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PRMT5 inhibition attenuates cartilage degradation by reducing MAPK and NF-κB signaling

Arthritis Research & Therapy volume 22, Article number: 201 (2020) Cite this article

Abstract

Objectives

A role for the type II arginine methyltransferase PRMT5 in various human diseases has been identified. In this study, the potential mechanism underlying the involvement of PRMT5 in the pathological process leading to osteoarthritis (OA) was investigated.

Methods

PRMT5 expression in cartilage tissues from patients with OA and control individuals was assessed by immunohistochemical staining. The regulatory and functional roles of PRMT5 in the chondrocytes of patients with OA and control individuals were determined by western blotting and reverse transcription polymerase chain reaction. The effects of the PRMT5 inhibitor EPZ on interleukin-1β-induced inflammation were examined in the chondrocytes of patients with OA and in the destabilized medial meniscus (DMM) of a mouse model of OA.

Results

PRMT5 was specifically upregulated in the cartilage of patients with OA. Moreover, adenovirus-mediated overexpression of PRMT5 in human chondrocytes caused cartilage degeneration. This degeneration was induced by elevated expression levels of matrix-degrading enzymes (matrix metalloproteinase-3 (MMP-3) and matrix metalloproteinase-13 (MMP-13)) in chondrocytes. The activation of the MAPK and nuclear factor κB signaling pathways was evidenced by elevated levels of p-p65, p-p38, and p-JNK. These effects were attenuated by inhibiting the expression of PRMT5. In the mouse model, EPZ inhibited PRMT5 expression, thus protecting mouse cartilage from DMM-induced OA.

Conclusions

Our results demonstrate that PRMT5 is a crucial regulator of OA pathogenesis, implying that EPZ has therapeutic value in the treatment of this cartilage-destroying disease.

Introduction

Osteoarthritis (OA) is a whole-joint disease characterized by chronic joint pain and loss of function, which occurs in 50% of the population ≥ 65 years of age [1, 2]. The development of OA includes degeneration of the articular cartilage, induction of a synovial inflammatory response, formation of osteophytes, and remodeling of the subchondral bone [3]. Among these pathological changes, cartilage degeneration is the key feature of OA; this is caused by activation of matrix-degrading enzymes, such as matrix metalloproteinase-3 (MMP-3) and matrix metalloproteinase-13 (MMP-13) [4,5,6]. Both enzymes are regulated by inflammatory cytokines (e.g., tumor necrosis factor α and interleukin (IL)-1β), which are released by chondrocytes [7, 8] and induce the production of MMPs by activating the nuclear factor (NF)-κB and mitogen-activated protein kinase (MAPK) cellular signaling pathways [9, 10]. Necrostatin-1, a cellular catabolic mediator in chondrocytes, also plays a role in OA: it upregulates matrix-degrading enzymes induced by IL-1β [11].

Arginine methylation is a post-translational modification commonly found in mammalian cells and catalyzed by proteins of the arginine methyltransferase (PRMT) family [12, 13]. PRMT5, a type II enzyme, is found in both the cytoplasm and the nucleus of cells [14, 15]; it is involved in many physiological processes, including adipogenesis [16], hematopoiesis [17], and spermatogenesis [18, 19]. The overexpression of PRMT5 in various tumors and in leukemia has also been reported [19,20,21]. Recent studies indicate that PRMT5 participates in the maintenance of chondrogenic progenitor cells in the limb bud [22]. It is also involved in inflammation, migration of fibroblast-like synoviocytes in rheumatoid arthritis, and induction of an inflammatory reaction in the endothelium [23, 24]. In addition, several studies have shown that PRMT5 regulates the NF-κB pathway [25,26,27,28], both via TRAIL [25] and by dimethylation of R30 on the p65 subunit [26].

Here, we report the specific upregulation of PRMT5 in human OA cartilage and show that the inhibition of PRMT5 expression attenuates IL-1β-mediated MMP-3 and MMP-13 expression levels through activation of the MAPK and NF-κB signaling pathways of chondrocytes. These results imply that PRMT5 acts as a catabolic regulator in the pathogenesis of OA.

Materials and methods

Clinical sample collection

Clinical specimens (cartilage) were obtained from three patients with OA (two women and one man; age 67.1 ± 8.4 years, range 58–75 years) who underwent total knee arthroplasty. The three patients in the control group (two women and one man; age 30.1 ± 5.6 years, range 18–42 years) underwent total knee arthroplasty related to osteosarcoma involving the knee joint patients; they had no history of OA. All surgeries were performed at the People’s Hospital of Zhengzhou University (Zhengzhou, China). The study was approved by the hospital’s Clinical Research Ethics Committee (approval no. 2017237), and informed consent was obtained from each tissue donor prior to inclusion in this study.

Animal models

Male C57BL/6 mice (12 weeks old and weighing 20–25 g) used in this study were housed at the Experimental Animal Center of the People’s Hospital of Zhengzhou University and fed a standard diet under specific pathogen-free conditions. An OA model was established in the mice by destabilized medial meniscus (DMM) surgery of the right knee joint, in accordance with a previously described protocol [29]. The 30 mice were randomly divided into three groups of 10 mice each: (1) in the sham group, sham-operated mice were administered vehicle (dimethylsulfoxide); (2) in the DMM group, the mice underwent DMM surgery and were administered vehicle; (3) in the DMM+EPZ group, the mice underwent DMM surgery and were administered the PRMT5 inhibitor EPZ (200 μg/kg). Vehicle or EPZ solution was injected intra-articularly, twice per week for 8 weeks.

Approval for the animal experiments was obtained from the Institutional Animal Care and Use Committee (IACUC) at the People’s Hospital of Zhengzhou University (ethical approval code: 2018526).

Micro-computed tomography imaging

All mouse (n = 10) knee joints were scanned at 100 kV and 98 μA using microcomputed tomography (μCT) (μ-CT50 Scanco Medical, Bassersdorf, Switzerland). The resolution was set to 10.5 μM. Image reconstruction and analysis were performed using the built-in software; these were followed by three-dimensional reconstruction and structural parameter analysis. The structural parameter analysis included determinations of bone volume/tissue volume, trabecular thickness, and trabecular separation.

Histological and immunochemical analyses

Human cartilage and mouse joint tissue samples were collected and fixed in 4% formalin, then incubated for 3 weeks in 10% EDTA and embedded in paraffin. The tissues were cut into 4-μm coronal sections for hematoxylin and eosin and safranin O-Fast green staining, as well as immunohistochemistry. For cartilage analysis and scoring, safranin O-Fast green staining was performed, according to the OARSI histologic scoring system [29, 30]. Briefly, the extent of the surface damage was scored in a blinded manner at the mouse tibia (lateral tibia (LT) and medial tibia (MT)) as well as femur (lateral femur (LF) and medial femur (MF)); the score for cartilage damage was calculated in a scale of 0 (normal) to 6 (bone loss, remodeling, deformation), based on the OA depth into the cartilage. The OARSI score was calculated based on averaging of maximum score among the four articular surfaces from ten mice.

Immunohistochemistry staining was performed using the DAB tissue staining SP-kit, in accordance with the standard protocol. Tissue sections were incubated overnight with specific anti-MMP-13, MMP-3, PRMT5, p-p38, and p-p65 antibodies at 4 °C and then analyzed by optical microscopy.

Cell experiments

Cartilage samples collected from patients with OA during total knee arthroplasty were washed, cut into pieces in 4 °C sterile phosphate buffer, and digested with 0.25% trypsin at 37 °C for 30 min; they were then incubated in 0.25% collagenase II at 37 °C for 24 h. The chondrocytes were cultured in DMEM/F12 with 10% fetal bovine serum, 100 U/mL penicillin, and 100 mg/mL streptomycin at 37 °C under 5% CO2. Chondrocytes were passaged twice before use in experiments. To study the induction of inflammation, passage 3 chondrocytes were seeded on six-well plates (2 × 105 cells/well) and treated with 10 ng/mL IL-1β for 72 h (Sigma-Aldrich, St. Louis, MO, USA). Levels of PRMT5, MMP-3, MMP-13, Collagen II, Sox9, and ADAMTs5 protein were then determined. To investigate the mechanism by which PRMT5 damages articular chondrocytes, we examined the expression of p38, JNK, ERK1/2, p65, IκB, p-JNK, p-p38, p-ERK1/2, p-IκB, and p-p65 in chondrocytes that had been stimulated with IL-1β for 0, 15, and 30 min.

Micromass cultures

Micromass cultures were performed as previously described [31]. Briefly, chondrocytes were plated at a density of 2.5 × 105 cells/10-μL drop. The cell culture medium was replaced with fresh culture medium every other day. On days 5 and 7, cartilage differentiation was determined by alcian blue staining; the cartilage was then extracted using 6 M guanidine hydrochloride. The absorbance of the supernatant at 600 nm was measured using a multi-mode microplate reader (BioTek, Winooski, VT, USA).

Adenovirus vector infection

Human PRMT5 cDNA was cloned and inserted into a pHBAd-MCMV-GFP expression vector (Wuhan Miaoling Biotechnology Co. Ltd., Hubei, China). Empty vectors were used as controls. Human chondrocytes were cultured in DMEM/F-12 medium without fetal bovine serum in 12-well plates. When the cultures had reached 70% confluency, they were transduced with pHBAd-MCMV-GFP-PRMT5 (ad-PRMT5) and the vector control (ad-NC), in accordance with the manufacturer’s instructions. After the direct addition of recombinant adenoviruses to the medium, the transduced cells were incubated for 4 h; the medium was then changed to vector-free medium. Samples were collected for the measurement of protein and mRNA expression, after the virus vector infection 72 h.

RNA extraction and quantitative real-time PCR

Total RNA was extracted from human chondrocytes using TRIzol reagent (Invitrogen, Carlsbad, CA, USA), in accordance with the manufacturer’s instructions. cDNA of each sample was synthesized from 1 μg of total RNA using the Revert Aid First Strand cDNA Synthesis Kit (Thermo Scientific, Waltham, MA, USA). The mRNA expression levels of PRMT5, MMP-3, MMP-13, Collagen II, Sox9, and ADAMTs5 were measured by using the qRT-PCR method, and the relative primers are listed in Table S1. Target mRNA expression levels were normalized against GAPDH. The relative expression levels were computed using the 2−ΔΔCt method.

Western blotting

The total protein of cartilage samples from OA patients was extracted using tissue homogenizer, and then RIPA buffer supplemented with protease and phosphatase inhibitor (Boster BIO, Wuhan, China) was added and ultimately the cell lysates were centrifuged at 16000×g for 20 min to remove the tissue. Protein concentrations of the samples were determined using a BCA protein assay kit (Boster BIO, Wuhan, China). Proteins were extracted from cells using 100 μL of RIPA buffer supplemented with protease and phosphatase inhibitor. Lysates were centrifuged for 20 min at 10,000g; 20 μg of total cellular protein per sample was loaded on a 10% sodium dodecyl sulfate-polyacrylamide gel, in accordance with the manufacturer’s protocol (Boster Bio, Wuhan, China). Protein samples were then transferred to the PVDF membranes (Millipore, Billerica, MA, USA) and blocked for 1 h with 5% skim milk in Tris-buffered saline with 0.1% Tween-20. The blots were then probed overnight at 4 °C with rabbit primary antibodies against PRMT5, MMP-3, MMP-13, Collagen II, Sox9, ADAMTs5, p38, JNK, ERK1/2, p65, IκB, p-JNK, p-p38, p-ERK1/2, p-IκB, p-p65, and GAPDH. After the blots were washed three times with Tris-buffered saline with 0.1% Tween-20, they were incubated with anti-mouse or anti-rabbit secondary antibodies. Immunoreactivity was detected with enhanced chemiluminescence (Bio-Rad Laboratories, Munich, Germany).

Statistical analysis

The data are presented as means ± standard deviations of at least three independent experiments. Student’s t tests were used to analyze the differences between the two groups, and one-way analysis of variance with the SNK post hoc test was used to compare the differences among the three groups. A two-tailed p value of < 0.05 was considered to indicate statistical significance.

Results

PRMT5 is upregulated in OA chondrocytes

To study the role of PRMTT5 in the pathogenesis of OA, we measured the expression of PRMTT5 in the cartilage from OA patients or normal individuals using immunohistochemistry. The results showed that PRMT5 protein levels were markedly elevated in OA human cartilage, compared with the control group cartilage (Fig. 1a, b). Furthermore, western blotting showed upregulation of PRMT5, p-p38, and p-p65 expressions (Fig. 1c), which indicated the activation of NF-κB and MAPK subtypes in OA human cartilage.

Fig. 1
figure 1

Overexpression of PRMT5 in human osteoarthritis (OA) cartilage. a Hematoxylin and eosin staining and representative immunohistochemical staining for PRMT5 in human cartilage in the control and OA groups. Scale bar = 100 μm. b Increase in the numbers of PRMT5-positive cells in human OA cartilage vs. control cartilage. Results are presented as percentages. c Representative western blots show increases in the expression levels of PRMT5, p-p65, and p-p38 in OA tissues; levels of p65, p38, and GAPDH were identical to those in the control group. d Histogram showing the relative protein expression levels of PRMT5, p-p65, and p-p38 in cartilage tissue. Data are presented as mean ± SD from 3 samples for each group in 3 independent experiments. Data were analyzed using Student’s t test. *P < 0.05 vs. the normal group

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PRMT5 overexpression causes cartilage degeneration

The role of PRMT5 in the regulation of cartilage metabolism was investigated by the transduction of primary culture human chondrocytes with a PRMT5 adenovirus vector, which resulted in the overexpression of the protein. As shown in Fig. 2a, compared with the control group, PRMT5 overexpression induced the upregulation of MMP-3, MMP-13, and ADAMTs5, as well as the downregulation of Collagen II and Sox9. Elevated PRMT5 levels also caused the upregulation of MMP-3, MMP-13, and ADAMTs5 mRNA expression, whereas the downregulation of Collagen II and Sox9 mRNA expression was observed (Fig. 2c).

Fig. 2
figure 2

Overexpression of PRMT5 contributes to cartilage degeneration. a Expression levels of MMP-3, MMP-13, ADAMTs5, Sox9, Collagen II, and PRMT5 in human chondrocytes from the control, Ad-NC, and Ad-PRMT5 groups were determined by western blotting. b Histogram showing the relative protein expression levels of PRMT5, MMP-3, MMP-13, ADAMTs5, Sox9, and Collagen II in human chondrocytes. c Changes in MMP-3, MMP-13, PRMT5, ADAMTs5, Sox9, and Collagen II gene expression levels in human chondrocytes transduced with Ad-PRMT5. Data of independent experiments (n = 3) were presented as mean ± SD and analyzed using the one-way analysis of variance with the SNK post hoc test. *P < 0.05 vs. the Ad-NC group

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PRMT5 inhibition attenuates IL-1β-stimulated induced chondrocyte catabolism

To determine the effect of PRMT5 inhibition on IL-1β-stimulated chondrocyte degeneration, primary cultures of human chondrocytes were co-treated with EPZ in the presence or absence of IL-1β for 72 h. As shown in Fig. 3a, MMP-3 and MMP-13 protein expression were upregulated, while Collagen II and Sox9 protein expression were downregulated in IL-1β-treated cells; in cells treated with both IL-1β and EPZ, the IL-1β-mediated responses were attenuated. The ability of EPZ to affect early chondrogenesis by primary culture human chondrocytes stimulated with IL-1β for 5 and 7 days was determined by using in vitro high-density micromass cultures. Figure 3c, d also shows that IL-1β reduced the alcian blue incorporation, an effect counteracted by the presence of EPZ.

Fig. 3
figure 3

Inhibition of PRMT5 attenuates IL-1β-stimulated chondrocyte catabolism. a Representative western blots showing the expression levels of MMP-3, MMP-13, Sox9, and Collagen II in IL-1β-stimulated human chondrocytes in response to EPZ. b Histogram showing the relative protein expression levels of MMP-3, MMP-13, Sox9, and Collagen II in human chondrocytes. c Alcian blue staining of micromass cultures incubated in the absence of IL-1β, with or without EPZ. d Alcian blue-stained cultures were extracted using 6 M guanidine hydrochloride; the absorbance of the supernatant was measured at 600 nm. Data of independent experiments (n = 3) were presented as mean ± SD and analyzed using the one-way analysis of variance with the SNK post hoc test. *P < 0.05 vs. the IL-1β group. #P < 0.05 vs. the con group

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PRMT5 inhibition confers protection against experimental OA

The effect of PRMT5 inhibition on experimental OA pathogenesis was assessed in a DMM mouse model. DMM results in cartilage erosion, osteophyte formation, and subchondral bone plate thickening [32, 33]; therefore, it serves as a model of OA. Figure 4a shows that EPZ significantly inhibited cartilage destruction in DMM mice; it also reduced the DMM-induced upregulation of MMP-3, MMP-13, and PRMT5 expression, whereas the downregulation of p-p38 and p-p65 expression were observed in the DMM+EPZ group, implying that EPZ can neutralize the activation of the NF-κB and MAPK pathways induced by DMM (Fig. 4c). The Osteoarthritis Research Society International score indicated a protective effect of EPZ on the articular cartilage (Fig. 4a–c). Dramatic changes in total subchondral bone tissue were revealed by μCT, with 47.5% and 36.2% reductions in bone volume/tissue volume and trabecular thickness, respectively, in DMM mice compared to sham-operated mice. Furthermore, trabecular separation increased by 16.8% in DMM mice, whereas EPZ attenuated tibial subchondral bone loss, compared to vehicle-treated DMM mice (Fig. 5).

Fig. 4
figure 4

EPZ reduces the progression of experimental OA. a Hematoxylin and eosin and safranin O-fast green staining of the coronal sections from the knee joint cartilage of sham, DMM, and DMM+EPZ mice. Scale bar = 100 μm. b Histopathological examination using the Osteoarthritis Research Society International criteria to assess cartilage degeneration. c MMP-3, MMP-13, PRMT5, p-p38, and p-p65 expression, as detected by immunohistochemical staining. Data were presented as mean ± SD from 10 samples. Data were analyzed using the one-way analysis of variance with the SNK post hoc test. *P < 0.05 vs. the DMM group. #P < 0.05 vs. the sham group

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Fig. 5
figure 5

EPZ inhibits DMM-induced subchondral bone loss in mouse tibia. a Three-dimensional images of the knee joints in each group, reconstructed using the built-in μCT software. b Structural parameters of the tibial subchondral bone, analyzed according to trabecular bone volume/tissue volume (BV/TV), trabecular thickness (Tb. Th), and trabecular separation (Tb. Sp). Data are presented as mean ± SD from 10 samples. Data were analyzed using the one-way analysis of variance with the SNK post hoc test. *P < 0.05 vs. the DMM group. #P < 0.05 vs. the sham group

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NF-κB and MAPK mediate PRMT5 activity in chondrocytes

To investigate the mechanism by which PRMT5 damages articular chondrocytes, we examined the activation statuses of the NF-κB and MAPK pathways in chondrocytes that had been stimulated with IL-1β in the presence or absence of EPZ. Figure 6 shows that EPZ inhibited the upregulation of phosphorylated-IκBα, p65, p38, and JNK, which had been induced by IL-1β. Thus, the effects of EPZ on IL-1β-induced PRMT5 included inhibition of the NF-κB and MAPK signaling pathways.

Fig. 6
figure 6

EPZ inhibits IL-1β-induced NF-κB and MAPKs in human chondrocytes. a Human chondrocytes were cultured for 16 h in serum-free medium, pretreated with EPZ (10 μM) for 24 h, then stimulated with IL-1β (10 ng/mL) at the indicated times. GAPDH, p38, JNK, ERK1/2, p-JNK, p-p38, and p-ERK1/2 expression levels were analyzed by western blotting. b Histogram showing the relative protein expression levels of p-JNK, p-p38, and p-ERK1/2 in human chondrocyte. c Chondrocytes were treated as above; the expression levels of GAPDH, p65, IκB, p-IκB, and p-p65 were analyzed by western blotting. d Histogram showing the relative protein expression levels of p-IκB, and p-p65 in human chondrocyte. Data of independent experiments (n = 3) were presented as mean ± SD and analyzed using the one-way analysis of variance with the SNK post hoc test. *P < 0.05 vs. the IL-1β group. #P < 0.05 vs. the con group

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Discussion

There remains no effective treatment for OA, and the mechanisms underlying its pathogenesis are poorly understood [34]. PRMT5 is abundantly expressed in a wide variety of human cells [35], and its expression is associated with the occurrence and progression of various diseases [36]; however, its role in the development and progression of OA has been unclear. Our study showed that PRMT5 contributes to OA pathogenesis in mice by modulating the expression levels of MMP-3 and MMP-13 in chondrocytes; in addition, PRMT5 is upregulated in IL-1β-stimulated chondrocytes of patients with OA. The ability of PRMT5 to increase the levels of catabolic factors suggests that it is a crucial catabolic regulator involved in OA.

Increasing evidences suggest that OA is a disease of the whole joint including the cartilage, synovium, ligaments, bone, and bone marrow. In recent years, the subchondral bone has been considered to be one of the main pathological features of OA [37,38,39]. In OA, there is a significant loss of trabecular bone from the tibial subchondral bone. Together with bone marrow lesions, this bone loss is closely linked to pain and is predictive of the severity of cartilage damage in OA. Osteoclasts play a role in the remodeling of the subchondral bone. In this study, we found that EPZ can inhibit DMM-induced subchondral bone loss. These study results were consistent with a previous study which showed that subchondral bone loss is in the DMM OA model [40]. On the contrary, some studies had found that trabecular bone volume/tissue volume (BV/TV) and tibial thickness increased in the subchondral bone of the DMM model [41, 42]. PRMT5 has been demonstrated to regulate osteoclast differentiation and protect against the bone-related effects of ovariectomy in our previous study [43]. However, this study revealed that EPZ by intra-articular injection could not affect the activation of osteoclast in the subchondral bone (Fig. S1). Evidences suggest that cross-talk between chondrocytes and subchondral bone may be involved in the pathology of OA [44, 45]. Therefore, we conferred that EPZ that mainly affected the metabolism of chondrocytes involved in the development of OA may be plausibility. NF-κB comprises a family of ubiquitously expressed transcription factors involved in immunity, stress responses (including responses to mechanical stress), and inflammatory diseases [46]. Our results indicated that the upregulation of MMP-3 and MMP-13 by IL-1β-induced PRMT5 during cartilage destruction is mediated by NF-κB. However, because the effect was only partially blocked by EPZ, other PRMT5-inducing signaling mechanisms may also be involved.

Ramachandran et al. showed that chondrocytes without PRMT5 were unable to undergo hypertrophic differentiation [47], a process related to articular cartilage degeneration. Dongying Chen et al. demonstrated the important roles of PRMT5 in inflammatory responses, cell proliferation, and migration and invasion of fibroblast-like synoviocytes in rheumatoid arthritis; notably, they showed that these responses are mediated by the NF-κB and AKT pathways [24]. Taken together, these results implicate PRMT5 in synovial lesions of OA. In contrast, Sun and colleagues showed that PRMT5 promotes the expression of Sox9 to maintain type collagen II expression levels in human juvenile costal chondrocytes [48]. The discrepancies among studies may be related to the different cell lines used in the respective experiments.

A limitation of our study was that only one time point was examined in the DMM mouse experiment, which evaluated the effect of PRMT5 on OA progression. In addition, while our results implicate the NF-κB pathway in PRMT5-mediated OA pathology, the specific mechanism linking the molecular events to cartilage damage remains unknown. Future research should involve analysis of multiple time points in animal studies and a larger number of patients in clinical studies to better understand the specific downstream mechanisms of PRMT5 in the development of OA.

Conclusions

Our study identified PRMT5 as a newly described catabolic regulator of OA pathogenesis. Overexpression of PRMT5 upregulated the expression levels of matrix-degrading enzymes in chondrocytes of patients with OA, an effect that could be partially attributed to the activation of the NF-κB and MAPK signaling pathways. Although the specific mechanism is not yet known, our results suggest that PRMT5 should be further explored for the prevention and treatment of OA.

Availability of data and materials

The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.

Abbreviations

DMM:

Destabilized medial meniscus

EPZ:

EPZ015666

IL:

Interleukin

MAPK:

Mitogen-activated protein kinase

MMP:

Matrix metalloproteinase

NF-κB:

Nuclear factor kappa-B

OA:

Osteoarthritis

PRMT5:

Protein arginine N-methyltransferase 5

μCT:

Microcomputed tomography

References

  1. Hunter DJ, Schofield D, Callander E. The individual and socioeconomic impact of osteoarthritis. Nat Rev Rheumatol. 2014;10:437–41.

    PubMed  Google Scholar 

  2. Hunter DJ, Bierma-Zeinstra S. Osteoarthritis. Lancet. 2019;393:1745–59.

    CAS  PubMed  Google Scholar 

  3. Glyn-Jones S, Palmer AJ, Agricola R, Price AJ, Vincent TL, Weinans H, et al. Osteoarthritis. Lancet. 2015;386:376–87.

    CAS  PubMed  Google Scholar 

  4. Blom AB, van Lent PL, Libregts S, Holthuysen AE, van der Kraan PM, van Rooijen N, et al. Crucial role of macrophages in matrix metalloproteinase-mediated cartilage destruction during experimental osteoarthritis: involvement of matrix metalloproteinase 3. Arthritis Rheum. 2007;56:147–57.

    CAS  PubMed  Google Scholar 

  5. Tetlow LC, Adlam DJ, Woolley DE. Matrix metalloproteinase and proinflammatory cytokine production by chondrocytes of human osteoarthritic cartilage: associations with degenerative changes. Arthritis Rheum. 2001;44:585–94.

    CAS  PubMed  Google Scholar 

  6. Li H, Wang D, Yuan Y, Min J. New insights on the MMP-13 regulatory network in the pathogenesis of early osteoarthritis. Arthritis Res Ther. 2017;19:248.

    PubMed  PubMed Central  Google Scholar 

  7. Kobayashi M, Squires GR, Mousa A, Tanzer M, Zukor DJ, Antoniou J, et al. Role of interleukin-1 and tumor necrosis factor alpha in matrix degradation of human osteoarthritic cartilage. Arthritis Rheum. 2005;52:128–35.

    CAS  PubMed  Google Scholar 

  8. Burrage PS, Mix KS, Brinckerhoff CE. Matrix metalloproteinases: role in arthritis. Front Biosci. 2006;11:529–43.

    CAS  PubMed  Google Scholar 

  9. Shanmugam MK, Ahn KS, Lee JH, Kannaiyan R, Mustafa N, Manu KA, et al. Celastrol attenuates the invasion and migration and augments the anticancer effects of bortezomib in a xenograft mouse model of multiple myeloma. Front Pharmacol. 2018;9:365.

    PubMed  PubMed Central  Google Scholar 

  10. Nissinen L, Kahari VM. Matrix metalloproteinases in inflammation. Biochim Biophys Acta. 1840;2014:2571–80.

    Google Scholar 

  11. Liang S, Lv ZT, Zhang JM, Wang YT, Dong YH, Wang ZG, et al. Necrostatin-1 attenuates trauma-induced mouse osteoarthritis and IL-1β induced apoptosis via HMGB1/TLR4/SDF-1 in primary mouse chondrocytes. Front Pharmacol. 2018;9:1378.

    CAS  PubMed  PubMed Central  Google Scholar 

  12. Jansson M, Durant ST, Cho EC, Sheahan S, Edelmann M, Kessler B, et al. Arginine methylation regulates the p53 response. Nat Cell Biol. 2008;10:1431–9.

    CAS  PubMed  Google Scholar 

  13. Krause CD, Yang ZH, Kim YS, Lee JH, Cook JR, Pestka S. Protein arginine methyltransferases: evolution and assessment of their pharmacological and therapeutic potential. Pharmacol Ther. 2007;113:50–87.

    CAS  PubMed  Google Scholar 

  14. Banasavadi-Siddegowda YK, Russell L, Frair E, Karkhanis VA, Relation T, Yoo JY, et al. PRMT5-PTEN molecular pathway regulates senescence and self-renewal of primary glioblastoma neurosphere cells. Oncogene. 2017;36:263–74.

    CAS  PubMed  Google Scholar 

  15. Pasternack DA, Sayegh J, Clarke S, Read LK. Evolutionarily divergent type II protein arginine methyltransferase in Trypanosoma brucei. Eukaryot Cell. 2007;6:1665–81.

    CAS  PubMed  PubMed Central  Google Scholar 

  16. LeBlanc SE, Konda S, Wu Q, Hu YJ, Oslowski CM, Sif S, et al. Protein arginine methyltransferase 5 (Prmt5) promotes gene expression of peroxisome proliferator-activated receptor γ2 (PPARγ2) and its target genes during adipogenesis. Mol Endocrinol. 2012;26:583–97.

    CAS  PubMed  PubMed Central  Google Scholar 

  17. Liu L, Zhao X, Zhao L, Li J, Yang H, Zhu Z, et al. Arginine methylation of SREBP1a via PRMT5 promotes de novo lipogenesis and tumor growth. Cancer Res. 2016;76:1260–72.

    CAS  PubMed  Google Scholar 

  18. Wang Y, Zhu T, Li Q, Liu C, Han F, Chen M, et al. Prmt5 is required for germ cell survival during spermatogenesis in mice. Sci Rep. 2015;5:11031.

    PubMed  PubMed Central  Google Scholar 

  19. Wang Y, Hu W, Yuan Y. Protein arginine methyltransferase 5 (PRMT5) as an anticancer target and its inhibitor discovery. J Med Chem. 2018;61:9429–41.

    CAS  PubMed  Google Scholar 

  20. Yoshimatsu M, Toyokawa G, Hayami S, Unoki M, Tsunoda T, Field HI, et al. Dysregulation of PRMT1 and PRMT6, type I arginine methyltransferases, is involved in various types of human cancers. Int J Cancer. 2011;128:562–73.

    CAS  PubMed  Google Scholar 

  21. Karkhanis V, Hu YJ, Baiocchi RA, Imbalzano AN, Sif S. Versatility of PRMT5-induced methylation in growth control and development. Trends Biochem Sci. 2011;36:633–41.

    CAS  PubMed  PubMed Central  Google Scholar 

  22. Norrie JL, Li Q, Co S, Huang BL, Ding D, Uy JC, et al. PRMT5 is essential for the maintenance of chondrogenic progenitor cells in the limb bud. Development. 2016;143:4608–19.

    CAS  PubMed  PubMed Central  Google Scholar 

  23. Bandyopadhyay S, Harris DP, Adams GN, Lause GE, McHugh A, Tillmaand EG, et al. HOXA9 methylation by PRMT5 is essential for endothelial cell expression of leukocyte adhesion molecules. Mol Cell Biol. 2012;32:1202–13.

    CAS  PubMed  PubMed Central  Google Scholar 

  24. Chen D, Zeng S, Huang M, Xu H, Liang L, Yang X. Role of protein arginine methyltransferase 5 in inflammation and migration of fibroblast-like synoviocytes in rheumatoid arthritis. J Cell Mol Med. 2017;21:781–90.

    CAS  PubMed  Google Scholar 

  25. Tanaka H, Hoshikawa Y, Oh-hara T, Koike S, Naito M, Noda T, et al. PRMT5, a novel TRAIL receptor-binding protein, inhibits TRAIL-induced apoptosis via nuclear factor-kappaB activation. Mol Cancer Res. 2009;7:557–69.

    CAS  PubMed  Google Scholar 

  26. Wei H, Wang B, Miyagi M, She Y, Gopalan B, Huang DB, et al. PRMT5 dimethylates R30 of the p65 subunit to activate NF-κB. Proc Natl Acad Sci U S A. 2013;110:13516–21.

    CAS  PubMed  PubMed Central  Google Scholar 

  27. Gulla A, Hideshima T, Bianchi G, Fulciniti M, Kemal Samur M, Qi J, et al. Protein arginine methyltransferase 5 has prognostic relevance and is a druggable target in multiple myeloma. Leukemia. 2018;32:996–1002.

    CAS  PubMed  Google Scholar 

  28. Harris DP, Chandrasekharan UM, Bandyopadhyay S, Willard B, DiCorleto PE. PRMT5-mediated methylation of NF-κB p65 at Arg174 is required for endothelial CXCL11 gene induction in response to TNF-α and IFN-γ costimulation. PLoS One. 2016;11:e0148905.

    PubMed  PubMed Central  Google Scholar 

  29. Glasson SS, Blanchet TJ, Morris EA. The surgical destabilization of the medial meniscus (DMM) model of osteoarthritis in the 129/SvEv mouse. Osteoarthr Cartil. 2007;15:1061–9.

    CAS  PubMed  Google Scholar 

  30. Glasson SS, Chambers MG, Van Den Berg WB and Little CB. The OARSI histopathology initiative recommendations for histological assessments of osteoarthritis in the mouse. Osteoarthritis Cartilage. 2010;null (undefined):S17–23.

  31. Kim GW, Han MS, Park HR, Lee EJ, Jung YK, Usmani SE, et al. CXC chemokine ligand 12a enhances chondrocyte proliferation and maturation during endochondral bone formation. Osteoarthr Cartil. 2015;23:966–74.

    PubMed  Google Scholar 

  32. Fang H, Huang L, Welch I, Norley C, Holdsworth DW, Beier F, et al. Early changes of articular cartilage and subchondral bone in the DMM mouse model of osteoarthritis. Sci Rep. 2018;8:2855.

    PubMed  PubMed Central  Google Scholar 

  33. Okura T, Matsushita M, Mishima K, Esaki R, Seki T, Ishiguro N, et al. Activated FGFR3 prevents subchondral bone sclerosis during the development of osteoarthritis in transgenic mice with achondroplasia. J Orthop Res. 2018;36:300–8.

    CAS  PubMed  Google Scholar 

  34. Kloppenburg M, Berenbaum F. Osteoarthritis year in review 2019: epidemiology and therapy. Osteoarthr Cartil. 2020;28:242–8.

  35. Onikubo T, Nicklay JJ, Xing L, Warren C, Anson B, Wang WL, et al. Developmentally regulated post-translational modification of nucleoplasmin controls histone sequestration and deposition. Cell Rep. 2015;10:1735–48.

    CAS  PubMed  PubMed Central  Google Scholar 

  36. Blanc RS, Richard S. Arginine methylation: the coming of age. Mol Cell. 2017;65:8–24.

    CAS  PubMed  Google Scholar 

  37. Inhibition of SDF-1α/CXCR4 signalling in subchondral bone attenuates post-traumatic osteoarthritis. Int J Mol Sci. 2016;17:943.

  38. Chen Y, Zhang D, Ho KW, Lin S, Suen WC, Zhang H, et al. GPR120 is an important inflammatory regulator in the development of osteoarthritis. Arthritis Res Ther. 2018;20:163.

    PubMed  PubMed Central  Google Scholar 

  39. Findlay DM, Kuliwaba JS. Bone-cartilage crosstalk: a conversation for understanding osteoarthritis. Bone Res. 2016;4:16028.

    CAS  PubMed  PubMed Central  Google Scholar 

  40. Pang C, Wen L, Qin H, Zhu B, Lu X, Luo S. Sotrastaurin, a PKC inhibitor, attenuates RANKL-induced bone resorption and attenuates osteochondral pathologies associated with the development of OA. J Cell Mol Med. 2020;24:8452–65.

    CAS  PubMed  PubMed Central  Google Scholar 

  41. Wang TR, Wang HD, Chen W, Yu TB, Qin Y, Zhang YZ. Proximal fibular osteotomy alleviates medial compartment knee osteoarthritis in a mouse model. Int Orthop. 2020;44:1107–13.

    PubMed  Google Scholar 

  42. Liu B, Ji C, Shao Y, Liang T, He J, Jiang H, et al. Etoricoxib decreases subchondral bone mass and attenuates biomechanical properties at the early stage of osteoarthritis in a mouse model. Biomed Pharmacother. 2020;127:110144.

    CAS  PubMed  Google Scholar 

  43. Dong Y, Song C, Wang Y, Lei Z, Xu F, Guan H, et al. Inhibition of PRMT5 suppresses osteoclast differentiation and partially protects against ovariectomy-induced bone loss through downregulation of CXCL10 and RSAD2. Cell Signal. 2017;34:55–65.

    CAS  PubMed  Google Scholar 

  44. Maas O, Joseph GB, Sommer G, Wild D, Kretzschmar M. Association between cartilage degeneration and subchondral bone remodeling in patients with knee osteoarthritis comparing MRI and (99m) Tc-DPD-SPECT/CT. Osteoarthr Cartil. 2015;23:1713–20.

    CAS  PubMed  Google Scholar 

  45. Ni Z, Zhou S, Li S, Kuang L, Chen H, Luo X, et al. Exosomes: roles and therapeutic potential in osteoarthritis. Bone Res. 2020;8:25.

    CAS  PubMed  PubMed Central  Google Scholar 

  46. Rigoglou S, Papavassiliou AG. The NF-κB signalling pathway in osteoarthritis. Int J Biochem Cell Biol. 2013;45:2580–4.

    CAS  PubMed  Google Scholar 

  47. Ramachandran J, Liu Z, Gray RS, Vokes SA. PRMT5 is necessary to form distinct cartilage identities in the knee and long bone. Dev Biol. 2019;456:154–63.

    CAS  PubMed  Google Scholar 

  48. Sun M, Hussain S, Hu Y, Yan J, Min Z, Lan X, et al. Maintenance of SOX9 stability and ECM homeostasis by selenium-sensitive PRMT5 in cartilage. Osteoarthr Cartil. 2019;27:932–44.

    CAS  PubMed  Google Scholar 

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Acknowledgements

The authors would like to thank all OA and osteosarcoma patients for their participation in the study.

Funding

This work was supported by the China Postdoctoral Fund Project (2018 M632780), the Ministry of Science and Technology National Key Research and Development Program (122300411149), the Natural Science Foundation of Henan Province (182300410349), and the Joint Construction Project of Henan Provincial Health Committee and Ministry of Health (201701017).

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Authors and Affiliations

  1. Department of Orthopedics, Henan Provincial People’s Hospital, Zhengzhou University People’s Hospital, Henan University People’s Hospital, No.7, Weiwu Road, Zhengzhou, 450003, Henan Province, China

    Yonghui Dong, Yongguang Yang, Jincheng Huang, Zhipeng Dai, Wendi Zheng, Zhen Li, Zheng Yao, Hongjun Zhang & Jia Zheng

  2. Department of pathophysiology, School of Basic Medical Sciences, Zhengzhou University, Zhengzhou, 450001, China

    Ping Wang

  3. Department of Molecular Pathology, The Affiliated Cancer Hospital of Zhengzhou University, Henan Cancer Hospital, Zhengzhou, 450008, China

    Ping Wang

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  1. Yonghui Dong
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  2. Ping Wang
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  9. Hongjun Zhang
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  10. Jia Zheng
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Contributions

JZ and YD designed the experiments and revised the manuscript. YD and PW conducted the experiments and prepared the manuscript. YY, JH, ZD, and WZ analyzed the data. CT, WP, and KL contributed reagents and materials. YJ and HZ assisted with the manuscript revision. All authors have read and approved the final manuscript.

Corresponding author

Correspondence to Jia Zheng.

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Ethics approval and consent to participate

The animal study in this research was approved by the Institutional Animal Care and Use Committee (IACUC) at the People’s Hospital of Zhengzhou University (approval no. 2018526). The clinical specimen study was approved by the People’s Hospital of Zhengzhou University Clinical Research Ethics Committee (approval no. 2017237), and informed consent was obtained from each donor.

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Dong, Y., Wang, P., Yang, Y. et al. PRMT5 inhibition attenuates cartilage degradation by reducing MAPK and NF-κB signaling. Arthritis Res Ther 22, 201 (2020). https://doi.org/10.1186/s13075-020-02304-x

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Keywords

Arthritis Research & Therapy

ISSN: 1478-6362

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