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. 2017 Jun 29;16(3):2740–2746. doi: 10.3892/mmr.2017.6886

Hypertrophic differentiation of mesenchymal stem cells is suppressed by xanthotoxin via the p38-MAPK/HDAC4 pathway

Zhen Cao 1,2, Yun Bai 2, Chuan Liu 2, Ce Dou 2, Jianmei Li 2, Junyu Xiang 2, Chunrong Zhao 2, Zhao Xie 3, Qiang Xiang 4, Shiwu Dong 2,✉
PMCID: PMC5548016  PMID: 28677757

Abstract

Chondrocyte hypertrophy is a physiological process in endochondral ossification. However, the hypertrophic-like alterations of chondrocytes at the articular surface may result in osteoarthritis (OA). In addition, the generation of fibrocartilage with a decreased biological function in tissue engineered cartilage, has been attributed to chondrocyte hypertrophy. Therefore, suppressing chondrocyte hypertrophy in OA and the associated regeneration of non-active cartilage is of primary concern. The present study examined the effects of xanthotoxin (XAT), which is classified as a furanocoumarin, on chondrocyte hypertrophic differentiation of mesenchymal stem cells. Following XAT treatment, the expression levels of genes associated with chondrocyte hypertrophy were detected via immunohistochemistry, western blotting and reverse transcription-quantitative polymerase chain reaction. The results revealed that XAT inhibited the expression of various chondrocyte hypertrophic markers, including runt related transcription factor 2 (Runx2), matrix metalloproteinase 13 and collagen type X α1 chain. Further exploration indicated that XAT reduced the activation of p38-mitogen activated protein kinase and then increased the expression of histone deacetylase 4 to suppress Runx2. The findings indicated that XAT maintained the chondrocyte phenotype in regenerated cartilage and therefore may exhibit promise as a potential drug for the treatment of OA in the future.

Keywords: xanthotoxin, mesenchymal stem cell, chondrocyte hypertrophy, MAPK, HDAC4

Introduction

Chondrocyte hypertrophic differentiation is a physiological stage in endochondral ossification which starts from the condensation of mesenchymal stem cells (MSCs) (1). Then MSCs which are located within the centre of condensation differentiate to chondrocytes (2). After proliferation, chondrocytes present hypertrophic morphology and secrete metal matrix proteinase to facilitate angiopoiesis and the formation of bone collar (3). However, the pathogenesis of osteoarthritis (OA) is that hyaline cartilages situated in the surface of osteoarticular manifest unbalanced homeostasis and chondrocytes differentiate into hypertrophy (4,5). Additionally, utilizing tissue engineering to repair cartilage defects, the regenerated cartilages are fibrocartilages and the chondrocytes from MSCs express hypertrophic marker protein (6,7). Thus it can be seen that inhibition of pathological chondrocyte hypertrophy is a very important proposition.

Xanthotoxin (XAT) is mainly isolated in plants such as Umbelliferae and Rutaceae which are used for the treatment of vitiligo, psoriasis and other skin diseases (8,9). Besides, XAT can also induce apoptosis of tumor cells (10,11). It was demonstrated that XAT had anticonvulsant pharmacological effects in the maximal electroshock-induced seizure test (12). However, the effect of XAT on chondrocyte differentiation remains unclear. Therefore, the purpose of this study is to investigate the effect of XAT on chondrocyte hypertrophy of MSCs.

Here, we set out to explore whether XAT could inhibit hypertrophic differentiation of MSCs. Furthermore, we also screened the upstream transcription factors of Runx2, a marker of chondrocyte hypertrophy, to find the molecular mechanism involved in the effect of XAT on chondrocyte hypertrophy.

Materials and methods

Reagents and cell culture

XAT (catalog no. M3501) was purchased from Sigma (St. Louis, MO, USA) which was dissolved in DMSO. Besides, the experimental concentration of DMSO is 0.1% and the control groups were given a DMSO vehicle treatment. C3H10T1/2 mesenchymal stem cells were purchased from the American Type Culture Collection (ATCC; Manassas, VA, USA). The cells were cultured in DMEM-F12 containing 10% fetal bovine serum (FBS) (both from Hyclone, Logan, UT, USA) and 1% penicillin-streptomycin solution (Beyotime, Shanghai, China) at 37°C with 5% CO2. The culture medium was replaced every 2–3 d until the cells reached 90% confluence. Cells were passaged by 0.25% trypsin (Hyclone) for 2 min at room temperature. The second generation cells were used for the following experiments.

In vitro cell proliferation assay

C3H10T1/2 cells were seeded (2×103/well) into 96-well plates (Corning, Corning, NY, USA) in triplicates and allowed to adhere overnight. On the following day, the medium was replaced by fresh medium with different concentrations of XAT (10, 50, 100, 150, and 250 nM). Cultures were incubated for 24 and 72 h. Then, 10 µl Cell Counting Kit-8 (CCK-8; Dojindo Laboratories, Japan) reagents were added to each well and incubated for an additional 4 h. The absorbance was read at the wavelength of 450 nm in an automated plate reader. Wells containing the CCK-8 reagents without cells were used as the blank control. Cell proliferation was assessed by the absorbance values according to the manufacturer's protocol.

Apoptosis assay

MSCs were seeded (5×105/well) into 6-well plates. XAT (50, 100, 150, 200, 250 nM) induced apoptosis of MSCs was detected by flow cytometry using Annexin V-FITC Apoptosis Detection kit (KGA; KeyGEN Biotechnology) according to the manufacturer's instructions. The apoptosis rate was assayed by using FACSCalibur flow cytometry (Becton Dickinson and Beckman-Coulter, San Jose, CA, USA) at 488 nm.

Chondrogenic differentiation assay and hypertrophic differentiation assay

C3H10T1/2 cells were trypsinized by 0.25% trypsin and modulated at a density of 105 cells/ml. Two millilitres of the suspension was placed into the center of each well on a 6-well plate (Corning). After incubation for 24 h at 37°C and 5% CO2, the medium was replaced by 2 ml chondrogenic differentiation medium (Hyclone). The chondrogenic differentiation medium composed of dexamethasone (100 nmol/l), ascorbate (50 µg/ml), ITS supplement, proline (40 µg/ml) and TGF-β3 (10 ng/ml) was replaced every 3 days.

C3H10T1/2 cells were treated by chondrogenic differentiation medium as previously described for 14 days. Then the cells were inducted by hypertrophic differentiation medium composed of dexamethasone (1 nmol/l), ascorbate (50 µg/ml), ITS supplement, proline (40 µg/ml) and triiodothyronine (T3, 100 ng/ml) for another 14 days. Each medium was replaced every 3 days.

Quantitative RT-PCR analysis

Total RNA was isolated using TRIzol reagent (Life Technologies, Carlsbad, NY, USA). Single-stranded cDNA was prepared from 1 µg of total RNA using reverse transcriptase with oligo-dT primer according the manufacturer's instructions (Takara, Liaoning, Dalian, China). Two microlitres of each cDNA was subjected to PCR amplification using specific primers with detailed information in Table I. The cycling conditions were set as 95°C for 30 sec, 40 cycles of 95°C for 5 sec, and 60°C for 30 sec (13). The relative mRNA level was calculated by the normalization to that of GAPDH.

Table I.

Primer sequences for qPCR.

Genes Forward (5′-3′) Reverse (5′-3′) Tm (°C)
HDAC4 CACTCCTCTACGGCACAAATCC CCAACACCACCACAAGGAAGC 60
Sox9 CCCAGCGAACGCACATCA TGGTCAGCGTAGTCGTATT 61
Col2a1 TGGTGGAGCAGCAAGAGC TGGACAGTAGACGGAGGAAA 60
GAPDH GTTGTCTCCTGCGACTTCA GGTGGTCCAGGGTTTCTTA 62
Col10a1 CTTTCTGGGATGCCGCTTGT GGGTCGTAATGCTGCTGCCTA 61
Runx2 CCAACTTCCTGTGCTCCGTG ATAACAGCGGAGGCATTTCG 63
Mmp13 TTGATGCCATTACCAGTCTCCG CACGGGATGGATGTTCATATGC 61
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Western blot analysis

The cells were extracted with lysis buffer containing 50 mM Tris (pH 7.6), 150 mM NaCl, 1% Triton X-100, 1% deoxycholate, 0.1% SDS, 1 mM PMSF and 0.2% Aprotinin (Beyotime). After we measured the protein concentration, the equal protein samples were mixed with 5X sample buffer (Beyotime) and boiled. The proteins (30 µg) were resolved by 10% SDS-PAGE gel and transferred on PVDF membrane (Millipore, Hong Kong, China) by using the semi-dry transfer method. After blocking in 10% nonfat dried milk in TBST for 2 h, the blots were incubated with primary antibodies including HDAC4 (rabbit polyclonal 1:500, ab12172), p38 (rabbit polyclonal 1:500, ab27986), Runx2 (rabbit polyclonal 1:500, ab23981), Col10a1 (rabbit polyclonal 1:500, ab58632) (all from Abcam), p-p38 (rabbit polyclonal 1:500, bs-50486R), Mmp13 (rabbit polyclonal 1:500, bs-0575R) (both from Bioss) and GAPDH (rabbit polyclonal 1:1,000, ab37168; Abcam) at 4°C overnight. After washing by TBST, the blots were incubated with a horseradish peroxidase-conjugated secondary antibody (diluted 1:2,000, sc-2374; Santa Cruz Biotechnology) at room temperature for 1 h. Blots against GAPDH served as loading control.

Glycosaminoglycan (GAG) synthesis analysis by alcian blue staining

To demonstrate the deposition of cartilage matrix proteoglycans, representative cultures were collected at day 28, Then sulfated cartilage glycosaminoglycans (GAGs) were measured by alcian blue (ScienCell) staining. The cells were fixed in 4% paraformaldehyde for 15 min and incubated in 3% acetic aicd for 3 min. Then the cells were stained with alcian blue for 30 min. The mean density was normalized to total cell number.

Immunohistochemistry

The cells were fixed in 4% paraformaldehyde for 15 min. This was followed by washing in phosphate-buffered saline (PBS) and treated with H2O2 (ZSGB-BIO, Peking, China) for 10 min to inactivate endogenous peroxidase. After treatment with normal goat serum (ZSGB-BIO) at room temperature for 15 min, cells were incubated with primary antibodies including Runx2 (rabbit polyclonal 1:150, ab23981) and Col10a1 (rabbit polyclonal 1:150, ab58632) (both from Abcam) at 4°C overnight. After washing, the cells were incubated with biotinylated goat anti-rabbit (ZSGB-BIO) secondary antibodies for 30 min, followed by washing and incubation with horseradish peroxidase (HRP) (ZSGB-BIO) for 15 min. The area of the immunocomplex was visualized by chromogen 3,3′-diaminobenzidine (DAB) for 5 min. The cells were investigated under the Olympus microscope. Image-Pro Plus 6.0 software was used to analyze the IOD and area to calculate mean density of images.

Statistics

All data are representative of at least three experiments of similar results performed in triplicate unless otherwise indicated. Data are expressed as mean ± SEM. One-way ANOVA followed by Student-Newman-Keuls post hoc tests was used to determine the significance of difference between results, with P<0.05, P<0.01 and P<0.001 being regarded as significant.

Results

Toxicity evaluation of XAT on MSCs

The chemical formula of XAT is shown (Fig. 1A) (14). MSCs were treated with basic medium for 24 h and 72 h with different concentrations of XAT followed by CCK-8 assays (Fig. 1B). The results showed that concentration of XAT higher than 100 nM inhibited proliferation of MSCs (P<0.05). After culturing MSCs with basic medium for 72 h, we also investigated effect of XAT on cell apoptosis by FCM (Fig. 1C). In the plots, X axis represented Annexin V-FITC and Y axis represented Propidium iodide. The results revealed that XAT concentration above 100 nM affected early cell apoptosis and above 150 nM promoted late cell apoptosis (P<0.05, Fig. 1D and E). Therefore, the safe concentration of XAT used in following experiments was 100 nM.

Figure 1.

Figure 1.

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High concentration of XAT inhibited MSCs proliferation and induced early and late stage cell apoptosis of MSCs. (A) Chemical formula of XTA. (B) CCK-8 analysis of cell viability of MSCs treated with different concentrations of XAT for 24 and 72 h. (C) FCM analysis of cell apoptosis rate of MSCs treated with basic medium for 72 h with different dosages of XAT treatments. X axis represents Annexin V-FITC and Y axis represents propidium iodide. (D) Quantification analysis of early stage cell apoptosis rate. (E) Quantification analysis of late stage cell apoptosis rate. The data in the figures represent the averages ± SD. Significant differences between the treatment and control groups are indicated in the graph with (*P<0.05) or (**P<0.01) or (***P<0.001).

XAT inhibited expression of chondrocyte hypertrophic marker genes

MSCs were treated with chondrogenic differentiation medium containing TGF-β3 (10 ng/ml) for 14 days. RT-PCR was performed to evaluate the expression of chondrogenic genes. The results showed that expressions of Sox9 and Col2a1 were increased (P<0.01) on day 14 compared with day 0 (Fig. 2A). Then the cells were induced by hypertrophic medium containing T3 (5 ng/ml) for another 14 days. Results of RT-PCR revealed that hypertrophic markers including Runx2 and Col10a1 were increased (P<0.01) on day 28 compared with day 14 (Fig. 2B). According to this in vitro culture system, we further research the effect of XAT on hypertrophic differentiation of MSCs. After treated with chondrogenic differentiation medium for 14 days without XAT, the cells were induced by hypertrophic medium with DMSO or with XAT (100 nM) for another 7 and 14 days. From the alcian blue stain, we found that the groups treated with XAT had higher (P<0.05) intensity than control groups. In addition, the intensity at the concentration of 100 nM was higher (P<0.05) than 50 nM (Fig. 2C and D). Besides, after treatment with XAT, expressions of Col10a1, Runx2 and Mmp13 on mRNA level were decreased (P<0.05) on day 17, 21 and 28 (Fig. 2E). Results of western blotting revealed that hypertrophic markers including Col10a1, Runx2 and Mmp13 were decreased (P<0.05) in cells treated with XAT on day 21 and 28 (Fig. 3A and B). We also performed immunohistochemistry to test the effect of XAT on expression of hypertrophic marker genes. The results showed that the mean density of Col10a1 and Runx2 in groups treated with XAT on day 28 (Fig. 3C and D) were lower (P<0.05) than those in groups without XAT. Taken together, these results demonstrated that chondrocyte hypertrophic differentiation of MSCs was inhibited by XAT at the concentration of 100 nM.

Figure 2.

Figure 2.

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Specific genes expression change during chondrogenic and hypertrophic differentiation. MSCs were induced by chondrogenic medium for 14 days and then treated with hypertrophic medium for another 14 days. (A) Relative mRNA expression levels of Sox9 and Col2a1 from MSCs in different groups (day 0 and 14). (B) Relative mRNA expression levels of Runx2 and Col10a1 from MSCs in different groups (day 14 and 28). XAT inhibited degradation of glycosaminoglycan and expressions of chondrocyte hypertrophic marker genes on mRNA level. (C) Representative alcian blue staining images of MSCs in different groups (day 28). (D) Quantification of mean intensity of alcian blue staining. (E) Relative mRNA expression levels of Col10a1, Runx2 and Mmp13 from MSCs in different groups (day 17, 21 and 28). The data in the figures represent the averages ± SD. Significant differences between the treatment and control groups are indicated in the graph with (*P<0.05) or (**P<0.01) or (***P<0.001).

Figure 3.

Figure 3.

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XAT inhibited expressions of chondrocyte hypertrophic marker genes on protein level. MSCs were induced by chondrogenic medium without XAT for 14 days and then treated with hypertrophic medium together with or without XAT for another 3, 7 and 14 days. (A) Representative western blot images of Col10a1, Runx2, Mmp13 and GAPDH from MSCs in different groups (day 21 and 28). (B) Quantification of normalized expression intensity of Col10a1 and Runx2 against GAPDH. (C) Representative immunohistochemical images of Runx2 and Col10a1 from MSCs in different groups (day 28). Scale bar represents 200 µm. (D) Quantification of mean intensity of Runx2 and Col10a1 in (C). The data in the figures represent the averages ± SD. Significant differences between the treatment and control groups are indicated in the graph with (*P<0.05) or (**P<0.01) or (***P<0.001).

XAT suppressed phosphorylation of p38 and promoted HDAC4 expression during chondrocyte hypertrophic differentiation of MSCs

To explore the molecular mechanisms involved in the effect of XAT on of MSCs, qPCR was performed to test the key transcriptional factors related to chondrocyte hypertrophy. Compared with control groups, we found expression of HDAC4 on mRNA level was increased (P<0.01) with XAT on day 21 and 28 (Fig. 4A). From the results of western blotting (Fig. 4B), HDAC4 expression was increased (P<0.05) on day 21 and 28 in the presence of XAT (Fig. 4C). To further illustrate the mechanism of XAT upregulating expression of HDAC4, we next performed western blotting to test the phosphorylation of p38-MAPK (Fig. 4B). The results revealed that, following XAT treatment, phosphorylation proportion of p38 was lower (P<0.05) than control groups on day 21 and 28 (Fig. 4D). Taken together, these results indicated that XAT suppressed phosphorylation of p38 and promoted HDAC4 expression during hypertrophic differentiation of MSCs.

Figure 4.

Figure 4.

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XAT suppressed phosphorylation of p38 and promoted HDAC4 expression during chondrocyte hypertrophic differentiation of MSCs. (A) Relative mRNA expression levels of HDAC4 from MSCs in different groups (day 17, 21 and 28). (B) Representative western blot images of HDAC4, p38, p-p38 and GAPDH from MSCs in different groups (day 21 and 28). (C) Quantification of normalized expression intensity of HDAC4 against GAPDH. (D) Quantification of normalized expression intensity of p38 against p-p38. (E) Schematic diagram of XAT function in chondrocyte hypertrophy. XAT inhibited phosphorylation of p38 and then promoted expression of HDAC4, ultimately suppressed expression of hypertrophic differentiation gene. The data in the figures represent the averages ± SD. Significant differences between the treatment and control groups are indicated in the graph with (*P<0.05) or (**P<0.01) or (***P<0.001).

Discussion

XAT also called Methoxsalen, has various functions, such as anti-inflammatory, analgesic and anti-oxidation (15–17). It is well established that chondrocyte hypertrophy is closely related to inflammation in osteoarticular (18). Based on the characteristics of XAT, we hypothesized that XAT might suppress chondrocyte hypertrophic differentiation of MSCs. A study has found XAT is a new class of anti-glioma drug via evaluating the effect of XAT in MDA-MB-231, CT-26 and SCC-3 cell lines (19). Besides, our group also confirmed that XAT prevents bone loss by inhibiting RANKL-induced osteoclastogenesis (20).

This is the only study to our knowledge to research the role of XAT on chondrocytes. In this study, we provide evidence that XAT could decrease glycosaminoglycan degradation and suppress expressions of chondrocyte hypertrophic genes including Runx2, Mmp13 and Col10a1. Then we draw a conclusion that XAT suppresses chondrocyte hypertrophic differentiation of MSCs. The transcription factor Runx2 is crucial for regulating chondrocyte hypertrophy (21,22). Overexpression of Runx2 in all chondrocytes resulted in premature chondrocyte hypertrophy (23). We screened several upstream genes of Runx2 to explore the mechanism such as Bapx1, Hoxa2 and HDAC4 through RT-PCR. A recent study showed that Sox9 directly promoted Bapx1 gene expression to repress Runx2 in chondrocytes (24). Besides, Hoxa2 restricted the chondrogenic domain and inhibited bone formation through suppressed Runx2 expression (25). Studies have found HDAC4, a member of the histone deacetylases, interacts with RUNX2 and decreases RUNX2 binding to DNA. Deletion of HDAC4 greatly promoted chondrocyte hypertrophy while forced expression of HDAC4 in chondrocytes suppressed hypertrophy (2,26). It has been confirmed that HDAC4, which was expressed in prehypertrophic chondrocytes, regulated chondrocyte hypertrophy by interacting with and inhibiting the activity of Runx2 (27). Besides, a study revealed that HDAC4 inhibited Runx2 promoter activity in a dosage-dependent manner (28). Therefore, Bapx1, Hoxa2 and HDAC4 might prevent hypertrophy of chondrocytes through reducing RUNX2 activity. Following XAT treatment, Bapx1 and Hoxa2 expression on mRNA level was not changed (data not shown) while HDAC4 expression was increased on day 21 and 28. The protein level was consistent with RT-PCR. Jun N-terminal kinase (JNK) and p38 mitogen-activated protein kinase (MAPK) signaling is associated with cancers and innate immunity. Inhibition of the p38-MAPK significantly reduced the proliferation and invasion of pancreatic cancer cells under high-glucose conditions (29). Besides, it has been confirmed that neospora caninum increased p38 phosphorylation to downregulate the host's innate immune responses (30). A recent study showed that p38 promotes HDAC4 degradation by increasing caspase-mediated cleavage (31). Our results showed XAT could increase phosphorylation of p38 in MSCs. So we figured out that XAT inhibited chondrocyte hypertrophy through down-regulating p38-MAPK signaling pathway, then reducing degradation of HDAC4 (Fig. 4E).

In OA, chondrocytes exhibit hypertrophic morphology and the homeostasis of chondrocyte is broken down. Hhpertrophic chondrocytes express crucial transcription factor Runx2 and secrete Mmp13, which leads to degradation of extracellular matrix (32). Then the function of articular cartilage is severely impaired. Moreover, regenerated cartilage which is constructed by tissue engineering always presents fibrocartilage but hyaline cartilage. Chondrocyte hypertrophic differentiation is the root to cause above phenomenon (33). Hence, inhibition of chondrocyte hypertrophy is the key point to treat arthritis and maintain the function of regenerated cartilage.

XAT, from the common spices, could suppress expressions of chondrocyte hypertrophic genes by inactivating p38-MAPK/HDAC4 signaling pathway. The above data indicate that XAT can be used as a potential drug for the treatment of arthritis and also for maintaining the homeostasis of regenerated cartilage in construction of tissue engineered cartilage.

Acknowledgements

This work was funded by grants from the Nature Science Foundation of China (no. 81571893 and 81271980), the National High-Tech R&D Program of China (863 Program, 2015AA020315) and the Key Project of Logistics Research Plan of PLA (BWS13C014).

References

  • 1.Hinton RJ, Jing Y, Jing J, Feng JQ. Roles of chondrocytes in endochondral bone formation and fracture repair. J Dent Res. 2017;96:23–30. doi: 10.1177/0022034516668321. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 2.Long F, Ornitz DM. Development of the endochondral skeleton. Cold Spring Harb Perspect Biol. 2013;5:a008334. doi: 10.1101/cshperspect.a008334. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 3.Cancedda R, Castagnola P, Cancedda FD, Dozin B, Quarto R. Developmental control of chondrogenesis and osteogenesis. Int J Dev Biol. 2000;44:707–714. [PubMed] [Google Scholar]
  • 4.Glyn-Jones S, Palmer AJ, Agricola R, Price AJ, Vincent TL, Weinans H, Carr AJ. Osteoarthritis. Lancet. 2015;386:376–387. doi: 10.1016/S0140-6736(14)60802-3. [DOI] [PubMed] [Google Scholar]
  • 5.Bianchi A, Guibert M, Cailotto F, Gasser A, Presle N, Mainard D, Netter P, Kempf H, Jouzeau JY, Reboul P. Fibroblast growth factor 23 drives MMP13 expression in human osteoarthritic chondrocytes in a Klotho-independent manner. Osteoarthritis Cartilage. 2016;24:1961–1969. doi: 10.1016/j.joca.2016.06.003. [DOI] [PubMed] [Google Scholar]
  • 6.Wang T, Lai JH, Yang F. Effects of hydrogel stiffness and extracellular compositions on modulating cartilage regeneration by mixed populations of stem cells and chondrocytes in vivo. Tissue Eng Part A. 2016;22:1348–1356. doi: 10.1089/ten.tea.2016.0306. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7.Di Luca A, Szlazak K, Lorenzo-Moldero I, Ghebes CA, Lepedda A, Swieszkowski W, Van Blitterswijk C, Moroni L. Influencing chondrogenic differentiation of human mesenchymal stromal cells in scaffolds displaying a structural gradient in pore size. Acta Biomater. 2016;36:210–219. doi: 10.1016/j.actbio.2016.03.014. [DOI] [PubMed] [Google Scholar]
  • 8.Garg BJ, Garg NK, Beg S, Singh B, Katare OP. Nanosized ethosomes-based hydrogel formulations of methoxsalen for enhanced topical delivery against vitiligo: Formulation optimization, in vitro evaluation and preclinical assessment. J Drug Target. 2016;24:233–246. doi: 10.3109/1061186X.2015.1070855. [DOI] [PubMed] [Google Scholar]
  • 9.Archier E, Devaux S, Castela E, Gallini A, Aubin F, Le Maître M, Aractingi S, Bachelez H, Cribier B, Joly P, et al. Carcinogenic risks of psoralen UV-A therapy and narrowband UV-B therapy in chronic plaque psoriasis: A systematic literature review. J Eur Acad Dermatol Venereol. 2012;26:S22–S31. doi: 10.1111/j.1468-3083.2012.04521.x. (Suppl 3) [DOI] [PubMed] [Google Scholar]
  • 10.Yang H, Xiong J, Luo W, Yang J, Xi T. 8-Methoxypsoralen induces intrinsic apoptosis in HepG2 cells: Involvement of reactive oxygen species generation and ERK1/2 pathway inhibition. Cell Physiol Biochem. 2015;37:361–374. doi: 10.1159/000430360. [DOI] [PubMed] [Google Scholar]
  • 11.Panno ML, Giordano F, Palma MG, Bartella V, Rago V, Maggiolini M, Sisci D, Lanzino M, De Amicis F, Andò S. Evidence that bergapten, independently of its photoactivation, enhances p53 gene expression and induces apoptosis in human breast cancer cells. Curr Cancer Drug Targets. 2009;9:469–481. doi: 10.2174/156800909788486786. [DOI] [PubMed] [Google Scholar]
  • 12.Zagaja M, Andres-Mach M, Patrzylas P, Pyrka D, Szpringer M, Florek-Łuszczki M, Żółkowska D, Skalicka-Woźniak K, Łuszczki JJ. Influence of xanthotoxin (8-methoxypsoralen) on the anticonvulsant activity of various novel antiepileptic drugs against maximal electroshock-induced seizures in mice. Fitoterapia. 2016;115:86–91. doi: 10.1016/j.fitote.2016.09.020. [DOI] [PubMed] [Google Scholar]
  • 13.Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2(−Delta Delta C(T)) method. Methods. 2001;25:402–408. doi: 10.1006/meth.2001.1262. [DOI] [PubMed] [Google Scholar]
  • 14.Tian W, Cai J, Xu Y, Luo X, Zhang J, Zhang Z, Zhang Q, Wang X, Hu L, Lin G. Determination of xanthotoxin using a liquid chromatography-mass spectrometry and its application to pharmacokinetics and tissue distribution model in rat. Int J Clin Exp Med. 2015;8:15164–15172. [PMC free article] [PubMed] [Google Scholar]
  • 15.Wolnicka-Glubisz A, Sarna T, Klosner G, Knobler R, Trautinger F. UVA activated 8-MOP and chlorpromazine inhibit release of TNF-alpha by post-transcriptional regulation. Photochem Photobiol Sci. 2004;3:334–336. doi: 10.1039/B302621C. [DOI] [PubMed] [Google Scholar]
  • 16.Chen YF, Tsai HY, Wu TS. Anti-inflammatory and analgesic activities from roots of Angelica pubescens. Planta Med. 1995;61:2–8. doi: 10.1055/s-2006-957987. [DOI] [PubMed] [Google Scholar]
  • 17.Ng TB, Liu F, Wang ZT. Antioxidative activity of natural products from plants. Life Sci. 2000;66:709–723. doi: 10.1016/S0024-3205(99)00642-6. [DOI] [PubMed] [Google Scholar]
  • 18.Caron MMJ, Emans PJ, Surtel DA, van der Kraan PM, van Rhijn LW, Welting TJ. BAPX-1/NKX-3.2 acts as a chondrocyte hypertrophy molecular switch in osteoarthritis. Arthritis Rheumatol. 2015;67:2944–2956. doi: 10.1002/art.39293. [DOI] [PubMed] [Google Scholar]
  • 19.de Oliveira DM, Lima RM Ferreira, Clarencio J, Velozo Eda S, de Amorim IA, da Andrade Mota TH, Costa SL, Silva FP, El-Bachá Rdos S. The classical photoactivated drug 8-methoxypsoralen and related compounds are effective without UV light irradiation against glioma cells. Neurochem Int. 2016;99:33–41. doi: 10.1016/j.neuint.2016.06.004. [DOI] [PubMed] [Google Scholar]
  • 20.Dou C, Chen Y, Ding N, Li N, Jiang H, Zhao C, Kang F, Cao Z, Quan H, Luo F, et al. Xanthotoxin prevents bone loss in ovariectomized mice through the inhibition of RANKL-induced osteoclastogenesis. Osteoporosis Int. 2016;27:2335–2344. doi: 10.1007/s00198-016-3496-8. [DOI] [PubMed] [Google Scholar]
  • 21.Liu CF, Samsa WE, Zhou G, Lefebvre V. Transcriptional control of chondrocyte specification and differentiation. Semin Cell Dev Biol. 2017;62:34–49. doi: 10.1016/j.semcdb.2016.10.004. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 22.Guo F, Han X, Wu Z, Cheng Z, Hu Q, Zhao Y, Wang Y, Liu C. ATF6a, a Runx2-activable transcription factor, is a new regulator of chondrocyte hypertrophy. J Cell Sci. 2016;129:717–728. doi: 10.1242/jcs.169623. [DOI] [PubMed] [Google Scholar]
  • 23.Takeda S, Bonnamy JP, Owen MJ, Ducy P, Karsenty G. Continuous expression of Cbfa1 in nonhypertrophic chondrocytes uncovers its ability to induce hypertrophic chondrocyte differentiation and partially rescues Cbfa1-deficient mice. Genes Dev. 2001;15:467–481. doi: 10.1101/gad.845101. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Yamashita S, Andoh M, Ueno-Kudoh H, Sato T, Miyaki S, Asahara H. Sox9 directly promotes Bapx1 gene expression to repress Runx2 in chondrocytes. Exp Cell Res. 2009;315:2231–2240. doi: 10.1016/j.yexcr.2009.03.008. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 25.Kanzler B, Kuschert SJ, Liu YH, Mallo M. Hoxa-2 restricts the chondrogenic domain and inhibits bone formation during development of the branchial area. Development. 1998;125:2587–2597. doi: 10.1242/dev.125.14.2587. [DOI] [PubMed] [Google Scholar]
  • 26.Chen W, Sheng P, Huang Z, Meng F, Kang Y, Huang G, Zhang Z, Liao W, Zhang Z. MicroRNA-381 regulates chondrocyte hypertrophy by inhibiting histone deacetylase 4 expression. Int J Mol Sci. 2016;17:E1377. doi: 10.3390/ijms17091377. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 27.Vega RB, Matsuda K, Oh J, Barbosa AC, Yang X, Meadows E, McAnally J, Pomajzl C, Shelton JM, Richardson JA, et al. Histone deacetylase 4 controls chondrocyte hypertrophy during skeletogenesis. Cell. 2004;119:555–566. doi: 10.1016/j.cell.2004.10.024. [DOI] [PubMed] [Google Scholar]
  • 28.Li P, Wei X, Guan Y, Chen Q, Zhao T, Sun C, Wei L. MicroRNA-1 regulates chondrocyte phenotype by repressing histone deacetylase 4 during growth plate development. FASEB J. 2014;28:3930–3941. doi: 10.1096/fj.13-249318. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Wang L, Bai YY, Yang Y, Hu F, Wang Y, Yu Z, Cheng Z, Zhou J. Diabetes mellitus stimulates pancreatic cancer growth and epithelial-mesenchymal transition-mediated metastasis via a p38 MAPK pathway. Oncotarget. 2016;7:38539–38550. doi: 10.18632/oncotarget.9533. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 30.Mota CM, Oliveira AC, Davoli-Ferreira M, Silva MV, Santiago FM, Nadipuram SM, Vashisht AA, Wohlschlegel JA, Bradley PJ, Silva JS, et al. Neospora caninum activates p38 MAPK as an evasion mechanism against innate immunity. Front Microbiol. 2016;7:1456. doi: 10.3389/fmicb.2016.01456. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 31.Zhou JM, Li PC, Chen Q, Wei X, Zhao T, Wang Z, Wei L. Mitogen-activated protein kinase p38 induces HDAC4 degradation in hypertrophic chondrocytes. Biochim Biophys Acta. 2015;1853:370–376. doi: 10.1016/j.bbamcr.2014.11.003. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 32.Kung LH, Zaki S, Ravi V, Rowley L, Smith MM, Bell KM, Bateman JF, Little CB. Utility of circulating serum miRNAs as biomarkers of early cartilage degeneration in animal models of post-traumatic osteoarthritis and inflammatory arthritis. Osteoarthritis Cartilage. 2017;25:426–434. doi: 10.1016/j.joca.2016.09.002. [DOI] [PubMed] [Google Scholar]
  • 33.Doran PM. Cartilage tissue engineering: What have we learned in practice? Methods Mol Biol. 2015;1340:3–21. doi: 10.1007/978-1-4939-2938-2_1. [DOI] [PubMed] [Google Scholar]

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