad, and the ugly. Eur Spine J 27:763–777
Gordon R, Bloxham S (2016) A systematic review of the effects of exercise and physical activity on non-specific chronic low back pain. Healthcare 4:22
Searle A, Spink M, Ho A et al (2015) Exercise interventions for the treatment of chronic low back pain: a systematic review and meta-analysis of randomised controlled trials. Clin Rehabil 29:1155–1167
Danneels LA, Vanderstraeten GG, Cambier DC et al (2000) CT imaging of trunk muscles in chronic low back pain patients and healthy control subjects. Eur Spine J 9:266–272
Hides J, Gilmore C, Stanton W et al (2008) Multifidus size and symmetry among chronic LBP and healthy asymptomatic subjects. Man Ther 13:43–49
Hides JA, Stokes MJ, Saide M et al (1994) Evidence of lumbar multifidus muscle wasting ipsilateral to symptoms in patients with acute/subacute low back pain. Spine 19:165–172
Hodges P, Holm AK, Hansson T et al (2006) Rapid atrophy of the lumbar multifidus follows experimental disc or nerve root injury. Spine 31:2926–2933
Hodges PW, James G, Blomster L et al (2014) Can proinflammatory cytokine gene expression explain multifidus muscle fiber changes after an intervertebral disc lesion? Spine 39:1010–1017
James G, Blomster L, Hall L et al (2016) Mesenchymal stem cell treatment of intervertebral disc lesion prevents fatty infiltration and fibrosis of the multifidus muscle, but not cytokine and muscle fiber changes. Spine 41:1208–1217
Kjaer P, Bendix T, Sorensen JS et al (2007) Are MRI-defined fat infiltrations in the multifidus muscles associated with low back pain? BMC Med 5:2
Battie MC, Niemelainen R, Gibbons LE et al (2012) Is level- and side-specific multifidus asymmetry a marker for lumbar disc pathology? Spine J 12:932–939
Zhao WP, Kawaguchi Y, Matsui H et al (2000) Histochemistry and morphology of the multifidus muscle in lumbar disc herniation: comparative study between diseased and normal sides. Spine 25:2191–2199
Abdelmagid SM, Barr AE, Rico M et al (2012) Performance of repetitive tasks induces decreased grip strength and increased fibrogenic proteins in skeletal muscle: role of force and inflammation. PLoS ONE 7:e38359
Fisher PW, Zhao Y, Rico MC et al (2015) Increased CCN2, substance P and tissue fibrosis are associated with sensorimotor declines in a rat model of repetitive overuse injury. J Cell Commun Signal 9:37–54
Stauber WT, Smith CA, Miller GR et al (2000) Recovery from 6 weeks of repeated strain injury to rat soleus muscles. Muscle Nerve 23:1819–1825
McAnulty RJ, Laurent GJ (1987) Collagen synthesis and degradation in vivo. Evidence for rapid rates of collagen turnover with extensive degradation of newly synthesized collagen in tissues of the adult rat. Collagen Relat Res 7:93–104
Kjaer M (2004) Role of extracellular matrix in adaptation of tendon and skeletal muscle to mechanical loading. Physiol Rev 84:649–698
Ignotz RA, Massague J (1986) Transforming growth factor-beta stimulates the expression of fibronectin and collagen and their incorporation into the extracellular matrix. J Biol Chem 261:4337–4345
Lijnen P, Petrov V (2002) Transforming growth factor-beta 1-induced collagen production in cultures of cardiac fibroblasts is the result of the appearance of myofibroblasts. Methods Find Exp Clin Pharmacol 24:333–344
Lipson KE, Wong C, Teng Y et al (2012) CTGF is a central mediator of tissue remodeling and fibrosis and its inhibition can reverse the process of fibrosis. Fibrogenes Tissue Repair 5:S24
Morales MG, Cabello-Verrugio C, Santander C et al (2011) CTGF/CCN-2 over-expression can directly induce features of skeletal muscle dystrophy. J Pathol 225:490–501
Trombetta-Esilva J, Bradshaw AD (2012) The function of SPARC as a mediator of fibrosis. Open Rheumatol J 6:146–155
Koon HW, Shih D, Karagiannides I et al (2010) Substance P modulates colitis-associated fibrosis. Am J Pathol 177:2300–2309
Wan Y, Meng F, Wu N et al (2017) Substance P increases liver fibrosis by differential changes in senescence of cholangiocytes and hepatic stellate cells. Hepatology 66:528–541
Yang Z, Zhang X, Guo N et al (2016) Substance P inhibits the collagen synthesis of rat myocardial fibroblasts induced by Ang II. Med Sci Monit Int Med J Exp Clin Res 22:4937–4946
Alameddine HS, Morgan JE (2016) Matrix metalloproteinases and tissue inhibitor of metalloproteinases in inflammation and fibrosis of skeletal muscles. J Neuromuscul Dis 3:455–473
Duarte S, Baber J, Fujii T et al (2015) Matrix metalloproteinases in liver injury, repair and fibrosis. Matrix Biol J Int Soc Matrix Biol 44–46:147–156
Daniels A, van Bilsen M, Goldschmeding R et al (2009) Connective tissue growth factor and cardiac fibrosis. Acta Physiol 195:321–338
Kjaer M, Magnusson P, Krogsgaard M et al (2006) Extracellular matrix adaptation of tendon and skeletal muscle to exercise. J Anat 208:445–450
Miller BF, Olesen JL, Hansen M et al (2005) Coordinated collagen and muscle protein synthesis in human patella tendon and quadriceps muscle after exercise. J Physiol 567:1021–1033
Moerch L, Pingel J, Boesen M et al (2013) The effect of acute exercise on collagen turnover in human tendons: influence of prior immobilization period. Eur J Appl Physiol 113:449–455
Kwak HB, Kim JH, Joshi K et al (2011) Exercise training reduces fibrosis and matrix metalloproteinase dysregulation in the aging rat heart. FASEB J 25:1106–1117
Wright KJ, Thomas MM, Betik AC et al (2014) Exercise training initiated in late middle age attenuates cardiac fibrosis and advanced glycation end-product accumulation in senescent rats. Exp Gerontol 50:9–18
Astrom MB, Feigh M, Pedersen BK (2010) Persistent low-grade inflammation and regular exercise. Front Biosci (Sch Ed) 2:96–105
Brandt C, Pedersen BK (2010) The role of exercise-induced myokines in muscle homeostasis and the defense against chronic diseases. J Biomed Biotechnol 2010:520258
Gleeson M, Bishop NC, Stensel DJ et al (2011) The anti-inflammatory effects of exercise: mechanisms and implications for the prevention and treatment of disease. Nat Rev Immunol 11:607–615
Pedersen BK (2017) Anti-inflammatory effects of exercise: role in diabetes and cardiovascular disease. Eur J Clin Investig 47:600–611
Petersen AM, Pedersen BK (2005) The anti-inflammatory effect of exercise. J Appl Physiol 98:1154–1162
James G, Millecamps M, Stone LS et al (2018) Dysregulation of the inflammatory mediators in the multifidus muscle after spontaneous intervertebral disc degeneration SPARC-null mice is ameliorated by physical activity. Spine 43:E1184–E1194
Millecamps M, Czerminski JT, Mathieu AP et al (2015) Behavioral signs of axial low back pain and motor impairment correlate with the severity of intervertebral disc degeneration in a mouse model. Spine J 15:2524–2537
Millecamps M, Tajerian M, Naso L et al (2012) Lumbar intervertebral disc degeneration associated with axial and radiating low back pain in ageing SPARC-null mice. Pain 153:1167–1179
Millecamps M, Tajerian M, Sage EH et al (2011) Behavioral signs of chronic back pain in the SPARC-null mouse. Spine 36:95–102
Miyagi M, Millecamps M, Danco AT et al (2014) ISSLS prize winner: increased innervation and sensory nervous system plasticity in a mouse model of low back pain due to intervertebral disc degeneration. Spine 39:1345–1354
Tajerian M, Alvarado S, Millecamps M et al (2011) DNA methylation of SPARC and chronic low back pain. Mol Pain 7:65
Moraska A, Deak T, Spencer RL et al (2000) Treadmill running produces both positive and negative physiological adaptations in Sprague-Dawley rats. Am J Physiol Regul Integr Comp Physiol 279:R1321–R1329
Girard I, Garland T Jr (2002) Plasma corticosterone response to acute and chronic voluntary exercise in female house mice. J Appl Physiol 92:1553–1561
Brown SH, Gregory DE, Carr JA et al (2011) ISSLS prize winner: adaptations to the multifidus muscle in response to experimentally induced intervertebral disc degeneration. Spine 36:1728–1736
Lehto M, Hurme M, Alaranta H et al (1989) Connective tissue changes of the multifidus muscle in patients with lumbar disc herniation. An immunohistologic study of collagen types I and III and fibronectin. Spine 14:302–309
Lukjanenko L, Jung MJ, Hegde N et al (2016) Loss of fibronectin from the aged stem cell niche affects the regenerative capacity of skeletal muscle in mice. Nat Med 22:897–905
Ramazani Y, Knops N, Elmonem MA et al (2018) Connective tissue growth factor (CTGF) from basics to clinics. Matrix Biol J Int Soc Matrix Biol 68–69:44–66
Song Y, Yao S, Liu Y et al (2017) Expression levels of TGF-beta1 and CTGF are associated with the severity of Duchenne muscular dystrophy. Exp Ther Med 13:1209–1214
Cicha I, Goppelt-Struebe M (2009) Connective tissue growth factor: context-dependent functions and mechanisms of regulation. BioFactors 35:200–208
Zhou XD, Xiong MM, Tan FK et al (2006) SPARC, an upstream regulator of connective tissue growth factor in response to transforming growth factor beta stimulation. Arthritis Rheum 54:3885–3889
Frara N, Fisher PW, Zhao Y et al (2018) Substance P increases CCN2 dependent on TGF-beta yet collagen type I via TGF-beta1 dependent and independent pathways in tenocytes. Connect Tissue Res 59:30–44
Chaqour B, Goppelt-Struebe M (2006) Mechanical regulation of the Cyr61/CCN1 and CTGF/CCN2 proteins. FEBS J 273:3639–3649
Schild C, Trueb B (2002) Mechanical stress is required for high-level expression of connective tissue growth factor. Exp Cell Res 274:83–91
Takahasi K, Sakurada T, Sakurada S et al (1987) Behavioural characterization of substance P-induced nociceptive response in mice. Neuropharmacology 26:1289–1293
Russell IJ (1998) Neurochemical pathogenesis of fibromyalgia. Z Rheumatol 57(Suppl 2):63–66
Lin CC, Chen WN, Chen CJ et al (2012) An antinociceptive role for substance P in acid-induced chronic muscle pain. Proc Natl Acad Sci USA 109:E76–E83
Martinez-Huenchullan S, McLennan SV, Verhoeven A et al (2017) The emerging role of skeletal muscle extracellular matrix remodelling in obesity and exercise. Obes Rev 18:776–790
Morales MG, Gutierrez J, Cabello-Verrugio C et al (2013) Reducing CTGF/CCN2 slows down mdx muscle dystrophy and improves cell therapy. Hum Mol Genet 22:4938–4951
Guzzoni V, Ribeiro MBT, Lopes GN et al (2018) Effect of resistance training on extracellular matrix adaptations in skeletal muscle of older rats. Front Physiol 9:374
Gosselin LE, Adams C, Cotter TA et al (1998) Effect of exercise training on passive stiffness in locomotor skeletal muscle: role of extracellular matrix. J Appl Physiol 85:1011–1016
Koskinen SO, Ahtikoski AM, Komulainen J et al (2002) Short-term effects of forced eccentric contractions on collagen synthesis and degradation in rat skeletal muscle. Pflugers Arch Eur J Physiol 444:59–72
Dutta S, Sengupta P (2016) Men and mice: relating their ages. Life Sci 152:244–248
Acknowledgements
This research was funded by the National Health and Medical Research Council (NHMRC) of Australia (Program Grant: APP1091302) and Canadian Health Institutes operating Grants MOP–102586 to LSS and MM. PWH supported by NHMRC Fellowship (APP1102905).
Author information
Authors and Affiliations
Corresponding author
Ethics declarations
Conflict of interest
There are no conflicts of interest related to this work.
Additional information
Publisher's Note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Electronic supplementary material
Below is the link to the electronic supplementary material.
Rights and permissions
About this article
Cite this article
James, G., Klyne, D.M., Millecamps, M. et al. ISSLS Prize in Basic science 2019: Physical activity attenuates fibrotic alterations to the multifidus muscle associated with intervertebral disc degeneration. Eur Spine J 28, 893–904 (2019). https://doi.org/10.1007/s00586-019-05902-9
Received:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1007/s00586-019-05902-9