- Research article
- Open Access
Increased caveolin-1 in intervertebral disc degeneration facilitates repair
Arthritis Research & Therapy volume 18, Article number: 59 (2016)
Preceding intervertebral disc (IVD) degeneration, the cell phenotype in the nucleus pulposus (NP) shifts from notochordal cells (NCs) to chondrocyte-like cells (CLCs). Microarray analysis showed a correlation between caveolin-1 expression and the phenotypic transition of NCs to CLCs. With a clinical directive in mind, the aim of this study was to determine the role of caveolin-1 in IVD degeneration. As a scaffolding protein, caveolin-1 influences several signaling pathways, and transforming growth factor (TGF)-β receptors have been demonstrated to colocalize with caveolin-1. Therefore, the hypothesis of this study was that caveolin-1 facilitates repair by enhancing TGF-β signaling in the IVD.
Protein expression (caveolin-1, apoptosis, progenitor cell markers, extracellular matrix, and phosphorylated Smad2 [pSmad2]) was determined in IVDs of wild-type (WT) and caveolin-1-null mice and canine IVDs of different degeneration grades (immunofluorescence, immunohistochemistry, and TUNEL assay). Canine/human CLC microaggregates were treated with chondrogenic medium alone or in combination with caveolin-1 scaffolding domain (CSD) peptide and/or caveolin-1 silencing RNA. After 28 days, gene and protein expression profiles were determined.
The NP of WT mice was rich in viable NCs, whereas the NP of caveolin-1-null mice contained more collagen-rich extracellular matrix and fewer cells, together with increased progenitor cell marker expression, pSmad2 TGF-β signaling, and high apoptotic activity. During canine IVD degeneration, caveolin-1 expression and apoptotic activity increased. In vitro caveolin-1 silencing decreased the CLC microaggregate glycosaminoglycan (GAG) content, which could be rescued by CSD treatment. Furthermore, CSD increased TGF-β/pSmad2 signaling at gene and protein expression levels and enhanced the anabolic effects of TGF-β1, reflected in increased extracellular matrix deposition by the CLCs.
Caveolin-1 plays a role in preservation of the NC phenotype. Additionally, it may be related to CLC apoptosis, given its increased expression in degenerated IVDs. Nevertheless, CSD enhanced CLC GAG deposition in vitro, and hence the increased caveolin-1 expression during IVD degeneration may also facilitate an ultimate attempt at repair. Further studies are needed to investigate how caveolin-1 modifies other signaling pathways and facilitates IVD repair.
Low back pain has been identified as one of the highest burden conditions by the World Health Organization and is the most common type of pain restricting daily activity . Low back pain is strongly related to intervertebral disc (IVD) degeneration . The IVD consists of a central nucleus pulposus (NP) and outer annulus fibrosus. During IVD degeneration, the glycosaminoglycan (GAG) and water content of the NP decreases. Like humans, dogs experience spontaneous IVD degeneration with similar characteristics . In both species, notochordal cells (NCs) are replaced by chondrocyte-like cells (CLCs) in the NP during maturation and early IVD degeneration. Therefore, the dog is considered to be a suitable animal model for human IVD degeneration . Dogs can be divided into chondrodystrophic (CD) and nonchondrodystrophic (NCD) breeds on the basis of their physical appearance. In CD dogs, replacement of NCs by CLCs starts around 1 year of age and IVD disease typically develops around 3–7 years of age, whereas in NCD dogs, NCs remain the predominant cell type until middle or old age and if IVD disease develops it occurs around 6–8 years of age . Current treatments for IVD disease (physiotherapy, medication, and surgery) are focused on reducing pain and spinal cord and/or nerve decompression but do not induce IVD repair. Therefore, there is substantial interest in agents stimulating biological repair of the degenerated IVD, resulting in functional restoration . Caveolin-1 could be such an agent, as its advantageous effects have been demonstrated in several tissue types [6–9].
The mammalian caveolin family consists of three proteins (caveolin-1, -2, and -3), which are integral membrane proteins essential for the structural integrity and function of caveolae (flask-shaped invaginations of the plasma membrane) of many differentiated cell types [10–12]. Caveolin-1 is involved in endocytosis, the formation and transport of caveolae, and cell adhesion and migration . Moreover, caveolin-1 is implicated in cell cycle regulation, senescence (cell cycle arrest due to resistance to external stimuli ), and apoptosis . As a scaffolding protein, it regulates signal transduction , and caveolin-binding motifs have been identified in several target proteins . The effect of caveolin-1 on signaling pathways is usually inhibitory due to sequestration and inactivation of molecules in caveolar membranes, but signaling can also be enhanced by bringing molecules together . Altogether, caveolin-1 has been shown to exert context-dependent effects (i.e., differing per tissue/cell type, age, and stage of degeneration) .
Caveolin-1 is differentially expressed in the IVD. The NP of early degenerated canine IVDs expresses lower caveolin-1 levels than healthy canine NC-rich NPs . In addition, the NP of wild-type (WT) mice is rich in viable NCs, whereas the NP of caveolin-1-null mice contains mainly CLCs . In humans, CLCs derived from degenerated IVDs express higher caveolin-1 levels than CLCs from nondegenerated IVDs . During IVD degeneration, accelerated cell senescence takes place [16, 17], and a positive relationship between caveolin-1 expression and premature stress-induced senescence has been reported in articular cartilage  and the IVD . Altogether, this implies that caveolin-1 could play an important role in IVD degeneration.
The aim of this study was to determine the role of caveolin-1 in IVD degeneration. Transforming growth factor (TGF)-β signaling is known to play a role in the degenerative and regenerative processes of cartilaginous tissues , and TGF-β receptors have been demonstrated to colocalize with caveolin-1 . Therefore, we hypothesized that caveolin-1 modifies canonical TGF-β signaling in the IVD and thereby facilitates repair. To assess the effect of in vivo caveolin-1 depletion, we studied murine caveolin-1-null IVDs. With a clinical directive in mind, functional studies were focused on the effect of caveolin-1 on CLCs because degenerated canine and human IVDs contain almost 100 % CLCs. Caveolin-1 expression and apoptosis levels were determined in canine IVDs of different degeneration grades, and human and canine CLCs were silenced for caveolin-1 and/or supplemented with caveolin-1 scaffolding domain (CSD) peptide in vitro to determine the (regenerative) effect of caveolin-1 on CLCs. In the present study, we show that while caveolin-1 preserved the NC phenotype, its expression increased in degenerated IVDs. Given that CSD supplementation enhanced the anabolic effects of TGF-β1 on CLCs in terms of increased GAG deposition in vitro, the increased caveolin-1 expression during IVD degeneration may facilitate an ultimate attempt at repair by decreasing the loss of GAGs.
Thoracic and lumbar spines were collected from 1.5-, 3-, and 6-month-old caveolin-1-null (Cav tm1Mls, JAX®; The Jackson Laboratory, Bar Harbor, ME, USA) and WT mice (B6129SF2, JAX®) of the same genetic background. Experimental procedures were performed according to the guidelines of the Utrecht University Ethics Committee (DEC 2008.III.01.001).
Paraffin-embedded tissue histology
Murine lumbar spines were fixed in 4 % neutral buffered formaldehyde (Klinipath, Duiven, the Netherlands), decalcified (7 days in 10 % ethylenediaminetetraacetic acid), and embedded in paraffin. Midsagittal 5-μm sections were mounted on KP+ microscope slides (KP-3056; Klinipath), stained with hematoxylin and eosin and Alcian Blue/picrosirius red , and immunohistochemically stained for Ki-67 and collagen type II (Table 1). An ApopTag® Plus Peroxidase In Situ Apoptosis Detection Kit (terminal deoxynucleotidyl transferase deoxyuridine triphosphtate nick-end labeling [TUNEL] assay, S7101; EMD Millipore, Billerica, MA, USA) was used to detect apoptotic cells on lumbar midsagittal sections. All lumbar IVDs were evaluated (approximately four IVDs per lumbar spine). Raw images of the sections were made using a Leica DFC420C digital camera (Leica Microsystems, Buffalo Grove, IL, USA) mounted to a BX60 microscope (Olympus America, Center Valley, PA, USA) with the Leica Application Suite (V4.2) software package. Adobe Photoshop CS6 software (Adobe, San Jose, CA, USA) was used to manually count (positively stained) cell numbers in each NP. The percentage of nuclei that stained positive for TUNEL over the total number of nuclei present was determined for every murine NP in conjunction with morphology to avoid false-positive results.
Thoracic IVDs were snap-frozen and stored at −70 °C until analysis. Ten-micrometer transverse cryosections were stained for caveolin-1, phosphorylated Smad2 (pSmad2 indicating activated TGF-β signaling), and the nucleus pulposus progenitor cell (NPPC) markers tyrosine-like receptor Tie2 and disialoganglioside 2 (GD2) (Table 2). Within 48 h, confocal images were obtained with a Zeiss LSM upright confocal laser scanning microscope, and the sections were analyzed with Zen software 2011 (Zeiss Microscopy, Thornwood, NY, USA) in two or three transverse thoracic NP sections per animal. On the basis of the observed expression pattern, caveolin-1, Tie2, and GD2 were scored as being present or not present. The percentage of nuclei that stained positive for pSmad2 over the total number of nuclei present (pSmad2 ratio) was manually counted and calculated per murine NP, and the mean pSmad2 ratio was determined per age group.
Caveolin-1 expression in canine IVD degeneration
Thirty-seven thoracolumbar or lumbosacral IVD samples from sixteen canine cadavers were studied. The dogs were of different breeds (5 CD, 11 NCD), ages (1–16 years), and sex (11 female, 5 male). The samples were divided into five different grades of degeneration on the basis of gross morphology of midsagittal sections, ranging from Thompson grade I for healthy to Thompson grade V for end-stage degeneration [22, 23]. The IVD donors were chosen on the basis of equal representation of all IVD degeneration grades (n = 8, 7, 8, 7, and 7 for grades I–V, respectively). All dogs had been killed in unrelated research projects or were client-owned dogs that were submitted to the Department of Pathobiology Faculty of Veterinary Medicine, Utrecht University, for necropsy. Five-micrometer-thick midsagittal consecutive IVD sections were mounted on KP+ microscope slides and processed for caveolin-1 immunohistochemistry (Table 1) and a TUNEL assay. Thereafter, raw images of the sections were made using a Leica DFC420C digital camera mounted to a BX60 microscope and the Leica Application Suite (V4.2) software package. Adobe Photoshop CS6 was used to manually count (positively stained) TUNEL cell numbers, and the integrated option “color range” was used to determine the area within the NP that stained positive for caveolin-1 (caveolin-1 ratio) in four randomly selected NP areas per IVD section. The mean percentage of nuclei that stained positive for TUNEL over the total number of nuclei present in the four randomly selected NP areas was determined in conjunction with morphology to avoid false-positive results.
In vitro effects of caveolin-1 peptide on human and canine CLCs derived from degenerated IVDs
In total, IVD tissue from 16 canine (11 CD, 5 NCD) and 3 human donors was collected. Complete spines (2–11 years of age, Thompson grade II or III) were collected from dogs that had been killed in unrelated research studies (approved by the Utrecht University Animal Ethics Committee). IVD tissue of three human donors (one male, two females, 47–63 years of age, Thompson grade III) derived from the L2–L5 spinal region were obtained at autopsy. Anonymous use of redundant tissue for research purposes is a standard treatment agreement with patients in University Medical Centre Utrecht (local medical Ethics committee number 12-364). Thus, all necessary consent from patients involved in the study was present. The material was collected as part of the activities of the tissue bank of the Department of Pathology, UMCU Biobank, UMC Utrecht. The scientific committee of the Department of Pathology at UMC Utrecht (Wetenschappelijke Adviesraad Biobank) approved the study. All tissue was used in line with the code “Proper Secondary Use of Human Tissue” as installed by the Dutch Federation of Biomedical Scientific Societies .
Cell culture and experimental design
CLCs were collected from the canine and human NPs as described previously  and thereafter expanded in expansion medium . NCD canine donors that contained only CLCs in the NP were selected using cytospins (Additional file 1). After the CLCs reached 80 % confluence in P2, they were plated in a 96-well plate (CLS7007, Costar®; Corning, Corning Life Sciences, NY, USA) at a density of 35,000 cells/well in 50 μl of chondrogenic culture medium composed of high-glucose Dulbecco’s modified Eagle’s medium + GlutaMAX (31966; Invitrogen, Carlsbad, CA, USA) with 1 % P/S (P11-010; GE Healthcare Life Sciences, Little Chalfont, UK), 1 % ITS+ premix (354352; Corning Life Sciences), 0.04 mg/ml L-proline (P5607; Sigma-Aldrich, St. Louis, MO, USA), 0.1 mM ascorbic acid 2-phosphate (A8960; Sigma-Aldrich), 1.25 mg/ml human serum albumin (human CLCs; Sanquin, Amsterdam, the Netherlands) or bovine serum albumin (canine CLCs, A9418; Sigma-Aldrich), and 10 ng/ml TGF-β1 (240-B; R&D Systems, Minneapolis, MN, USA). The microaggregates were cultured for 14 days (21 % O2, 5 % CO2, 37 °C).
Caveolin-1 expression was silenced in CLCs from six CD canine donors, and the following conditions were tested: mock (100 nM Stealth™ RNAi Negative Control Duplex; Invitrogen), silencing RNA (siRNA) (100 nM caveolin-1 Stealth™ RNAi siRNA Duplex; Invitrogen), and siRNA + CSD (100 nM caveolin-1 siRNA oligo and 10 μM CSD, ALX-153-064; Enzo Life Sciences, Farmingdale, NY, USA). The canine CLCs were transfected with 3 μl/ml Lipofectamine™ RNAiMAX (13778-075; Invitrogen) at the moment of plating. Six hours after plating, the 96-well plates were centrifuged at 50 g for 5 minutes to induce microaggregate formation. Stealth™ RNAi siRNA Duplex (10620312; Invitrogen) was used to silence caveolin-1 (NM_001003296): 5′ CACACCAAGGAAAUCGACCUGGUCA 3′ (guanine-cytosine [GC] percentage 52 %). Stealth™ RNAi Negative Control Duplex (GC percentage 48 %, 12935-300; Invitrogen) was used to determine the effect of Stealth™ RNAi siRNA Duplex versus background (mock).
To determine the optimal conditions for CSD to exert its effects, CLCs from three human donors as well as five CD and five NCD canine donors with the following conditions were studied: T2 (chondrogenic culture medium with 2 ng/ml TGF-β1), T2C10 (2 ng/ml TGF-β1 and 10 μM CSD), T2C25 (2 ng/ml TGF-β1 and 25 μM CSD), T10 (10 ng/ml TGF-β1), T10C10 (10 ng/ml TGF-β1 and 10 μM CSD), and T10C25 (10 ng/ml TGF-β1 and 25 μM CSD).
Two microaggregates per donor and condition were snap-frozen at day 4, and RNA was extracted, cDNA was made, and real-time quantitative polymerase chain reaction was performed for the target genes aggrecan (ACAN), a disintegrin and metalloproteinase with thrombospondin motifs 5 (ADAMTS5), activin receptor-like kinase 1 (ALK1), activin receptor-like kinase 5 (ALK5), BCL2-associated protein (BAX), B-cell CLL/lymphoma 2 (BCL2), caspase 3 (CASP3), caveolin-1 (CAV1), cyclin D1 (CCND1), collagen type I, alpha 1 (COL1A1), collagen type II, alpha 1 (COL2A1), inhibitor of DNA binding 1 (ID1), matrix metalloproteinase 13 (MMP13), plasminogen activator inhibitor 1 (PAI1, a readout for activated Smad2/3 signaling [27–29]), (sex determining region Y)-box 9 (SOX9), and tissue inhibitor of metalloproteinase 1 (TIMP1), as well as the reference genes glyceraldehyde 3-phosphate dehydrogenase (GAPDH), ribosomal protein S19 (RPS19), hypoxanthine-guanine phosphoribosyltransferase (HPRT), and succinate dehydrogenase subunit A (SDHA) as described previously . An overview of the primer pairs is given in Additional file 2. In addition, two microaggregates per condition per donor were collected at days 7 and 14, and the GAG and DNA content of the CLC microaggregates and GAG release into the culture medium were determined as described previously .
To determine caveolin-1 protein silencing efficiency, two snap-frozen microaggregates per condition per donor were pooled, crushed, and dissolved in radioimmunoprecipitation assay (RIPA) buffer at days 7 and 14. Caveolin-1 protein was measured using an enzyme-linked immunosorbent assay (SEA214Ca, Cloud-Clone Corp., Houston, TX, USA). Histopathological evaluation of the microaggregates was performed with Safranin O/Fast Green staining  and collagen types I and II immunohistochemistry (Table 1). Western blot analysis was performed as described previously for pSmad2 (Ser465/467, 60 kDa, 3101; Cell Signaling Technology, Danvers, MA, USA) and β-actin (42 kDa, pan Ab-5; Neomarkers, Fremont, CA, USA) . CD canine CLCs (n = 200,000; mixture of the previously used CD canine donors) were plated per well (six-well plate, 657160, CELLSTAR®; Greiner Bio-One, Monroe, NC, USA) in expansion medium. After 5 days, the cells were treated with 3 ml of chondrogenic culture medium with or without CSD. The following conditions were tested: T2, T2C10, T2C25, T10, T10C10, and T10C25. After 24 h of treatment, protein samples were obtained and homogenized in RIPA buffer containing 0.6 mM phenylmethylsulfonyl fluoride, 17 μg/ml aprotinin, and 1 mM sodium orthovanadate (Sigma-Aldrich). Protein concentrations were measured using the Qubit® Protein Assay Kit (Q32851; Invitrogen) according to the manufacturer’s instructions. The mean volume of the protein bands on the blots was determined by volumetric (INT*mm2) band analysis using Quantity One software (Bio-Rad Laboratories, Hercules, CA, USA). The mean volume of pSmad2 was divided by the mean volume of β-actin (pSmad2/β-actin ratio) to correct for different protein concentrations applied to the membranes.
Statistical analysis was performed using IBM SPSS version 22 (IBM Armonk, NY, USA) and RStudio (version 0.96; RStudio, Boston, MA, USA) software. All data were examined for normal distribution (Shapiro-Wilk test). Kruskal-Wallis and Mann-Whitney U tests were performed on nonnormally distributed data, whereas generalized linear regression models based on analysis of variance were used for normally distributed data. A Cox proportional hazards model was used for genes with undetectable expression (cycle threshold value >40). To find correlations between the caveolin-1/TUNEL ratio and IVD degeneration score, partial correlations (corrected for donor) were determined. All of the above-mentioned tests were followed by a Benjamini-Hochberg false discovery rate post hoc correction for multiple comparisons. A p value less than 0.05 was considered significant.
Effect of in vivo caveolin-1 inactivation on the murine nucleus pulposus
In vivo caveolin-1 loss did not affect the morphometry of the murine IVDs (Additional file 3). However, there was a distinct difference in morphology between NP cells of WT and caveolin-1-null mice. The NP of WT mice was rich in large, vacuolated NCs, whereas the NP of caveolin-1-null mice contained relatively few, smaller, nonvacuolated chondrocyte- and fibroblast-like cells at every studied age (Fig. 1a). NCs were diffusely scattered throughout the NP of 1.5-month-old WT mice, whereas they were located mainly in the center of the NP, surrounded by a rim of chondroid matrix in 3- and 6-month-old WT mice. The NP cell numbers in WT mice did not change considerably during aging, whereas NP cell numbers of caveolin-1-null mice decreased over time with significantly fewer cells at 1.5 and 6 months of age (p < 0.05) (Fig. 1b). At the ages tested, the proportion of positively stained TUNEL cell nuclei (TUNEL ratio) was significantly higher in the NP of caveolin-1-null mice than in WT mice (p < 0.05) (Fig. 1b), indicating that the in vivo loss of caveolin-1 induced apoptosis of murine NP cells, leading to lower cell numbers. In vivo caveolin-1 loss did not affect the expression of the cell proliferation–associated protein Ki-67; there was no positive Ki-67 staining in WT or caveolin-1-null mice NPs (data not shown). In the caveolin-1-null mice, GAGs and collagen type II were abundantly present in the extracellular matrix (ECM), whereas they were present to a lesser extent in WT NPs (Fig. 2).
Immunofluorescent staining confirmed that caveolin-1-null NP cells expressed no caveolin-1 at the protein level, whereas NCs of WT mice abundantly expressed caveolin-1 in their cytoplasm and cell membranes at every studied age (Fig. 3). In vivo caveolin-1 inactivation increased the expression of NPPC markers Tie2 (differentiation marker for dormant NPPCs ) and GD2 (NPPC proliferation marker ). Caveolin-1-null NP cells abundantly expressed these markers at every studied age, whereas WT NCs expressed Tie2 only at 1.5 months of age and GD2 at 1.5 and 6 months of age (Fig. 3). GD2 was intracellularly compartmentalized in caveolin-1-null NP cells but localized in the cell membrane of WT mice NCs. Moreover, the percentage of cells expressing nuclear pSmad2 protein was significantly higher in the 1.5-month-old murine caveolin-1-null NPs compared with murine WT NPs of the same age. The percentage of cells expressing pSmad2 was significantly increased in the 3-month-old WT NPs compared with the 1.5-month-old WT NPs. At 3 and 6 months of age, WT and caveolin-1-null NP cells showed a similar percentage of pSmad2-positive stained nuclei, indicating comparable levels of activated TGF-β/Smad2 signaling (p < 0.05) (Fig. 4).
Caveolin-1 expression and apoptosis during canine IVD degeneration
Apoptotic (TUNEL-positive) cell nuclei were observed in healthy NC-containing NPs and in degenerated CLC-containing NPs (Fig. 5a). NPs obtained from IVDs with Thompson grades IV and V demonstrated significantly more apoptotic cells than healthy and early degenerated NPs (Thompson grades I and II) in CD and NCD dogs (p < 0.05) (Fig. 5b). Also, there was a significant positive correlation between apoptosis levels and IVD degeneration grade in CD and NCD dogs (r = 0.607 and r = 0.486, respectively; p < 0.05) (Fig. 5b). There were no statistically significant differences between CD and NCD dogs for apoptosis levels per Thompson grade.
Caveolin-1 expression was localized in the cytoplasm and cell membranes of NCs from healthy NPs and in CLCs from (severely) degenerated NPs (Fig. 5a). No correlation between caveolin-1 expression and donor age was observed (data not shown). Also, there were no statistically significant differences between CD and NCD dogs for caveolin-1 expression per Thompson grade. The expression of caveolin-1 significantly increased during IVD degeneration in CD dogs (p < 0.05) (Fig. 5c). Caveolin-1 expression and IVD degeneration grade (Thompson grades I–V) did not correlate in NCD dogs (r = −0.247), while in CD dogs there was a strong positive correlation between caveolin-1 expression and IVD degeneration grade (r = 0.719, p < 0.01) (Fig. 5c). However, given that NC-rich Thompson grade I IVDs were available only from NCD dogs, when excluding those Thompson grade I IVDs, caveolin-1 expression weakly correlated with IVD degeneration for the range of Thompson grades II–V in the NCD dogs (r = 0.349) (Fig. 5c). No statistically significant correlation between caveolin-1 expression and apoptosis levels was found in CD or NCD canine NPs (data not shown).
In vitro effects of caveolin-1 on human and canine CLCs
Effect of caveolin-1 silencing in canine CLCs in vitro
With a clinical directive in mind, caveolin-1 was silenced and CSD peptide (which mimics the function of caveolin-1 [8, 9, 32–34]) was added to canine and human CLCs derived from degenerated IVDs to determine whether caveolin-1 modifies TGF-β signaling in CLCs with concurrent effects on ECM level. CAV1 messenger RNA (mRNA) knockdown in the caveolin-1-silenced CLCs was 70 % compared with mock-treated CLCs at day 4 (p < 0.001) (Fig. 6a). CSD treatment upregulated CAV1 mRNA expression in canine CLCs silenced for caveolin-1 (p < 0.05). Caveolin-1 protein knockdown was 53 % compared with mock-treated CLCs at day 7 and 48 % at day 14 (Fig. 6a). While PAI1 expression was decreased in caveolin-1-silenced CLCs compared with mock-treated CLCs (p < 0.05), ALK5 and PAI1 expression were increased by CSD treatment of these CLCs (p < 0.01) (Fig. 6b), which indicated activated TGF-β/Smad2/3 signaling under the influence of CSD at least at the gene expression level. Expression of the antiapoptotic BCL2 gene was decreased by caveolin-1 silencing, whereas the addition of CSD reversed this effect (p < 0.05) (Fig. 6b). Gene expression of MMP13, ACAN (Fig. 6b), COL1A1, COL2A1, SOX9, TIMP1, ALK1, ID1, CCND1, BAX, and CASP3 (data not shown) was not significantly different between the conditions.
Caveolin-1-silenced CLCs showed increased ADAMTS5 expression compared with mock-treated CLCs (p < 0.05), whereas CSD treatment reversed this effect (p < 0.01) (Fig. 6b). Also, the GAG content of caveolin-1-silenced microaggregates was significantly less than in mock-treated microaggregates at day 7 (17 %; p < 0.05), but not at day 14 (10 %) (Fig. 6c). CSD treatment increased the GAG content of caveolin-1-silenced microaggregates at day 14 (14 %; p < 0.05). GAG release into the culture medium (data not shown) and the DNA content (Fig. 6c) of the microaggregates was not considerably different between the conditions.
All CLC microaggregates stained positive for GAGs and collagen types I and II (Fig. 6c). In the mock-treated microaggregates, and mainly in the caveolin-1-silenced microaggregates supplemented with CSD, a collagen type II–positive rim was present, but not in the caveolin-1-silenced microaggregates not supplemented with CSD.
Dose–response effect of caveolin-1 peptide on canine and human CLCs in vitro
Because CSD treatment rescued the effects of caveolin-1 silencing and exerted anabolic effects on canine CLCs by modifying TGF-β signaling at the gene expression level, different concentrations (i.e., 2 ng/ml TGF-β1 [T2], 10 ng/ml TGF-β1 [T10], 10 μM CSD [C10], and 25 μM CSD [C25]) were tested to determine the additive effect of CSD on TGF-β1 treatment of human, CD, and NCD canine CLCs. The DNA content of CD and NCD canine T10-treated microaggregates was significantly higher than that of T2-treated microaggregates (p < 0.05), whereas this was not observed in human microaggregates (Fig. 7). Only in NCD canine donors, T2C25-treated microaggregates showed an increased DNA content compared with T2C10-treated microaggregates (p < 0.05). CSD treatment did not affect the DNA content of human and CD canine microaggregates.
In CD and NCD donors, the GAG content of the T2C25-treated microaggregates was significantly higher (35 % for CD, 25 % for NCD) than the GAG content of T2-treated microaggregates (Fig. 7). Additionally, only in CD donors was the GAG content of the T10C25-treated microaggregates significantly higher (26 %) than the GAG content of the T10-treated microaggregates. GAG release in the culture medium was decreased by approximately three times in T2C25-treated CLC microaggregates compared with T2-treated CLC microaggregates in all species (p < 0.05) (Fig. 7). Total GAG production (GAG content in the microaggregates plus GAG release into the culture medium) appeared to be 20–40 % decreased by 25 μM CSD treatment in all species and was significantly decreased in T2C25-treated CD and NCD canine CLCs compared with T2- and T2C10-treated CD and NCD canine CLCs (p < 0.05), but not significantly different between the differentially treated human CLCs (data not shown). The GAG content of human CLC microaggregates was lower than the GAG content of CD and NCD canine microaggregates. In contrast to canine CLC microaggregates, human CLC microaggregates demonstrated no collagen type II protein deposition (Fig. 7). Furthermore, CSD treatment increased collagen type I deposition in human CLC microaggregates, whereas this was not observed in canine CLC microaggregates.
Western blot analysis demonstrated that pSmad2 protein expression was 1.7 times higher in CD canine CLCs treated with 2 ng/ml TGF-β1 than in those treated with 10 ng/ml TGF-β1 (Fig. 8). pSmad2 protein expression was 1.3–1.5 times higher in the canine CLCs treated with 10 or 25 μM CSD and 2 ng/ml TGF-β1 than in those treated with only 2 ng/ml TGF-β1 (Fig. 8). Furthermore, pSmad2 protein expression was 1.1–1.2 times higher in the CLCs treated with 10 or 25 μM CSD and 10 ng/ml TGF-β1 than in those treated with only 10 ng/ml TGF-β1 (Fig. 8). Altogether, this indicates that CSD peptide treatment enhanced TGF-β/pSmad2 signaling.
The present study demonstrates that caveolin-1 plays a role in IVD degeneration. In vivo studies with murine caveolin-1-null NPs demonstrated that caveolin-1 was essential for NC preservation. Furthermore, we have demonstrated that caveolin-1 expression and apoptosis levels were significantly increased during CD canine IVD degeneration. In addition, in vitro caveolin-1 silencing decreased CLC ECM deposition, while CSD supplementation increased TGF-β/pSmad2 signaling at the gene and protein expression levels and enhanced the anabolic effects of TGF-β1 on CLCs, resulting in higher ECM deposition. Taken together, this may indicate that the increased caveolin-1 expression during IVD degeneration facilitates an anabolic reparative response of the CLCs at least by modifying TGF-β signaling rather than being merely correlated with CLC apoptosis.
Caveolin-1 is essential for NC physiology
Histological analysis of caveolin-1-null NPs revealed that apoptotic cells were present in the healthy WT murine NP at 1.5, 3, and 6 months of age, implying that during IVD tissue homeostasis, there is physiologic turnover of NP cells (they proliferate and undergo apoptosis). Affirmatively, previous work already demonstrated apoptotic cells in IVDs from 2-week-old WT mice . Caveolin-1-null NPs showed the absence of typical NCs in favor of chondrocyte/fibroblast-like cells with an increased apoptotic activity, suggesting that caveolin-1 is essential for NC preservation. In line with this thought, NPs of NCD dogs with Thompson grade I, rich in NC cells, abundantly expressed caveolin-1, while the caveolin-1-null mice had lost their NCs already when they were skeletally mature (young adult), which is rather comparable with the loss of NCs in young adult CD dogs and humans. In the NP of 1.5-month-old caveolin-1-null mice (with lower total NP cells numbers than WT mice), Tie2+/GD2+ progenitor cells were present, and TGF-β signaling mediated by pSmad2 probably facilitated abundant ECM deposition. Affirmatively, Tie2+/GD2+ NP cells have been shown to possess superior ECM production, self-renewal, multipotent differentiation, and proliferation capacity . Increased cell proliferation is associated with late-stage IVD degeneration . Notably, the NPPC proliferation marker GD2 was expressed in caveolin-1-null and WT mice NPs, but Ki-67 positivity was not detected. The short Ki-67 protein half-life (90 minutes) and nutritionally deprived NP environment may explain the absence of Ki-67 in murine NPs . GD2 appeared intracellularly compartmentalized in caveolin-1-null NP cells but localized to the cell membrane of WT NCs. We hypothesize that in the caveolin-1-null NP phenotype, GD2 may not mark proliferating cells per se if the different localization could render GD2 inactive, but researchers in future studies should look into the functionality of GD2 in caveolin-1-null NP cells.
Altogether, caveolin-1 plays a role in the preservation of healthy NCs because in vivo inactivation of caveolin-1 induced a change in cell phenotype from NCs toward CLCs with high apoptotic activity in mice. Activated NPPCs and TGF-β/pSmad2 signaling probably resulted into GAG- and collagen-rich ECM deposition in the caveolin-1-null mice NP. The caveolin-1-null mice showed several metabolic/endocrine disorders [37–39] that could have influenced their NP phenotype (e.g., insulin resistance leading to diabetes mellitus, which has been associated with premature NC senescence and apoptosis) . Further studies need to be concentrated at earlier stages of development to delineate how caveolin-1 preserves NCs, including modification of mitogen-activated protein kinase/extracellular signal-regulated kinase, Wnt , Indian hedgehog and/or sonic hedgehog signaling pathways [41, 42], and/or glucose transport [43, 44].
Caveolin-1 increases during IVD degeneration, mediating a reparative response
Caveolin-1 is known to induce apoptosis via—among others—cell cycle arrest in the G2/M phase  and by influencing the expression of the antiapoptosis protein survivin [46, 47]. Caveolin-1 may induce senescence in CLCs, given that, in NPs derived from degenerated CD canine and human IVDs, caveolin-1 expression  and apoptosis levels were positively correlated with IVD degeneration grade. However, a causative relationship in the IVD remains to be determined. On the basis of the results of the present study, it is tempting to hypothesize that the increased caveolin-1 expression in degenerated IVDs may be part of an ultimate attempt at (unsuccessful) repair. With a clinical directive in mind (degenerated human and canine IVDs contain almost 100 % CLCs), the effect of caveolin-1 was investigated in human and canine CLCs derived from degenerated IVDs by silencing for caveolin-1 and/or supplementing with CSD peptide. Caveolin-1 silencing decreased antiapoptotic BCL2 expression, whereas CSD addition increased it to baseline levels again, opposing the hypothesis that caveolin-1 itself induces CLC apoptosis. Furthermore, caveolin-1 silencing increased ADAMTS5 expression and decreased the GAG content of the microaggregates, whereas when the canine CLCs were treated with CSD, ADAMTS5 expression decreased and the GAG content was restored. In line with this, GAG release was decreased in 25 μM CSD-treated human and canine CLCs. Notably, caveolin-1 silencing and CSD supplementation did not influence collagen type I deposition by canine CLCs, while its deposition was increased by CSD treatment in human CLCs. It is plausible that caveolin-1 exerts a protective effect by decreasing ECM degradation, given its well-described anti-inflammatory properties [48–50]. This altogether implies that decreased GAG degradation resulted in the significantly increased GAG content of CSD-treated canine CLCs. The underlying mechanisms for the latter could be decreased ECM degradation and/or more collagen type II protein expression that enables the deposition  and prevents the release of GAGs.
The results of this study imply that caveolin-1 regulates TGF-β signaling in CLCs in vitro, because caveolin-1 silencing decreased, whereas CSD supplementation increased TGF-β/Smad2 signaling at the gene and protein expression levels. TGF-β signals through two membrane TGF-β receptors type I (ALK1 and ALK5) and one TGF-β receptor type II. These TGF-β receptors have been demonstrated to colocalize with caveolin-1 . TGF-β receptor type II phosphorylates TGF-β receptor type I. When ALK5 is phosphorylated, Smad2/3 signaling becomes activated and ECM is produced. However, when ALK1 is phosphorylated, Smad1/5/8 signaling becomes activated, which inhibits Smad2/3 signaling and ECM production [52, 53]. In this study, we have demonstrated that CSD enhanced the anabolic effect of TGF-β1 in terms of ECM deposition in the microaggregates. Caveolin-1 silencing decreased PAI1 (a classical readout for activated Smad2/3 TGF-β signaling [27–29]) gene expression, while CSD supplementation increased ALK5 and PAI1 gene expression, did not influence ALK1 or ID1 (readout for activated Smad1/5/8 signaling) gene expression, and increased pSmad2 protein expression. This all indicates that caveolin-1 indeed enhanced TGF-β/Smad2/3 signaling.
There is evidence that caveolin-1 acts differently according to stimulating and/or inhibiting signals and cellular context (e.g., cell type, age, and disease and/or health stage of the tissue) [7, 11, 54]. In the present study, caveolin-1 enhanced TGF-β signaling mediated by pSmad2 in CLCs from degenerated IVDs in vitro, while the opposite was true in earlier reports [14, 55–57]. In line with our results, however, TGF-β signaling is reduced in caveolin-1-deficient fibroblasts  and regenerating hepatocytes of caveolin-1-null mice . Notably, in caveolin-1-silenced canine CLCs, ECM production was decreased, whereas in caveolin-1-null mice, which initially contained primarily NCs, abundant ECM was deposited. This implies that caveolin-1 may indeed have different functions in NCs and CLCs, because caveolin-1 is required for NC preservation, whereas in CLCs it may be related to apoptosis and/or it may influence signaling pathways (such as TGF-β) that support ECM deposition.
The present study demonstrates that caveolin-1 plays a role in IVD degeneration. The abundant expression of caveolin-1 in NCs from NCD dogs and the loss of healthy NCs in the NP of caveolin-1-null mice indicate that caveolin-1 supports preservation of the NC phenotype. In the CD canine NP, both caveolin-1 expression and apoptosis levels had a positive correlation with IVD degeneration grade, indicating that caveolin-1 may be related with CLC apoptosis. Nevertheless, ECM deposition was decreased by in vitro caveolin-1 silencing of canine CLCs, whereas CSD peptide increased TGF-β/pSmad2 signaling at the gene and protein expression levels and enhanced the anabolic effects of TGF-β1 with concomitant increased ECM deposition. This implies that the increased caveolin-1 expression during IVD degeneration may be an anabolic repair response rather than merely being correlated with CLC apoptosis. Further studies are needed to investigate how caveolin-1 modifies other signaling pathways and facilitates IVD repair.
a disintegrin and metalloproteinase with thrombospondin motifs 5
activin receptor-like kinase 1
activin receptor-like kinase 5
B-cell CLL/lymphoma 2–associated protein
B-cell CLL/lymphoma 2
bovine serum albumin
- CASP3 :
- CAV1 :
- CCND1 :
- COL1A1 :
collagen type I, alpha 1
- COL2A1 :
collagen type II, alpha 1
caveolin-1 scaffolding domain
- GAPDH :
glyceraldehyde 3-phosphate dehydrogenase
- HPRT :
- ID1 :
inhibitor of DNA binding 1
matrix metalloproteinase 13
nucleus pulposus progenitor cell
- PAI1 :
plasminogen activator inhibitor 1
- RPS19 :
ribosomal protein S19
- SDHA :
succinate dehydrogenase subunit A
- SOX9 :
(sex determining region Y)-box 9
transforming growth factor
- TIMP1 :
tissue inhibitor of metalloproteinase 1
terminal deoxynucleotidyl transferase deoxyuridine triphosphate nick-end labeling
Murray CJ, Vos T, Lozano R, Naghavi M, Flaxman AD, Michaud C, et al. Disability-adjusted life years (DALYs) for 291 diseases and injuries in 21 regions, 1990–2010: a systematic analysis for the Global Burden of Disease Study 2010. Lancet. 2012;380(9859):2197–223.
Freemont AJ. The cellular pathobiology of the degenerate intervertebral disc and discogenic back pain. Rheumatology (Oxford). 2009;48(1):5–10.
Bergknut N, Rutges JP, Kranenburg HJ, Smolders LA, Hagman R, Smidt HJ, et al. The dog as an animal model for intervertebral disc degeneration? Spine (Phila Pa 1976). 2012;37(5):351–8.
Smolders LA, Bergknut N, Grinwis GC, Hagman R, Lagerstedt AS, Hazewinkel HA, et al. Intervertebral disc degeneration in the dog. Part 2: chondrodystrophic and non-chondrodystrophic breeds. Vet J. 2013;195(3):292–9.
Bach FC, Willems N, Penning LC, Ito K, Meij BP, Tryfonidou MA. Potential regenerative treatment strategies for intervertebral disc degeneration in dogs. BMC Vet Res. 2014;10:3.
Head BP, Hu Y, Finley JC, Saldana MD, Bonds JA, Miyanohara A, et al. Neuron-targeted caveolin-1 protein enhances signaling and promotes arborization of primary neurons. J Biol Chem. 2011;286(38):33310–21.
Baker N, Tuan RS. The less-often-traveled surface of stem cells: caveolin-1 and caveolae in stem cells, tissue repair and regeneration. Stem Cell Res Ther. 2013;4(4):90.
Tourkina E, Richard M, Gooz P, Bonner M, Pannu J, Harley R, et al. Antifibrotic properties of caveolin-1 scaffolding domain in vitro and in vivo. Am J Physiol Lung Cell Mol Physiol. 2008;294(5):L843–61.
Zhang GY, Yu Q, Cheng T, Liao T, Nie CL, Wang AY, et al. Role of caveolin-1 in the pathogenesis of tissue fibrosis by keloid-derived fibroblasts in vitro. Br J Dermatol. 2011;164(3):623–7.
Zou H, Stoppani E, Volonte D, Galbiati F. Caveolin-1, cellular senescence and age-related diseases. Mech Ageing Dev. 2011;132(11-12):533–42.
Mercier I, Jasmin JF, Pavlides S, Minetti C, Flomenberg N, Pestell RG, et al. Clinical and translational implications of the caveolin gene family: lessons from mouse models and human genetic disorders. Lab Invest. 2009;89(6):614–23.
Okamoto T, Schlegel A, Scherer PE, Lisanti MP. Caveolins, a family of scaffolding proteins for organizing “preassembled signaling complexes” at the plasma membrane. J Biol Chem. 1998;273(10):5419–22.
Hulit J, Bash T, Fu M, Galbiati F, Albanese C, Sage DR, et al. The cyclin D1 gene is transcriptionally repressed by caveolin-1. J Biol Chem. 2000;275(28):21203–9.
Gvaramia D, Blaauboer ME, Hanemaaijer R, Everts V. Role of caveolin-1 in fibrotic diseases. Matrix Biol. 2013;32(6):307–15.
Smolders LA, Meij BP, Onis D, Riemers FM, Bergknut N, Wubbolts R, et al. Gene expression profiling of early intervertebral disc degeneration reveals a down-regulation of canonical Wnt signaling and caveolin-1 expression: implications for development of regenerative strategies. Arthritis Res Ther. 2013;15(1):R23.
Heathfield SK, Le Maitre CL, Hoyland JA. Caveolin-1 expression and stress-induced premature senescence in human intervertebral disc degeneration. Arthritis Res Ther. 2008;10(4):R87.
Le Maitre CL, Freemont AJ, Hoyland JA. Accelerated cellular senescence in degenerate intervertebral discs: a possible role in the pathogenesis of intervertebral disc degeneration. Arthritis Res Ther. 2007;9(3):R45.
Dai SM, Shan ZZ, Nakamura H, Masuko-Hongo K, Kato T, Nishioka K, et al. Catabolic stress induces features of chondrocyte senescence through overexpression of caveolin 1: possible involvement of caveolin 1-induced down-regulation of articular chondrocytes in the pathogenesis of osteoarthritis. Arthritis Rheum. 2006;54(3):818–31.
Zhao W, Wang T, Luo Q, Chen Y, Leung VY, Wen C, Shah MF, Pan H, Chiu K, Cao X, Lu WW. Cartilage degeneration and excessive subchondral bone formation in spontaneous osteoarthritis involves altered TGF-β signaling. J Orthop Res. In press. doi:10.1002/jor.23079.
Mayoral R, Valverde AM, Llorente Izquierdo C, González-Rodríguez A, Boscá L, Martín-Sanz P. Impairment of transforming growth factor β signaling in caveolin-1-deficient hepatocytes: role in liver regeneration. J Biol Chem. 2010;285(6):3633–42.
Gruber HE, Ingram J, Hanley Jr EN. An improved staining method for intervertebral disc tissue. Biotech Histochem. 2002;77(2):81–3.
Bergknut N, Grinwis G, Pickee E, Auriemma E, Lagerstedt AS, Hagman R, et al. Reliability of macroscopic grading of intervertebral disk degeneration in dogs by use of the Thompson system and comparison with low-field magnetic resonance imaging findings. Am J Vet Res. 2011;72(7):899–904.
Bergknut N, Meij BP, Hagman R, de Nies KS, Rutges JP, Smolders LA, et al. Intervertebral disc disease in dogs - part 1: a new histological grading scheme for classification of intervertebral disc degeneration in dogs. Vet J. 2013;195(2):156–63.
Rutges JP, Nikkels PG, Oner FC, Ottink KD, Verbout AJ, Castelein RJ, et al. The presence of extracellular matrix degrading metalloproteinases during fetal development of the intervertebral disc. Eur Spine J. 2010;19(8):1340–6.
Willems N, Bach FC, Plomp SG, van Rijen MH, Wolfswinkel J, Grinwis GC, et al. Intradiscal application of rhBMP-7 does not induce regeneration in a canine model of spontaneous intervertebral disc degeneration. Arthritis Res Ther. 2015;17:137.
Bach FC, de Vries SA, Krouwels A, Creemers LB, Ito K, Meij BP, et al. The species-specific regenerative effects of notochordal cell-conditioned medium on chondrocyte-like cells derived from degenerated human intervertebral discs. Eur Cell Mater. 2015;30:132–47.
Mallat Z, Tedgui A. The role of transforming growth factor β in atherosclerosis: novel insights and future perspectives. Curr Opin Lipidol. 2002;13(5):523–9.
Cunha SI, Pietras K. ALK1 as an emerging target for antiangiogenic therapy of cancer. Blood. 2011;117(26):6999–7006.
Vaughan DE. PAI-1 and TGF-β: unmasking the real driver of TGF-β-induced vascular pathology. Arterioscler Thromb Vasc Biol. 2006;26(4):679–80.
Spee B, Arends B, van den Ingh TS, Brinkhof B, Nederbragt H, Ijzer J, et al. Transforming growth factor β-1 signalling in canine hepatic diseases: new models for human fibrotic liver pathologies. Liver Int. 2006;26(6):716–25.
Sakai D, Nakamura Y, Nakai T, Mishima T, Kato S, Grad S, et al. Exhaustion of nucleus pulposus progenitor cells with ageing and degeneration of the intervertebral disc. Nat Commun. 2012;3:1264.
Bernatchez PN, Bauer PM, Yu J, Prendergast JS, He P, Sessa WC. Dissecting the molecular control of endothelial NO synthase by caveolin-1 using cell-permeable peptides. Proc Natl Acad Sci U S A. 2005;102(3):761–6.
Bucci M, Gratton JP, Rudic RD, Acevedo L, Roviezzo F, Cirino G, et al. In vivo delivery of the caveolin-1 scaffolding domain inhibits nitric oxide synthesis and reduces inflammation. Nat Med. 2000;6(12):1362–7.
Miyasato SK, Loeffler J, Shohet R, Zhang J, Lindsey M, Le Saux CJ. Caveolin-1 modulates TGF-β1 signaling in cardiac remodeling. Matrix Biol. 2011;30(5-6):318–29.
Dahia CL, Mahoney EJ, Durrani AA, Wylie C. Postnatal growth, differentiation, and aging of the mouse intervertebral disc. Spine (Phila Pa 1976). 2009;34(5):447–55.
Johnson WE, Eisenstein SM, Roberts S. Cell cluster formation in degenerate lumbar intervertebral discs is associated with increased disc cell proliferation. Connect Tissue Res. 2001;42(3):197–207.
Pojoga LH, Underwood PC, Goodarzi MO, Williams JS, Adler GK, Jeunemaitre X, et al. Variants of the caveolin-1 gene: a translational investigation linking insulin resistance and hypertension. J Clin Endocrinol Metab. 2011;96(8):E1288–92.
Senou M, Costa MJ, Massart C, Thimmesch M, Khalifa C, Poncin S, et al. Role of caveolin-1 in thyroid phenotype, cell homeostasis, and hormone synthesis: in vivo study of caveolin-1 knockout mice. Am J Physiol Endocrinol Metab. 2009;297(2):E438–51.
Le Lay S, Kurzchalia TV. Getting rid of caveolins: phenotypes of caveolin-deficient animals. Biochim Biophys Acta. 2005;1746(3):322–33.
Jiang L, Zhang X, Zheng X, Ru A, Ni X, Wu Y, et al. Apoptosis, senescence, and autophagy in rat nucleus pulposus cells: implications for diabetic intervertebral disc degeneration. J Orthop Res. 2013;31(5):692–702.
Karpen HE, Bukowski JT, Hughes T, Gratton JP, Sessa WC, Gailani MR. The sonic hedgehog receptor patched associates with caveolin-1 in cholesterol-rich microdomains of the plasma membrane. J Biol Chem. 2001;276(22):19503–11.
Dahia CL, Mahoney E, Wylie C. Shh signaling from the nucleus pulposus is required for the postnatal growth and differentiation of the mouse intervertebral disc. PLoS One. 2012;7(4):e35944.
Zhang QQ, Huang L, Han C, Guan X, Wang YJ, Liu J, et al. Caveolin-1 and glucose transporter 4 involved in the regulation of glucose-deprivation stress in PC12 cells. Sheng Li Xue Bao. 2015;67(4):349–56.
González-Muñoz E, López-Iglesias C, Calvo M, Palacín M, Zorzano A, Camps M. Caveolin-1 loss of function accelerates glucose transporter 4 and insulin receptor degradation in 3 T3-L1 adipocytes. Endocrinology. 2009;150(8):3493–502.
Kang J, Park JH, Lee HJ, Jo U, Park JK, Seo JH, et al. Caveolin-1 modulates docetaxel-induced cell death in breast cancer cell subtypes through different mechanisms. Cancer Res Treat. In press. doi: 10.4143/crt.2015.227.
Zhang M, Lin L, Lee SJ, Mo L, Cao J, Ifedigbo E, et al. Deletion of caveolin-1 protects hyperoxia-induced apoptosis via survivin-mediated pathways. Am J Physiol Lung Cell Mol Physiol. 2009;297(5):L945–53.
Torres VA, Tapia JC, Rodriguez DA, Lladser A, Arredondo C, Leyton L, et al. E-cadherin is required for caveolin-1-mediated down-regulation of the inhibitor of apoptosis protein survivin via reduced β-catenin-Tcf/Lef-dependent transcription. Mol Cell Biol. 2007;27(21):7703–17.
Feng H, Guo L, Song Z, Gao H, Wang D, Fu W, et al. Caveolin-1 protects against sepsis by modulating inflammatory response, alleviating bacterial burden, and suppressing thymocyte apoptosis. J Biol Chem. 2010;285(33):25154–60.
Yuan K, Huang C, Fox J, Gaid M, Weaver A, Li G, et al. Elevated inflammatory response in caveolin-1-deficient mice with Pseudomonas aeruginosa infection is mediated by STAT3 protein and nuclear factor κB (NF-κB). J Biol Chem. 2011;286(24):21814–25.
Wang P, Zhu F, Tong Z, Konstantopoulos K. Response of chondrocytes to shear stress: antagonistic effects of the binding partners Toll-like receptor 4 and caveolin-1. FASEB J. 2011;25(10):3401–15.
Yuan M, Leong KW, Chan BP. Three-dimensional culture of rabbit nucleus pulposus cells in collagen microspheres. Spine J. 2011;11(10):947–60.
Blaney Davidson EN, Remst DF, Vitters EL, van Beuningen HM, Blom AB, Goumans MJ, et al. Increase in ALK1/ALK5 ratio as a cause for elevated MMP-13 expression in osteoarthritis in humans and mice. J Immunol. 2009;182(12):7937–45.
Kwon YJ, Lee JW, Moon EJ, Chung YG, Kim OS, Kim HJ. Anabolic effects of Peniel 2000, a peptide that regulates TGF-β1 signaling on intervertebral disc degeneration. Spine (Phila Pa 1976). 2013;38(2):E49–58.
Boscher C, Nabi IR. Caveolin-1: role in cell signaling. Adv Exp Med Biol. 2012;729:29–50.
Meyer C, Liu Y, Kaul A, Peipe I, Dooley S. Caveolin-1 abrogates TGF-β mediated hepatocyte apoptosis. Cell Death Dis. 2013;4:e466.
Razani B, Zhang XL, Bitzer M, von Gersdorff G, Bottinger EP, Lisanti MP. Caveolin-1 regulates transforming growth factor (TGF)-β/SMAD signaling through an interaction with the TGF-β type I receptor. J Biol Chem. 2001;276(9):6727–38.
Del Galdo F, Sotgia F, de Almeida CJ, Jasmin JF, Musick M, Lisanti MP, et al. Decreased expression of caveolin 1 in patients with systemic sclerosis: crucial role in the pathogenesis of tissue fibrosis. Arthritis Rheum. 2008;58(9):2854–65.
Samarakoon R, Chitnis SS, Higgins SP, Higgins CE, Krepinsky JC, Higgins PJ. Redox-induced Src kinase and caveolin-1 signaling in TGF-β1-initiated SMAD2/3 activation and PAI-1 expression. PLoS One. 2011;6(7):e22896.
This work was supported by AOSpine Research Network grants (SRN2011_11, AOSPINE 106540) and the Dutch Arthritis Foundation (LLP22). Neither funding body played any role in study design; collection, analysis, or interpretation of data; manuscript writing; or the decision to submit the manuscript for publication. The authors thank Anita Krouwels for supplying the human CLCs and Willem de Jong, Bianca Kuster, Dirk Vestjens, and Birgit Seubers for assistance during the execution of experiments.
The authors declare that they have no competing interests.
FCB participated in the design and coordination of the study, carried out material collection, executed the experiments, performed data analysis and drafted the manuscript. YZ executed the immunofluorescence experiments. LCV executed caveolin-1 culture experiments. NB carried out canine IVD sample collection and graded these samples macroscopically, microscopically and on MR imaging. AMB, LBC, KI, DS and DC participated in the design and coordination of the study. BM and MT carried out sample collection and designed and coordinated the study. All authors read and approved the manuscript after revising it critically for important intellectual content.
Additional file 1:
Cytospins of canine CLC donors. (DOCX 1497 kb)
Additional file 2:
Overview of the primer pairs. (DOCX 25 kb)
Additional file 3:
Morphometry of murine IVDs. (DOCX 499 kb)
Rights and permissions
Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
About this article
Cite this article
Bach, F.C., Zhang, Y., Miranda-Bedate, A. et al. Increased caveolin-1 in intervertebral disc degeneration facilitates repair. Arthritis Res Ther 18, 59 (2016). https://doi.org/10.1186/s13075-016-0960-y
- Intervertebral disc
- Nucleus pulposus
- Back pain