The unfolded protein response genes in human osteoarthritic chondrocytes: PERK emerges as a potential therapeutic target
© The Author(s). 2016
Received: 14 March 2016
Accepted: 30 June 2016
Published: 19 July 2016
The unfolded protein response (UPR) is activated following an endoplasmic reticulum (ER) stress. The aim of this study was to investigate the global expression of UPR genes in human OA chondrocytes in induced (I)-UPR conditions, and to explore the regulation and role of the UPR genes in homeostatic (H)-UPR conditions in human normal and OA chondrocytes.
Gene expression was determined by PCR array and qPCR. Protein production in cartilage was determined by immunohistochemistry, gene silencing by specific siRNAs, and gene regulation by treating chondrocytes with cytokines and growth factors associated with cartilage pathobiology.
Several UPR genes, among them ERN1, PERK, and CREB3L2 were downregulated in OA compared to normal chondrocytes at both the mRNA and protein levels, but the ER stress response triggered by thapsigargin or tunicamycin treatment was similar in normal and OA chondrocytes. The activation of ER stress sensors (phosphorylated PERK, cleavage of ATF6B, and the spliced mRNA forms of XBP1) was not significantly increased in OA chondrocytes/cartilage. PDGF-BB and IL-6 significantly downregulated the expression of ERN1, PERK, and CREB3L2, but not that of ATF6B. Silencing experiments done under conditions of no ER stress (physiological conditions) revealed that decreasing ERN1 expression led to decreased COL2a1, MMP-13, ADAMTS4 and ADAMTS5 expression, while decreasing CREB3L2 and ATF6B led to decreased ADAMTS5 and ADAMTS4 expression, respectively. Importantly, the downregulation of PERK expression increased COL1a1 and suppressed COL2a1 expression.
Although the level of ER stress is not significantly increased in OA chondrocytes, these cells respond strongly to an acute ER stress despite the decreased expression of ERN1, PERK, and CREB3L2. Emerging findings revealed for the first time that these genes play a role in cartilage biology in conditions where an acute ER stress response is not triggered and OA is not characterized by an overall basal activation of the ER stress response. Importantly, these findings identify PERK as a potential target for new OA treatment avenues.
KeywordsPERK Osteoarthritis Chondrocyte ER stress Unfolded protein response
Osteoarthritis (OA) is a progressive disease of the joints resulting in the degradation of articular cartilage. Several signalling pathways, transcription factors, and cytokines contribute to the progression of this disease, and it is likely that other molecules will be discovered as well, as more is yet to be learned to fully understand this pathology.
The endoplasmic reticulum (ER) stress response has attracted attention as a new area of research in OA cartilage biology. ER stress can be triggered by oxidative stress, heat shock, hypoxia, expression of mutant proteins and drugs such as thapsigargin (Tg), which disrupts ER calcium ion balance , and tunicamycin (Tm), which inhibits N-linked glycosylation . The cellular response, known as the unfolded protein response (UPR), serves to counter the stresses that occur by the presence of misfolded proteins in the ER in an attempt to restore homeostasis [3–8]. Three major families of ER stress sensors have been identified in mammalian cells: the endoplasmic reticulum to nucleus 1 (ERN1, also called IRE1), PRKR-like endoplasmic reticulum kinase (PERK, or EIF2AK3), and activating transcription factor 6 (ATF6). The ATF6 family comprises several members, among them ATF6B, CAMP-responsive element-binding protein 3-like 2 (CREB3L2), and old astrocyte specifically induced substance (OASIS), which are involved in different cellular processes or expressed preferentially depending on cell type [9, 10]. As an example, CREB3L2 has been identified as a transcription factor expressed strongly in chondrocytes . Accumulation of unfolded proteins in the ER initiates the activation of ERN1, PERK, and ATF6, leading to the upregulation of several genes such as the glucose-regulated protein 78 (GRP78 or BiP or HSPA5), a chaperone that binds preferentially to the unfolded proteins.
Accumulative evidence has implicated UPR proteins in physiological processes beyond the control of protein folding . In those instances, ERN1, PERK, and ATF6 can be activated without the presence of misfolded proteins and the dissociation of GRP78, and the final outcome is different from that triggered by the ER stress [12, 13].
Drug discovery efforts have recently identified the UPR proteins as therapeutic targets to treat several diseases . However, although the expression and roles of some individual UPR genes have been investigated in OA [15, 16], the global response of chondrocytes to ER stress has not been looked at. The present study had two major aims. The first one was the evaluation of the global expression of the UPR genes in normal and OA chondrocytes in response to an induced ER stress (I-UPR conditions) in order to assess their impact during OA. Importantly, our second aim was to examine how the deregulation of the major representative ER stress sensors could affect cartilage metabolism under conditions where an ER stress is not induced (homeostatic or H-UPR).
Human normal cartilage was obtained from femoral condyles and tibial plateaus from individuals within 12 hours of death (n = 18, 60 ± 19 years [mean age ± standard deviation (SD)]) and OA cartilage from patients undergoing total knee arthroplasty (n = 42, 69 ± 9 years). Human normal individuals had no history of joint disease and died of causes unrelated to arthritic diseases. The cartilage was examined macroscopically and microscopically to ensure that only normal tissue was used. All OA patients had been evaluated by a certified rheumatologist and diagnosed as having OA according to the American College of Rheumatology criteria . These specimens represented moderate-to-severe OA. The Institutional Ethics Committee Board of the University of Montreal Hospital Research Centre (CRCHUM) approved the use of the human articular tissues and patients signed informed consent.
Human chondrocytes were released from the cartilage as described , seeded at high density (105/cm2), and cultured in Dulbecco’s modified Eagle’s medium (DMEM; Wisent, St-Bruno, QC, Canada) supplemented with 10 % heat-inactivated fetal bovine serum (FBS; PAA Laboratories Inc., Etobicoke, ON, Canada) and an antibiotic mixture (100 units/ml penicillin base and 100 μg/ml streptomycin base; Wisent) at 37 °C in a humidified atmosphere of 5 % CO2/95 % air. To preserve the chondrocyte phenotype, primary cells were used when comparing expression levels in normal and OA chondrocytes, and first-passage for experiments involving cultured cells. Of note, the cartilage and chondrocyte data are representative of independent assays and ‘n’ indicates the number of different patients.
An ER stress response was triggered by treating chondrocytes with Tm (500 ng/ml) or Tg (50 nM) for 20 hours in DMEM containing 10 % fetal bovine serum (FBS); under those conditions, neither Tg nor Tm affected cell viability (n = 8) as determined by the Thiazolyl Blue Tetrazolium Bromide (MTT, Sigma-Aldrich, Oakville, ON, Canada) assay as described  with modification . The basal activation of the ER stress response in OA chondrocytes was determined by monitoring the three main sensors (ERN1, PERK, and ATF6B). OA chondrocytes were incubated without (basal control) and with Tg (50 nM) and Tm (500 ng/ml) for 20 minutes as controls for induced ER stress activation. The phosphorylation status of PERK was assessed by immunohistochemistry (IHC), the cleavage of ATF6B was assessed by Western blots using a specific antibody (see below), and the spliced forms of X-box binding protein 1 (XBP1) (target of ERN1) were monitored by polymerase chain reaction (PCR) using specific primers.
Gene regulation was performed by treating cells with growth factors and cytokines for 24 hours in DMEM containing 0.5 % FBS. Activin A (ActA), transforming growth factor beta (TGF-β), platelet-derived growth factor-BB (PDGF-BB), interleukin-4 (IL-4), IL-6, and IL-8 were used at a concentration of 10 ng/ml, IL-1β at 100 pg/ml, and tumour necrosis factor alpha (TNF-α) at 5 ng/ml.
Overall expression of 84 key UPR genes was determined with the RT2 Profiler PCR Arrays (PAHS-089Z; Qiagen, Venlo, The Netherlands) on an ABI 7900HT qPCR instrument (Applied Biosystems, Foster City, CA, USA) equipped with SDS 2.3 software, using RT2 SYBR Green ROX qPCR Master Mix (Qiagen). Total ribonucleic acid (RNA) from human chondrocytes was isolated and reverse-transcribed according to the manufacturer’s instructions. Data were analyzed by the 2-ΔΔCt method. The relative quantity of complementary deoxyribonucleic acid (cDNA) was calculated using ribosomal protein large PO (RPLPO) as internal controls. All the PCR array data have been submitted to the Gene Expression Omnibus (GEO) public repository with the accession numbers GSE73749 (normal versus OA), GSE73748 (effect of Tm) and GSE73746 (effect of Tg).
Quantification of mRNA and qPCR
Total RNA was extracted and messenger RNA (mRNA) levels quantified by real-time PCR (qPCR) with the SYBR Green PCR Master Mix (Qiagen) as described . For total RNA quantification of expression between normal and OA chondrocytes, internal standards were added at known concentrations in the PCR reactions so as to give absolute numbers. The values of each sample were calculated as the ratio of the number of molecules of the target gene/number of molecules of the housekeeping gene. When evaluating the effect of a treatment, the expression level of each control was assigned an arbitrary value of 1, and the treated cells were evaluated as fold change over control and calculated as 2-ΔΔCt. Primer efficiencies for the genes under study were the same as those for the housekeeping gene, RPLPO. The sequences of the human specific primers used are listed in Additional file 1.
The localization of ERN1, PERK, ATF6B, and CREB3L2 in normal and OA cartilage was determined by IHC as previously described . In brief, the cartilage was fixed in TissuFix (Chaptec, Montreal, QC, Canada) and embedded in paraffin. Sections (5 μm) were deparaffinized in xylene followed by a graded series of alcohol washes. Sections were treated with 1 % hyaluronidase for 60 minutes at 37 °C (ERN1 only), 0.25 units/ml protease-free chondroitinase ABC in 0.1 M Tris acetate (Sigma-Aldrich), 0.3 % Triton for 30 minutes and 3 % H2O2 for 15 minutes at room temperature and proteinase K (20 μg/ml, 10 minutes at 37 °C for CREB3L2 only). 2 % goat serum (Vector Laboratories, Burlington, ON, Canada) was used for 45 minutes at room temperature to block unspecific staining prior to the addition of the primary antibodies.
The primary antibodies were diluted in goat serum and incubated overnight at 4 °C. Primary antibodies were all rabbit anti-human against ERN1 (monoclonal immunoglobulin G (IgG) 1/50; Cell Signaling Technology, Danvers, MA, USA), PERK (monoclonal IgG 1/100; Cell Signaling Technology), phosphorylated PERK (pPERK) (polyclonal IgG, 1/50, Santa Cruz Biotechnology, Santa Cruz, CA, USA), ATF6B (polyclonal IgG 1/100; Abcam, Cambridge, MA, USA), and CREB3L2 (polyclonal IgG 1/25; Santa Cruz Biotechnology). The tissues were washed in phosphate-buffered saline (PBS), then incubated with a secondary anti-rabbit antibody using a Vectastain ABC kit (Vector Laboratories) following the manufacturer’s instructions. The staining was developed with 3,3′-diaminobenzidine containing hydrogen peroxide, and sections were counterstained with eosin (0.03 % in 80 % ethanol). The eosin staining offers a good cell contrast allowing visualization of all the cells. Control procedures were performed by a substitution of the primary antibody with a nonspecific rabbit IgG (Santa Cruz Biotechnology) following the same experimental protocol; the results showed only background staining as illustrated in Additional file 2.
Antigen levels were quantified as described . The total number of chondrocytes and the number of positively stained chondrocytes were quantitated separately for each zone of the cartilage. The final results are expressed as the percentage of positively stained chondrocytes.
Small interfering RNA (siRNA; Ambion-Life Technologies, Waltham, MA, USA) specific for the genes under study were transfected into the chondrocytes as described  for 48 hours (gene expression) or 72 hours (protein production). Cells either non-transfected or transfected with non-targeting (random) siRNAs (ON-TARGETplus Non-targeting siRNA; Dharmacon, Lafayette, CO, USA) served as controls and gave similar results. RNA was quantitated by qPCR and data normalized to the housekeeping gene RPLPO. When monitoring the effect of IL-1β on gene expression in the silenced chondrocytes, the cells were first transfected for 24 hours with the siRNAs, then IL-1β (100 pg/ml) was added and the cells incubated for another 24 hours in DMEM containing 0.5 % FBS.
Total cellular proteins were extracted and processed for Western blotting as described . For the silencing experiments, the primary antibodies were those used for the IHC assays with dilutions of 1/2000 (ERN1), 1/1000 (PERK and ATF6B) and 1/100 (CREB3L2). The secondary antibody was an anti-rabbit IgG (1/10,000; Pierce, Rockford, IL, USA). Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) (monoclonal IgG, 1/20,000, Cell Signaling Technology) was used as the housekeeping (control) protein.
Values are expressed as mean ± standard error of the mean (SEM). Statistical significance was assessed with the unpaired t test or a one-sample t test where appropriate; a p value ≤0.05 was considered significant.
Several UPR genes are differentially expressed between normal and OA chondrocytes
UPR genes having 1.3-fold change expression in human chondrocytes as determined by PCR array*
A) Osteoarthritic chondrocytes (n = 3) compared to normal chondrocytes (n = 3)
B) Osteoarthritic chondrocytes (n = 3) treated with thapsigargin (50 nM) compared to untreated (control) chondrocytes
C) Osteoarthritic chondrocytes (n = 3) treated with tunicamycin (500 ng/ml) compared to untreated (control) chondrocytes
Next, we looked at whether the expression of ERN1, PERK, ATF6B, and CREB3L2 was reflected in protein production by performing IHC directly on cartilage to determine both the amount and location in the cartilage of the proteins tested. The number of chondrocytes that stained positive for ERN1 (Fig. 1a) and ATF6B (Fig. 1c), was less than 5 % in the lower zone of the cartilage, whereas PERK (Fig. 1b) and CREB3L2 (Fig. 1d) were detected in both the upper and lower zones of the cartilage, although at a reduced level in the lower zone compared to the upper zone. ERN1, PERK, and CREB3L2 production was significantly reduced in the upper zone of the OA cartilage, but ATF6B was similar in both normal and OA cartilage. The IHC data (from cartilage) mirrored the qPCR data (from isolated chondrocytes), indicating that the expression/production of the representatives of the three main branches of the ER stress response are downregulated in OA chondrocytes/cartilage.
Basal activation status of the ER stress response in OA chondrocytes
When activated by ER stress, ATF6B (approximately 75 kDa) is cleaved into fragments, one of which acts as a transcription factor following its transfer to the nucleus. The cleavage of ATF6B was assayed by Western blot with an antibody recognizing the C-terminus of the protein. Samples treated with Tg (50 nM) and Tm (500 ng/ml), agents well known to induce an ER stress response (I-UPR conditions), were included as controls for the cleavage of the protein. As illustrated in Fig. 2b, Tg or Tm treatments significantly reduced the levels of the uncleaved ATF6B in OA chondrocytes, suggesting that if activated, it is not at its maximal levels. Although the antibody could in theory also detect the small cleaved fragment, under our experimental conditions this fragment was barely detectable, possibly due to further degradation.
The presence of the XBP1-spliced mRNA was determined by PCR with primers that amplify both the unspliced (amplification product of 145 bp) and spliced (amplification product of 119 bp) forms. Samples treated with Tg (50 nM) and Tm (500 ng/ml) were also included as controls of XBP1 mRNA splicing. Data (Fig. 2c) show that the unspliced mRNA was the only XBP1 mRNA species detected in all the untreated OA cells. This is in contrast to the Tg- and Tm-treated OA chondrocytes, which showed only the activated (spliced) XBP1 mRNA species.
Taken together, these results indicate that the ER stress response is not globally or fully activated in OA chondrocytes.
Regulation of UPR genes under I-UPR conditions in normal and OA chondrocytes
Expression of UPR genes in response to treatment with thapsigargin and tunicamycin in human chondrocytes
5.29 ± 1.49
7.15 ± 0.61
3.76 ± 1.12
4.12 ± 0.36
3.54 ± 0.34
2.52 ± 0.21
2.18 ± 0.48
1.59 ± 0.12
1.05 ± 0.06
0.82 ± 0.08
1.07 ± 0.30
0.86 ± 0.12
1.15 ± 0.26
1.38 ± 0.34
1.15 ± 0.20
1.20 ± 0.16
38.54 ± 6.27
35.68 ± 4.45
19.18 ± 2.40
16.74 ± 2.31
22.08 ± 6.72
25.64 ± 6.49
13.66 ± 3.06
6.34 ± 1.66
15.04 ± 4.37
12.33 ± 1.77
9.56 ± 2.86
7.76 ± 0.75
0.79 ± 0.11
0.84 ± 0.11
0.51 ± 0.09
0.68 ± 0.09
Regulation and role of UPR genes under H-UPR conditions
As the role of UPR proteins under I-UPR conditions has already been investigated [24–26], we further explored the regulation and role of the UPR genes under H-UPR conditions. To this end, we hypothesized that some of those proteins played a role under H-UPR conditions, different from those under I-UPR. We first looked at factors that could be responsible, under homeostatic conditions, for the downregulation of ERN1, PERK, and CREB3L2 in OA chondrocytes and secondly determined their potential role in regulation of genes involved in OA pathology.
ERN1, PERK, and CREB3L2 expression is downregulated by PDGF-BB and IL-6 in OA chondrocytes
We have shown that the expression of ERN1 and PERK was decreased in OA cells and that IL-1β increased PERK and ERN1 expression. As IL-1β is known to be increased in OA , we further determined whether the presence of PDGF-BB and IL-6 could interfere with the upregulation of ERN1 and PERK by IL-1β. To this end, OA chondrocytes were monitored for the expression of IL-1β following PDGF-BB and IL-6 treatments. Data show that treatment of OA chondrocytes with PDGF-BB resulted in a significantly decreased expression of IL-1β (n = 6, mean fold change over control ± SEM 0.50 ± 0.13, p = 0.013 [one-sample t test]), but that treatment with IL-6 did not significantly affect IL-1β expression (n = 6, 1.8 ± 1.0, p = 0.437). These results show that the presence of PDGF-BB can interfere with the expression levels of IL-1β and ultimately those of ERN1 and PERK.
ERN1, PERK, ATF6B, and CREB3L2 regulate collagen and protease gene expression
Thus, under H-UPR conditions, increasing PERK may contribute to an increase in type II collagen and a decrease in type I collagen expression, whereas increasing ERN1, ATF6B, and CREB3L2 could have detrimental effects as they would upregulate MMP-13, ADAMTS4, and ADAMTS5, known catabolic factors involved in cartilage destruction.
As IL-1β is an important factor in the regulation of collagen and protease genes, we examined whether the decreased expression of ERN1, PERK, ATF6B, or CREB3L2 affected its action. IL-1β significantly reduced COL2a1 and increased MMP-13 (data not shown), ADAMTS4, and ADAMTS5 expression (Fig. 4b), but did not affect COL1a1 expression (data not shown). Silencing ERN1 did not affect the stimulatory effect of IL-1β on MMP-13 and ADAMTS4 or its inhibitory effect on COL2a1 (data not shown). IL-1β did not maximally stimulate ADAMTS4 in the silenced ATF6B or ADAMTS5 in the silenced CREB3L2 chondrocytes (Fig. 4b). IL-1β did not affect COL1a1 in PERK-silenced chondrocytes (data not shown), but significantly reduced COL2a1 (Fig. 4b). Thus, a lower expression of PERK has a twofold effect: it reduces COL2a1 expression and, in the presence of IL-1β such as occurs in OA, the COL2a1 expression is further reduced.
The event that triggers the initiation of OA is still a matter of intense research. OA is a multifactorial process with several factors contributing to the degradation of the cartilage. In this work, we examined whether OA was characterized by an overall activation of the ER stress response. We first looked at the global expression of UPR genes in human OA chondrocytes, the activation status of the ER stress sensors, and the response of OA cells under induced (I)-UPR conditions. We found that despite the decreased expression/production of several UPR genes in OA, the global induced ER stress response is similar to that of normal chondrocytes, and that the three main sensors of the ER stress were not activated or fully activated in OA cells. Based on these data, OA is not likely the result of an overall activation of the ER stress pathways. Interestingly, data revealed that the reduced expression of the UPR genes could influence the progression of OA under homeostatic (H)-UPR conditions, in which ERN1, PERK, and CREB3L2 can act as regulators of some collagens/MMPs. As the decrease in PERK favours a reduced expression of type II collagen (COL2a1) and increased type I collagen, these findings lead us to propose PERK as a potential target for OA therapeutic strategies. However, further studies are needed to confirm this finding.
Our finding that OA cells are not characterized by an increased activation of the ER stress response is in contrast to previous reports suggesting that GRP78 and phosphorylated PERK increased with the severity of cartilage degeneration [15, 16]. However, Takada et al  only looked at OA cartilage and indeed detected activated pPERK in this tissue, as we found in our OA samples. The amount of pPERK in our OA samples, however, was not greater than that found in the normal cartilage. Takada et al  also investigated the presence, by gel electrophoresis, of the XBP1 spliced form. They looked at OA human cartilage samples but from different regions named mild, moderate, and severe degeneration from the same knee. They showed that the spliced form of XBP1 was barely or not at all detectable in the mild and severe regions of the cartilage. Although present in moderate OA cartilage, it was less abundant than the unspliced form, indicating that the XBP1 spliced form was not the major form expressed. In our study, we used cartilage samples taken from the whole OA knee to obtain a global picture of XBP1 activity and did not detect the spliced form.
We have shown that PDGF-BB and IL-6 will add to the degenerative process of OA through the downregulation of ERN1 and PERK, which, in turn, will affect collagen expression. This finding adds to the known effects of PDGF-BB on chondrocyte proliferation, differentiation and proteoglycan production , and downregulation of the IL-1β-induced nuclear factor kappa B (NF-kB) signalling . Data also revealed a new role for IL-6, known as an independent predictor of the appearance of knee OA, for its association with local inflammation [30, 31], and for its capacity to downregulate the expression of type II collagen . As we have shown that IL-6 decreases ERN1 and PERK expression and that a decrease in these two proteins leads to a decreased expression of type II collagen, these data illustrate the versatility of action of this cytokine on type II collagen expression in OA chondrocytes.
The finding that IL-1β upregulated ERN1 and PERK was unexpected, considering that their expression was decreased in OA chondrocytes and that IL-1β is known to be increased in diseased cartilage . It is possible that the increased presence of PDGF-BB in the OA cartilage  would have a threefold effect: a decreased expression of ERN1 and PERK by directly reducing their expression, a decreased IL-1β expression as our results have shown, and an interference with the stimulatory effect of IL-1β on those genes .
An emerging finding is that, under homeostasis, the decreased expression of the UPR genes ERN1, PERK, ATF6B, and CREB3L2 in human chondrocytes will affect the regulation of some collagens/MMPs. As reported in other systems, PERK and ERN1 play dual roles depending on whether they are activated by physiological factors or by ER stress and the cellular response will differ depending on the stimuli. For instance, Lipson et al  reported that activation of ERN1 in pancreatic β cells transiently exposed to high glucose resulted in an increased insulin biosynthesis not involving the activation of the ER stress response, but that a chronic exposure to high glucose triggered the ER stress response and the suppression of the insulin gene expression. Another example of the role of UPR genes in the absence of ER stress has been shown in endothelial cells, where vascular endothelial growth factor (VEGF) signals through ATF6 and PERK via the mammalian target of rapamycin complex 1 (mTORC1) complex . In the present study, we identify ERN1 and PERK as regulators of collagen and protease expression in OA chondrocytes under H-UPR conditions. The regulation of collagen synthesis in chondrocytes is crucial as the type of collagen produced influences the quality of the cartilage matrix. In OA, there is a loss of the structural collagen, the type II, and an increase in type I collagen known to weaken the cartilage, which undermine the integrity of the extracellular cartilage matrix, in turn affecting the cartilage properties. Our data showing that a decreased expression of ERN1 and PERK in OA chondrocytes could induce a decreased expression of type II collagen and, in the case of PERK, an increased expression of type I collagen, are of great importance as this would favour a microenvironment change in the extracellular matrix and contribute to the degeneration process. In turn, increasing the molecules ERN1 and PERK in OA cartilage could be foreseen as having therapeutic potential. However, as ERN1, ATF6B, and CREB3L2 affect proteases involved in cartilage degradation, their usage during OA could be detrimental. In contrast, an increase in PERK, in addition to acting in a reverse manner on both types of collagen, could also counteract the inhibitory effect of IL-1β on type II collagen.
In conclusion, we showed that the level of ER stress is not significantly elevated in OA chondrocytes. Furthermore, under I-UPR conditions, OA chondrocytes respond strongly to ER stress despite the decreased expression of several ER stress genes. Importantly, and for the first time, this study reveals new roles for ERN1, PERK, ATF6B, and CREB3L2 in cartilage under H-UPR conditions as regulators of collagen and/or protease genes, and identifies PERK as a potential target for new therapeutic strategies for OA as increasing PERK may lead to an increase in type II collagen and a decrease in type I collagen expression and, in so doing, could restore to some extent homeostatic conditions in OA cartilage.
ActA, Activin A; ADAMTS, a disintegrin and metalloproteinase with thrombospondin motifs; ATF6, activating transcription factor 6; cDNA, complementary DNA; CREB3L2, CAMP-responsive element-binding protein 3-like 2; DDIT3, DNA damage-inducible transcript 3; DMEM, Dulbecco’s modified Eagle’s medium; DNA, deoxyribonucleic acid; DNAJB9, DnaJ (Hsp40) homolog, subfamily B, member 9; ER, endoplasmic reticulum; ERN 1, endoplasmic reticulum to nucleus 1; ERO1LB, ERO1-like beta (S. Cerevisiae); FBS, fetal bovine serum; GAPDH, glyceraldehyde-3-phosphate dehydrogenase; GRP78, glucose-regulated protein 78; HERPUD1, homocysteine-inducible, endoplasmic reticulum stress-inducible, ubiquitin-like domain member 1; H-UPR, homeostatic unfolded protein response; IgG, immunoglobulin G; IHC, immunohistochemistry; IL, interleukin; I-UPR, induced unfolded protein response; MMP, matrix metalloproteinases; mRNA, messenger RNA; mTORC1, mammalian target of rapamycin complex 1; NF-kB, nuclear factor kappa B; NRF2, nuclear factor erythroid 2; OA, osteoarthritis; OASIS, old astrocyte specifically induced substance; PCR, polymerase chain reaction; PDGF-BB, platelet-derived growth factor-BB; PERK, PRKR-like endoplasmic reticulum kinase; pPERK, phosphorylated PERK; qPCR, quantitative real-time PCR; RNA, ribonucleic acid; RPLPO, ribosomal protein large PO; SD, standard deviation; SEM, standard error of mean; siRNA, small interfering RNA; SREBP2, sterol regulatory element-binding protein 2; Tg, thapsigargin; TGF-β, transforming growth factor beta; Tm, tunicamycin; TNF-α, tumour necrosis factor alpha; UPR, unfolded protein response; VEGF, vascular endothelial growth factor; XBP1, X-box binding protein 1
The authors acknowledge Frédéric Paré and François Mineau for their expert technical skills and Virginia Wallis for her assistance with the manuscript preparation.
The study was funded by the Osteoarthritis Research Unit of the University of Montreal Hospital Research Centre (CRCHUM) and by the Chair in Osteoarthritis of the University of Montreal.
Availability of data and materials
All the PCR array data have been submitted to the Gene Expression Omnibus (GEO) public repository with the accession numbers GSE73749 (normal versus osteoarthritis), GSE73748 (effect of Tm) and GSE73746 (effect of Tg).
YHL, GT, MK, JPP, and JMP conceived the study. YHL, GT, DH, HF, and JMP were responsible for the data collection and analysis. GT and JMP interpreted the data. YHL, GT, and JMP undertook the literature search. GT, DH, and JMP generated the figures. YHL, GT, DH, MK, HF, JPP, and JMP were involved in the drafting or critical revision of the manuscript and approved the final submitted version.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
The Institutional Ethics Committee Board of the University of Montreal Hospital Research Centre (CRCHUM) approved the use of the human articular tissues and patients signed informed consent.
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- Wictome M, Henderson I, Lee AG, East JM. Mechanism of inhibition of the calcium pump of sarcoplasmic reticulum by thapsigargin. Biochem J. 1992;283(Pt 2):525–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Reiling JH, Clish CB, Carette JE, Varadarajan M, Brummelkamp TR, Sabatini DM. A haploid genetic screen identifies the major facilitator domain containing 2A (MFSD2A) transporter as a key mediator in the response to tunicamycin. Proc Natl Acad Sci U S A. 2011;108(29):11756–65.View ArticlePubMedPubMed CentralGoogle Scholar
- Bukau B, Weissman J, Horwich A. Molecular chaperones and protein quality control. Cell. 2006;125(3):443–51.View ArticlePubMedGoogle Scholar
- Bernales S, Papa FR, Walter P. Intracellular signaling by the unfolded protein response. Annu Rev Cell Dev Biol. 2006;22:487–508.View ArticlePubMedGoogle Scholar
- Malhotra JD, Kaufman RJ. The endoplasmic reticulum and the unfolded protein response. Semin Cell Dev Biol. 2007;18(6):716–31.View ArticlePubMedPubMed CentralGoogle Scholar
- Boot-Handford RP, Briggs MD. The unfolded protein response and its relevance to connective tissue diseases. Cell Tissue Res. 2010;339(1):197–211.View ArticlePubMedGoogle Scholar
- Hetz C. The unfolded protein response: controlling cell fate decisions under ER stress and beyond. Nat Rev Mol Cell Biol. 2012;13(2):89–102.PubMedGoogle Scholar
- Walter P, Ron D. The unfolded protein response: from stress pathway to homeostatic regulation. Science. 2011;334(6059):1081–6.View ArticlePubMedGoogle Scholar
- Asada R, Kanemoto S, Kondo S, Saito A, Imaizumi K. The signalling from endoplasmic reticulum-resident bZIP transcription factors involved in diverse cellular physiology. J Biochem. 2011;149(5):507–18.View ArticlePubMedGoogle Scholar
- Hai T, Hartman MG. The molecular biology and nomenclature of the activating transcription factor/cAMP responsive element binding family of transcription factors: activating transcription factor proteins and homeostasis. Gene. 2001;273(1):1–11.View ArticlePubMedGoogle Scholar
- Saito A, Hino S, Murakami T, Kanemoto S, Kondo S, Saitoh M, et al. Regulation of endoplasmic reticulum stress response by a BBF2H7-mediated Sec23a pathway is essential for chondrogenesis. Nat Cell Biol. 2009;11(10):1197–204.View ArticlePubMedGoogle Scholar
- Lipson KL, Fonseca SG, Ishigaki S, Nguyen LX, Foss E, Bortell R, et al. Regulation of insulin biosynthesis in pancreatic beta cells by an endoplasmic reticulum-resident protein kinase IRE1. Cell Metab. 2006;4(3):245–54.View ArticlePubMedGoogle Scholar
- Karali E, Bellou S, Stellas D, Klinakis A, Murphy C, Fotsis T. VEGF signals through ATF6 and PERK to promote endothelial cell survival and angiogenesis in the absence of ER stress. Mol Cell. 2014;54(4):559–72.View ArticlePubMedGoogle Scholar
- Rutkowski DT, Hegde RS. Regulation of basal cellular physiology by the homeostatic unfolded protein response. J Cell Biol. 2010;189(5):783–94.View ArticlePubMedPubMed CentralGoogle Scholar
- Takada K, Hirose J, Senba K, Yamabe S, Oike Y, Gotoh T, et al. Enhanced apoptotic and reduced protective response in chondrocytes following endoplasmic reticulum stress in osteoarthritic cartilage. Int J Exp Pathol. 2011;92(4):232–42.View ArticlePubMedPubMed CentralGoogle Scholar
- Nugent AE, Speicher DM, Gradisar I, McBurney DL, Baraga A, Doane KJ, et al. Advanced osteoarthritis in humans is associated with altered collagen VI expression and upregulation of ER-stress markers Grp78 and bag-1. J Histochem Cytochem. 2009;57(10):923–31.View ArticlePubMedPubMed CentralGoogle Scholar
- Altman RD, Asch E, Bloch DA, Bole G, Borenstein D, Brandt KD, et al. Development of criteria for the classification and reporting of osteoarthritis. Classification of osteoarthritis of the knee. Arthritis Rheum. 1986;29:1039–49.View ArticlePubMedGoogle Scholar
- Tardif G, Pelletier JP, Boileau C, Martel-Pelletier J. The BMP antagonists follistatin and gremlin in normal and early osteoarthritic cartilage: an immunohistochemical study. Osteoarthritis Cartilage. 2009;17(2):263–70.View ArticlePubMedGoogle Scholar
- Mosmann T. Rapid colorimetric assay for cellular growth and survival: application to proliferation and cytotoxicity assays. J Immunol Methods. 1983;65:55–63.View ArticlePubMedGoogle Scholar
- Notoya K, Jovanovic DV, Reboul P, Martel-Pelletier J, Mineau F, Pelletier JP. The induction of cell death in human osteoarthritis chondrocytes by nitric oxide is related to the production of prostaglandin E2 via the induction of cyclooxygenase-2. J Immunol. 2000;165:3402–10.View ArticlePubMedGoogle Scholar
- Tardif G, Pelletier JP, Fahmi H, Hum D, Zhang Y, Kapoor M, et al. NFAT3 and TGF-beta/SMAD3 regulate the expression of miR-140 in osteoarthritis. Arthritis Res Ther. 2013;15(6):R197.View ArticlePubMedPubMed CentralGoogle Scholar
- Tardif G, Hum D, Pelletier JP, Boileau C, Ranger P, Martel-Pelletier J. Differential gene expression and regulation of the bone morphogenetic protein antagonists follistatin and gremlin in normal and osteoarthritic human chondrocytes and synovial fibroblasts. Arthritis Rheum. 2004;50(8):2521–30.View ArticlePubMedGoogle Scholar
- Fan Z, Tardif G, Boileau C, Bidwell JP, Geng C, Hum D, et al. Identification in human osteoarthritic chondrocytes of proteins binding to the novel regulatory site AGRE in the human matrix metalloprotease 13 proximal promoter. Arthritis Rheum. 2006;54(8):2471–80.View ArticlePubMedGoogle Scholar
- Oliver BL, Cronin CG, Zhang-Benoit Y, Goldring MB, Tanzer ML. Divergent stress responses to IL-1beta, nitric oxide, and tunicamycin by chondrocytes. J Cell Physiol. 2005;204(1):45–50.View ArticlePubMedGoogle Scholar
- Yang L, Carlson SG, McBurney D, Horton Jr WE. Multiple signals induce endoplasmic reticulum stress in both primary and immortalized chondrocytes resulting in loss of differentiation, impaired cell growth, and apoptosis. J Biol Chem. 2005;280(35):31156–65.View ArticlePubMedGoogle Scholar
- Uehara Y, Hirose J, Yamabe S, Okamoto N, Okada T, Oyadomari S, et al. Endoplasmic reticulum stress-induced apoptosis contributes to articular cartilage degeneration via C/EBP homologous protein. Osteoarthritis Cartilage. 2014;22(7):1007–17.View ArticlePubMedGoogle Scholar
- Martel-Pelletier J, Lajeunesse D, Pelletier JP. Etiopathogenesis of osteoarthritis. In: Koopman WJ, Moreland LW, eds. Arthritis & Allied Conditions. A Textbook of Rheumatology. 15th ed. Baltimore: Lippincott, Williams & Wilkins; 2005. p. 2199-226.Google Scholar
- Kieswetter K, Schwartz Z, Alderete M, Dean DD, Boyan BD. Platelet derived growth factor stimulates chondrocyte proliferation but prevents endochondral maturation. Endocrine. 1997;6(3):257–64.View ArticlePubMedGoogle Scholar
- Montaseri A, Busch F, Mobasheri A, Buhrmann C, Aldinger C, Rad JS, et al. IGF-1 and PDGF-bb suppress IL-1beta-induced cartilage degradation through down-regulation of NF-kappaB signaling: involvement of Src/PI-3 K/AKT pathway. PLoS One. 2011;6(12):e28663.View ArticlePubMedPubMed CentralGoogle Scholar
- Livshits G, Zhai G, Hart DJ, Kato BS, Wang H, Williams FM, et al. Interleukin-6 is a significant predictor of radiographic knee osteoarthritis: The Chingford Study. Arthritis Rheum. 2009;60(7):2037–45.View ArticlePubMedPubMed CentralGoogle Scholar
- Pearle AD, Scanzello CR, George S, Mandl LA, DiCarlo EF, Peterson M, et al. Elevated high-sensitivity C-reactive protein levels are associated with local inflammatory findings in patients with osteoarthritis. Osteoarthritis Cartilage. 2007;15(5):516–23.View ArticlePubMedGoogle Scholar
- Poree B, Kypriotou M, Chadjichristos C, Beauchef G, Renard E, Legendre F, et al. Interleukin-6 (IL-6) and/or soluble IL-6 receptor down-regulation of human type II collagen gene expression in articular chondrocytes requires a decrease of Sp1.Sp3 ratio and of the binding activity of both factors to the COL2A1 promoter. J Biol Chem. 2008;283(8):4850–65.View ArticlePubMedGoogle Scholar
- Moos V, Fickert S, Muller B, Weber U, Sieper J. Immunohistological analysis of cytokine expression in human osteoarthritic and healthy cartilage. J Rheumatol. 1999;26:870–9.PubMedGoogle Scholar