To investigate the functional effects of resveratrol (RSV) on mesenchymal stem cells (MSCs), we treated MSCs with RSV continuously during ex vivo expansion. MSCs were continuously treated with RSV from passage (P) 0 to P5. A proliferative capacity of RSV-treated MSCs was higher than that of non-treated MSCs and similar with P1-MSCs. Continuous treatment of RSV on MSCs increased the stemness and inhibited the senescence. During chondrogenic differentiation in vitro, RSV-treated MSCs had higher differentiation potential and reduced hypertrophic maturation, which are limitations for hyaline cartilage formation. The histological analysis of micromass demonstrated increased chondrogenic differentiation potential. We further explored the therapeutic effectiveness of this method in a rabbit osteochondral defect model. A rabbit osteochondral defect model was established to investigate the hyaline cartilage regeneration potential of RSV-treated MSCs. Moreover, the cartilage regeneration potential of RSV-treated MSCs was greater than that of untreated MSCs. The expression levels of chondrogenic markers increased and those of hypertrophic markers decreased in RSV-treated MSCs compared with untreated MSCs. Sustained treatment of RSV on MSCs during ex vivo expansion resulted in the maintenance of stemness and enhanced chondrogenic differentiation potential. Consequentially, highly efficient MSCs promoted superior hyaline cartilage regeneration in vivo. This novel treatment method provides a basis for cell-based tissue engineering.
Osteoarthritis (OA) involves cartilage damage, dysfunctional chondrocyte proliferation, and hypertrophic maturation1,2,3,4. Several types of therapies are currently used for cartilage regeneration, including bone marrow-stimulating techniques, mosaicplasty, and cell-based therapies5. Cell-based therapies are increasingly used as a prospective treatment. Autologous chondrocyte implantation is commonly used for cartilage regeneration, requiring the in vitro expansion of autologous chondrocytes6. Nevertheless, these techniques have several shortcomings, such as their complexity, cost, and the loss of cartilage capacity7,8. Therefore, cell-based therapeutic approaches using mesenchymal stem cells (MSCs) have emerged for cartilage regeneration9,10,11.
MSCs have various advantages for clinical applications, such as anti-inflammatory and immunosuppressive effects, high effectiveness, and a lack of severe side effects12. Additionally, MSCs possess a high stemness capacity and thereby have the potential for multipotency, including chondrogenic differentiation. For these reasons, MSCs are a promising cell source for cartilage regeneration13,14,15. However, several factors limit the clinical application of MSCs. For example, hundreds of millions of MSCs are required. MSCs can be isolated from various organs, but the number of isolated cells is insufficient. To obtain sufficient MSCs, long-term in vitro expansion is necessary16; however, acquiring an effective quantity of MSCs with sustained self-renewal and multi-lineage differentiation potential is difficult17,18. Moreover, MSCs tend to become fibro-like tissues after the induction of chondrogenic differentiation19,20, and they exhibit fibro-like tissue regeneration in vivo. Therefore, the identification of new environments for the development of highly efficient MSCs with an enhanced self-renewal capacity and chondrogenic differentiation potential is necessary.
Mohyeldin et al.21 demonstrated that MSCs require physiological oxygen levels of between 2 and 8%. Under hypoxic conditions, the expression levels of hypoxia-inducible factors increase, leading to the upregulation of Oct-4, Sox2, and Nanog, which are critical transcription factor for stemness22. Previous studies have suggested that under hypoxic conditions, MSCs have enhanced proliferative potential and stemness during in vitro cultivation23. In fact, antioxidants, such as resveratrol24, palm vitamin E25, butylated hydroxyanisole26, and butylated hydroxytoluene27, are known to not only suppress reactive oxygen species, but also delay disease progression and influence lipid peroxidation28. Butylated hydroxyanisole and butylated hydroxytoluene are frequently used as additives in the food industry26,29; however, their use is restricted owing to their potential toxicity and carcinogenic effects28. Thus, the discovery of new, safe antioxidants that can overcome the disadvantages of chemical antioxidants is necessary.
The antioxidant resveratrol (RSV; 3,5,4ʹ-hydroxystilbene), a natural compound, is a phytoalexin produced by plants in response to environmental stress30,31,32. RSV has critical roles in the inhibition of oxidative damage33 as well as in cell survival and proliferation34,35,36. Furthermore, RSV is known to enhance activity of sirtuin 1 (SIRT1), an NAD+-dependent lysine deacetylase. During in vitro cultivation, MSCs occasionally become senescent, leading to a loss of stemness. Previously, Yuan et al.35 demonstrated that the knockdown of SIRT1 in early-passage MSCs using shRNA results in a loss of proliferative capacity and promotes cellular senescence. In contrast, the overexpression of SIRT1 in MSCs delays cellular senescence and cells maintain multipotency during long-term in vitro cultivation35. Moreover, RSV enhances the osteogenic and adipogenic differentiation potential of MSCs, but prolonged treatment of MSCs with RSV induces senescence37,38. Other studies have demonstrated that RSV has negative effects on MSCs during adipogenic and osteogenic differentiation39,40. These incompatible results regarding the effects of RSV on senescence and differentiation in MSCs may be explained by dose- or duration-dependent effects34. Hence, a novel RSV treatment method for MSCs is necessary. Additionally, the effect of RSV on chondrogenic differentiation has not been elucidated. In this study, we developed a novel treatment method using RSV that yields consistent results. Moreover, we evaluated the stemness and chondrogenic differentiation potential of MSCs after treatment with RSV. This novel treatment method provides a basis for cell-based tissue engineering.
Increased stemness and decreased senescence of RSV-treated MSCs
During in vitro cultivation, we continuously treated MSCs with RSV from P0 to P5 (P5-RMSC), and other cells were cultured up to P5 without RSV treatment (P5-MSC) (Fig. 1a). To investigate whether RSV treatment increases the self-renewal capacity of MSCs, we evaluated the cell morphology and proliferative potential. P5-RMSCs had a similar morphology to that of P1-MSCs, i.e., cells were small and spindle-shaped. However, P5-MSCs had a large, flat appearance (Fig. 1b). P5-MSCs had a decreased proliferative capacity over time, whereas the P5-RMSCs had a similar proliferative capacity to that of P1-MSCs (Fig. 1c). To determine the effects of RSV on senescence and stemness, we assessed protein expression levels of senescence and stemness markers such as P16, P21, P53 and Nanog, Oct4, Sox2, respectively. In P5-RMSCs, the stemness markers were up-regulated and senescence markers were down-regulated, similar to the expression levels in P1-MSCs, however, the opposite results were obtained for P5-MSCs, which exhibited the upregulation of senescence markers and down-regulation of stemness markers (Fig. 1d, e). Therefore, continuous treatment of RSV on MSCs was able to maintain the stemness and inhibit senescence, suggesting that it is a useful method for the establishment of highly efficient MSCs.
Enhancement of the chondrogenic differentiation potential in RSV-treated MSCs
To evaluate the chondrogenic differentiation potential, we performed micromass culture using P1-MSC, P5-MSC, and P5-RMSC. The mRNA levels of Sox-5, -6, -9, Col2a1, and aggrecan, which are chondrogenic markers, were higher in P5-RMSC than in P5-MSC and were similar to the levels in P1-MSC (Fig. 2a). The protein expression levels of chondrogenic markers were comparable in P1-MSC and P5-RMSC and a quantitative analysis supported this finding (Fig. 2b, c). To further demonstrate the increased chondrogenic differentiation potential of P5-RMSC, we performed SafO and AB staining. The P5-MSC group had a much smaller micromass size than those of the P1-MSC and P5-RMSC groups, which both had higher contents of glycosaminoglycan (GAG) and proteoglycan (PG) (Fig. 3a). We evaluated the expression levels of col2a1 and aggrecan in micromass pellets by immunocytochemistry. P5-RMSC had high expression levels of col2a1 and aggrecan, similar to the expression levels in P1-MSC (Fig. 3b, c). Accordingly, P5-RMSC, which had enhanced stemness, had superior chondrogenic differentiation potential compared to that of P5-MSC.
Inhibition of the hypertrophic maturation of RSV-treated MSCs
During chondrogenic differentiation, hypertrophic maturation inhibits hyaline cartilage regeneration19,41. To determine whether P5-RMSC exhibited inhibited hypertrophic maturation during chondrogenic differentiation in vitro, we evaluated the both mRNA and protein expression levels of hypertrophic markers. P5-RMSC had lower expression levels of hypertrophic markers than those in P5-MSC (Fig. 4a, b). Additionally, an immunocytochemical analysis demonstrated that the expression of col10a1, a key marker of hypertrophic maturation, was significantly decreased in P5-RMSC (Fig. 4c). Consequentially, sustained treatment of MSCs with RSV enhanced the chondrogenic differentiation potential and prevented hypertrophic maturation during in vitro chondrogenic differentiation via improved stemness.
Increased cartilage regeneration potential in vivo
To determine whether continuous treatment of RSV on MSCs could enhance the cartilage regeneration capacity in vivo, we established a rabbit osteochondral defect model (Fig. 5a). At 8 weeks post operation, we observed the gross morphology of regenerated cartilage. In the Hy/RMSC group, the surface of the defect site was almost fully filled with cartilage-like tissue, along with nearby cartilage. The Hy/RMSC group showed transparent cartilage-like tissues, whereas the defect, Hy, and Hy/MSC groups had incomplete cartilage tissue formation (Fig. 5b). These results indicate that the regeneration of intact cartilage surface tissues is possible via continuous treatment of RSV on MSCs.
Histological analysis of regenerated cartilage in the rabbit osteochondral defect model
We observed regenerated cartilage at defect sites by MT and H&E staining. The MT stain showed higher collagen deposition on cartilage surface of the Hy/RMSC group compared to the Hy/MSC group (Fig. 6a). In the H&E stain, the Hy/RMSC group had chondrocyte-like cells with smooth cartilage-like tissues, which were similar in morphology to normal cartilage. However, the defect, Hy, and Hy/MSC groups showed fibrous tissue formation (Fig. 6b). Safranin O/Fast Green staining demonstrated increased GAG formation in the Hy/RMSC group; the Hy/MSC group showed slightly greater synthesis of GAG than those of the other groups (Fig. 6c). Additionally, O’Driscoll histological scoring was performed, and the Hy/MSC group had a slightly higher score than those of the defect or Hy group, and the Hy/RMSC group had a significantly higher score (Fig. 6d). These results demonstrate that the Hy/MSC group had slight differences in cartilage regeneration, but Hy/RMSC group exhibited significant differences in functional cartilage regeneration.
Effects of cartilage regeneration for RSV-treated MSCs based on both chondrogenic and hypertrophic markers
Next, we evaluated the expression of extracellular matrix (ECM) proteins, type II collagen and aggrecan, in regenerated cartilage tissues by immunohistochemistry. The Hy/RMSC group showed higher expression levels of ECM proteins than those of the Hy/MSC group, which exhibited slight expression of these proteins. A quantitative analysis demonstrated that there was significantly higher expression of both type II collagen and aggrecan in the Hy/RMSC group than in other groups (Fig. 7a, b). Moreover, the expression of a hypertrophic marker, type X collagen, was assessed. The Hy/RMSC group showed very low expression of type X collagen, while other groups had high expression levels. A quantitative analysis showed that type X collagen expression was significantly lower in the Hy/RMSC group than in other groups (Fig. 7c). As a result, the continuous treatment of MSCs with RSV resulted in enhanced cartilage regeneration potential and the inhibition of hypertrophic maturation, which limits the use of MSCs for cell therapy19,41.
In the present study, MSCs were continuously treated with RSV from P0 to P5, and the maintenance of their stemness was confirmed. Continuous treatment maintained the activity of sirtuin 1 (SIRT1). P5-RMSC had increased protein levels of stemness markers and decreased levels of senescence markers compared with those in P5-MSC. As shown in our previous study, the maintenance of SIRT1 activity sustains the expression of SOX237; thus, the stemness of MSCs could be maintained over time.
P5-RMSC had similar stemness to that of P1-MSC and improved chondrogenic differentiation potential (Figs. 2 and 3). Additionally, hypertrophic maturation was inhibited in P5-RMSC, resulting in the increased expression of type X collagen (COL10A1), matrix metalloproteinase 13 (MMP13), and alkaline phosphatase (ALP) (Fig. 4)19,41. To confirm the efficiency of the cartilage regenerative potential of P5-RMSC, which had similar stemness to that of P1-MSC, we established an osteochondral defect model in rabbits with a depth of 3 mm and a diameter of 6 mm, a critical size threshold for rabbit models42. This critical size of osteochondral defect sites results in an inability to self-heal. At 8 weeks post operation, P5-RMSC showed smoother and more intact cartilage that was well attached to nearby cartilage compared to other groups (Figs. 5 and 6). P5-RMSC had higher expression of ECM proteins and lower expression of hypertrophic maturation markers (Fig. 7). Therefore, P5-RMSC had increased cartilage regeneration potential with hyaline-like tissue formation in the rabbit osteochondral defect model when compared with P5-MSC. These results demonstrate that our innovative treatment method with RSV promotes the maintenance of stemness in MSCs over time and thus can increase the cartilage regeneration potential (Fig. 8).
During long-term ex vivo expansion, MSCs do not grow infinitely, leading to senescence43. Bonab et al.17 demonstrated that bone marrow-derived MSCs exhibit decreased population doubling and shorter telomere lengths as cells are subcultured. Furthermore, clinical history, age, and genetic makeup determine the length of the expansion period and quality of MSCs44. Thus, retaining MSCs with sustained stemness is essential.
Several studies have demonstrated that long-term exposure to RSV could increase the senescence of MSCs34; during osteogenic differentiation, RSV adversely affects adipogenic differentiation45. For the chondrogenic differentiation of MSCs, previous studies have demonstrated that treatment with RSV during the chondrogenic differentiation period enhances chondrogenic potential and inhibits inflammatory and degradative processes in cartilage via the activation of SIRT146. Additionally, the treatment of chondrocytes with RSV up-regulates SIRT1 expression, but leads to hypertrophic maturation47. Unlike previous studies, our results showed that stemness can be maintained in P5-MSC via continuous treatment with RSV, thus maintaining their chondrogenic differentiation potential. We also confirmed the inhibition of hypertrophic maturation both in vitro and in vivo. For clinical applications, the recommended number of passages for MSCs is 3–548,49. In general, MSCs at passages 1–2 have high multipotency and MSCs at passages 4–5 have low multipotency and a loss of replicative potential50,51. Accordingly, in our study, we continuously treated MSCs with RSV from P0 to P5 to verify the sustained stemness of MSCs at passage 5.
In our in vivo study, the defect group showed slight regeneration of cartilage-like tissues (Fig. 6). Although the osteochondral defect sizes were fixed at 3 mm in depth, during the surgical procedure, the bone marrow concentrates affected the regeneration of cartilage-like tissues in the defect group. In fact, bone marrow concentrates containing a variety of heterogenous cells and a lack of MSCs are known to contribute to fibrocartilage formation, rather than hyaline cartilage52. Thus, the bone marrow concentrates did not affect the cartilage regenerative potential in the Hy/MSC and Hy/RMSC groups. The Hy/RMSC group had hyaline-like cartilage tissue formation (Figs. 6 and 7).
Taken together, the continuous treatment of RSV on MSCs during in vitro cultivation resulted in sustained stemness and chondrogenic differentiation potential, similar to that of P1-MSC, thereby improving hyaline cartilage regeneration (Fig. 8). Therefore, the novel treatment method with RSV could provide a foundation for studies in cell-based tissue engineering with minimal side effects.
Materials and methods
Isolation and identification of MSCs from human bone marrow aspirates
Bone marrow aspirates were acquired from the posterior iliac crest of 10 healthy donors after obtaining approval from the Institutional Review Board of Yonsei University College of Medicine. MSCs were isolated and cultivated as previously described53.
Chemical treatment of MSCs
Resveratrol (RSV; Sigma, St. Louis, MO, USA) was dissolved in ethanol (EtOH) at 1 µM. RSV was continuously applied to MSCs from P0 to P5 (P5-RMSC) and cells were subcultured as previously described54. MSCs were evaluated up to P5 based on previous studies indicating that MSCs at passages 3–5 are optimal for clinical applications48,49.
In vitro chondrogenic differentiation of MSCs
For the chondrogenic differentiation of MSCs, the micromass culture method was used, as previously reported55. Briefly, 10 µl of resuspended cells at a density of 1 × 105 cells per well was added to the center of the wells in 24-well plates. Cells were allowed to attach for 2 h and chondrogenic medium was then added. The chondrogenic medium was replenished every 3 days.
Quantitative real-time PCR (qRT-PCR)
Extraction of total RNA harvested from cells was performed using TRIzol (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s protocols. To synthesize cDNA, the Omniscript Reverse Transcription Kit (Qiagen, Hilden, Germany) was used for the reverse transcription of 2 μg of RNA. To conduct real-time PCR, 2×qPCRBIO SyGreen Mix (PCR Biosystems, London, UK) was used with 80 ng of cDNA. To quantify the relative expression levels of target genes, beta-actin (β-actin) was used as an internal control. Validated primers targeting Sox9 (P232240), IHH (P101104), and ALP (P324388) were used. Other primers were designed, as shown in Table 1, and all primers were purchased from Bioneer (Daejeon, Korea). Real-time PCR was performed using the ABI7900 (Applied Biosystems, Carlsbad, CA, USA) in accordance with a previous report55.
Western blot analysis
Cell pellets were lysed and quantified as previously reported56. The samples (10–30 μg of protein) were separated by 10% sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) (Sigma) and transferred onto polyvinylidene difluoride (PVDF) membranes (Amersham Pharmacia, Escondido, CA, USA). Briefly, after blocking with 5% skim milk, membranes were incubated with primary anti-SOX9 (1:3000, Millipore, Billerica, MA, USA), anti-RUNX2, anti-P16 (1:3000, Abcam, Cambridge, UK), anti-COL2A1, anti-AGGRECAN, anti-OCT4, anti-MMP13, anti-COL1A1, anti-P21, anti-P53 (1:500, Santa Cruz Biotechnology, Santa Cruz, CA, USA), anti-NANOG (1:1000, BD biosciences, San Jose, CA, USA), anti-SOX2 (1:1000, Cell signaling Technology, Inc., Danver MA, USA), anti-HSP90 or anti-β-ACTIN (1:1,000, Santa Cruz Biotechnology) overnight at 4 °C. Then, membranes were incubated with secondary HRP-conjugated antibodies (1:5000, Santa Cruz Biotechnology) for 1 h at room temperature.
Hydrogel precursor preparation
The hydrogel (Hy) was prepared as described previously57,58. In short, the cosolvent consisted of water and dimethylformamide at a ratio of 3:2; it was supplemented with 1-ethyl-3-(3-dimethylaminopropyl)-carbodiimide (EDC) and N-hydroxysuccinimide (NHS), which activates 3-(4-hydroxyphenyl)propionic acid (HPA), and this solution was added to a preheated gelatin solution. After 24 h of reaction at 40 °C, the solution was dialyzed with deionized water, filtered, and lyophilized.
Twenty New Zealand white rabbits (male, 3.5–4 kg; Doo Yeol Biotech, Seocho-gu, Seoul, Korea) were used to establish the osteochondral defect model according to previously methods59. Briefly, full-thickness cylindrical osteochondral defect sites with a diameter of 6 mm (3-mm depth) were formed on the surface of the femoral patellar groove using the osteochondral autotransfer system (OATS; Arthrex, Naples, FL, USA). For each osteochondral defect site, the following treatments were applied: None (defect), hydrogel only (Hy), Hy + P5-MSC (Hy/MSC), and Hy + P5-RMSC (Hy/RMSC). A total of 2 × 106 in vitro cultured MSCs were mixed with the GH polymer (5 wt%) that containing 0.0015 mg/mL of horseradish peroxidase (HRP). The hydrogel formation was occurred when the solution mixed with same volume of GH polymer (5 wt%) that containing 0.005 wt% hydrogen peroxide (H2O2)60. At 8 weeks after the operation, the rabbits were euthanized and defect sites were extracted for the histological analysis. All animal experiments were approved by the Committee on the Ethics of Animal Experiments of Yonsei University College of Medicine (Permit No. 2016-0200).
The samples obtained from osteochondral knee defects and micromass pellets were fixed for 7 days and 24 h in 10% formalin, respectively. After fixation, the specimens were embedded in paraffin and then paraffin sections were deparaffinized, rehydrated, and washed with PBS. The sections were stained with Masson’s trichrome (MT), hematoxylin–eosin (H&E), Safranin O (SafO), and Alcian blue (AB), as previously described59. The stained sections were observed using a VS 120 virtual microscope (Olympus, Tokyo, Japan). A quantitative analysis was performed using ImageJ v.1.48 (Aspire Software International, Leesburg, VA, USA). Moreover, the O’Drsicoll histological scoring system was used for the histological assessment61, and the regenerated cartilage was assessed by three blinded experts.
After washing paraffin sections with PBS, they were incubated in hydrogen peroxidase for 10 min to minimize nonspecific background staining. To detect chondrogenic markers, the sections were incubated with anti-COL2A1, anti-AGGRECAN, and anti-COL10A1 (1:100, Santa Cruz Biotechnology) antibodies at 4 °C for at least 12 h. The attachment of secondary antibodies and fluorescent protein-conjugated secondary antibodies was performed following previously described methods59. Nuclei were stained with 4ʹ,6-diamidino-2-phenylindole (Sigma). An inverted fluorescence microscope (IX-71; Olympus, Tokyo, Japan) was used to acquire images and expression levels were quantified using ImageJ.
Each experiment was performed in triplicate using samples from more than three donors. To detect differences between two groups, t-tests were used. The statistical significance of the differences among three or more groups was evaluated using one-way analysis of variance (ANOVA) with Tukey’s post hoc tests. All results are presented as means and 95% CIs of the values from three different donors per group.
Johnson, K. et al. A stem cell-based approach to cartilage repair. Science 336, 717–721 (2012).
Lawrence, R. C. et al. Estimates of the prevalence of arthritis and other rheumatic conditions in the United States. Part II. Arthritis Rheum. 58, 26–35 (2008).
Ruan, M. Z. et al. Proteoglycan 4 expression protects against the development of osteoarthritis. Sci. Transl. Med. 5, 176ra134 (2013).
Yamashita, A. et al. Generation of scaffoldless hyaline cartilaginous tissue from human iPSCs. Stem Cell Rep. 4, 404–418 (2015).
Madeira, C., Santhagunam, A., Salgueiro, J. B. & Cabral, J. M. Advanced cell therapies for articular cartilage regeneration. Trends Biotechnol. 33, 35–42 (2015).
Narcisi, R. et al. Long-term expansion, enhanced chondrogenic potential, and suppression of endochondral ossification of adult human MSCs via WNT signaling modulation. Stem Cell Rep. 4, 459–472 (2015).
Schulze-Tanzil, G., Mobasheri, A., de Souza, P., John, T. & Shakibaei, M. Loss of chondrogenic potential in dedifferentiated chondrocytes correlates with deficient Shc-Erk interaction and apoptosis. Osteoarthr. Cartil. 12, 448–458 (2004).
Kondo, M., Yamaoka, K. & Tanaka, Y. Acquiring chondrocyte phenotype from human mesenchymal stem cells under inflammatory conditions. Int. J. Mol. Sci. 15, 21270–21285 (2014).
Ahmed, T. A. & Hincke, M. T. Mesenchymal stem cell-based tissue engineering strategies for repair of articular cartilage. Histol. Histopathol. 29, 669–689 (2014).
Barry, F. & Murphy, M. Mesenchymal stem cells in joint disease and repair. Nat. Rev. Rheumatol. 9, 584–594 (2013).
Richardson, S. M. et al. Mesenchymal stem cells in regenerative medicine: opportunities and challenges for articular cartilage and intervertebral disc tissue engineering. J. Cell. Physiol. 222, 23–32 (2010).
Jo, C. H. et al. Intra-articular injection of mesenchymal stem cells for the treatment of osteoarthritis of the knee: a proof-of-concept clinical trial. Stem Cells 32, 1254–1266 (2014).
Dennis, J. E. et al. A quadripotential mesenchymal progenitor cell isolated from the marrow of an adult mouse. J. Bone Miner. Res. 14, 700–709 (1999).
Pittenger, M. F. et al. Multilineage potential of adult human mesenchymal stem cells. Science 284, 143–147 (1999).
Prockop, D. J. Marrow stromal cells as stem cells for nonhematopoietic tissues. Science 276, 71–74 (1997).
Turinetto, V., Vitale, E. & Giachino, C. Senescence in human mesenchymal stem cells: functional changes and implications in stem cell-based therapy. Int. J. Mol. Sci. 17, E1164 (2016).
Bonab, M. M. et al. Aging of mesenchymal stem cell in vitro. BMC Cell. Biol. 7, 14 (2006).
Li, Z. et al. Epigenetic dysregulation in mesenchymal stem cell aging and spontaneous differentiation. PLoS ONE 6, e20526 (2011).
Hellingman, C. A. et al. Fibroblast growth factor receptors in in vitro and in vivo chondrogenesis: relating tissue engineering using adult mesenchymal stem cells to embryonic development. Tissue Eng. Part A 16, 545–556 (2010).
Scotti, C. et al. Recapitulation of endochondral bone formation using human adult mesenchymal stem cells as a paradigm for developmental engineering. Proc. Natl Acad. Sci. USA 107, 7251–7256 (2010).
Mohyeldin, A., Garzon-Muvdi, T. & Quinones-Hinojosa, A. Oxygen in stem cell biology: a critical component of the stem cell niche. Cell Stem. Cell 7, 150–161 (2010).
Forristal, C. E., Wright, K. L., Hanley, N. A., Oreffo, R. O. & Houghton, F. D. Hypoxia inducible factors regulate pluripotency and proliferation in human embryonic stem cells cultured at reduced oxygen tensions. Reproduction 139, 85–97 (2010).
Fotia, C., Massa, A., Boriani, F., Baldini, N. & Granchi, D. Hypoxia enhances proliferation and stemness of human adipose-derived mesenchymal stem cells. Cytotechnology 67, 1073–1084 (2015).
Gaspar Tosato, M. et al. Resveratrol enhancement on survival of staphylococcus aureus under levofloxacin and photodynamic treatments. Int. J. Antimicrob. Agents 51, 255–259 (2017).
Zadeh-Ardabili, P. M. et al. Palm vitamin E reduces locomotor dysfunction and morphological changes induced by spinal cord injury and protects against oxidative damage. Sci. Rep. 7, 14365 (2017).
Papuc, C., Predescu, C. N., Tudoreanu, L., Nicorescu, V. & Gajaila, I. Comparative study of the influence of hawthorn (Crataegus monogyna) berries ethanolic extract and butylated hydroxylanisole (BHA) on lipid peroxidation, myoglobin oxidation, consistency and firmness of minced pork during refrigeration. J. Sci. Food Agric. 98, 1346–1361 (2017).
Omaye, S. T., Reddy, K. A. & Cross, C. E. Effect of butylated hydroxytoluene and other antioxidants on mouse lung metabolism. J. Toxicol. Environ. Health 3, 829–836 (1977).
Gülçin, İ. Antioxidant properties of resveratrol: a structure–activity insight. Innov. Food Sci. Emerg. 11, 210–218 (2010).
Bonilla, J., Atares, L., Chiralt, A. & Vargas, M. Recent patents on the use of antioxidant agents in food. Recent Pat. Food Nutr. Agric. 3, 123–132 (2011).
Signorelli, P. & Ghidoni, R. Resveratrol as an anticancer nutrient: molecular basis, open questions and promises. J. Nutr. Biochem. 16, 449–466 (2005).
Valenzano, D. R. et al. Resveratrol prolongs lifespan and retards the onset of age-related markers in a short-lived vertebrate. Curr. Biol. 16, 296–300 (2006).
Joe, A. K. et al. Resveratrol induces growth inhibition, S-phase arrest, apoptosis, and changes in biomarker expression in several human cancer cell lines. Clin. Cancer Res. 8, 893–903 (2002).
de la Lastra, C. A. & Villegas, I. Resveratrol as an anti-inflammatory and anti-aging agent: mechanisms and clinical implications. Mol. Nutr. Food Res. 49, 405–430 (2005).
Peltz, L. et al. Resveratrol exerts dosage and duration dependent effect on human mesenchymal stem cell development. PLoS ONE 7, e37162 (2012).
Yuan, H. F. et al. SIRT1 is required for long-term growth of human mesenchymal stem cells. J. Mol. Med. 90, 389–400 (2012).
Dai, Z. et al. Resveratrol enhances proliferation and osteoblastic differentiation in human mesenchymal stem cells via ER-dependent ERK1/2 activation. Phytomedicine 14, 806–814 (2007).
Yoon, D. S. et al. SIRT1 directly regulates SOX2 to maintain self-renewal and multipotency in bone marrow-derived mesenchymal stem cells. Stem Cells 32, 3219–3231 (2014).
Caldarelli, I. et al. Resveratrol mimics insulin activity in the adipogenic commitment of human bone marrow mesenchymal stromal cells. Int. J. Biochem. Cell. Biol. 60, 60–72 (2015).
Bäckesjö, C.-M., Li, Y., Lindgren, U. & Haldosén, L.-A. Activation of Sirt1 decreases adipocyte formation during osteoblast differentiation of mesenchymal stem cells. J. Bone Miner. Res. 21, 993–1002 (2006).
Fischer-Posovszky, P. et al. Resveratrol regulates human adipocyte number and function in a Sirt1-dependent manner. Am. J. Clin. Nutr. 92, 5–15 (2010).
Hellingman, C. A. et al. Smad signaling determines chondrogenic differentiation of bone-marrow-derived mesenchymal stem cells: inhibition of Smad1/5/8P prevents terminal differentiation and calcification. Tissue Eng. Part A 17, 1157–1167 (2011).
Cook, J. L. et al. Animal models of cartilage repair. Bone Joint Res. 3, 89–94 (2014).
Sotiropoulou, P. A., Perez, S. A., Salagianni, M., Baxevanis, C. N. & Papamichail, M. Characterization of the optimal culture conditions for clinical scale production of human mesenchymal stem cells. Stem Cells 24, 462–471 (2006).
Duggal, S. & Brinchmann, J. E. Importance of serum source for the in vitro replicative senescence of human bone marrow derived mesenchymal stem cells. J. Cell. Physiol. 226, 2908–2915 (2011).
Backesjo, C. M., Li, Y., Lindgren, U. & Haldosen, L. A. Activation of Sirt1 decreases adipocyte formation during osteoblast differentiation of mesenchymal stem cells. Cells Tissues Organs 189, 93–97 (2009).
Buhrmann, C., Busch, F., Shayan, P. & Shakibaei, M. Sirtuin-1 (SIRT1) is required for promoting chondrogenic differentiation of mesenchymal stem cells. J. Biol. Chem. 289, 22048–22062 (2014).
Kim, H. J., Braun, H. J. & Dragoo, J. L. The effect of resveratrol on normal and osteoarthritic chondrocyte metabolism. Bone Joint Res. 3, 51–59 (2014).
Horwitz, E. M. et al. Isolated allogeneic bone marrow-derived mesenchymal cells engraft and stimulate growth in children with osteogenesis imperfecta: Implications for cell therapy of bone. Proc. Natl Acad. Sci. USA 99, 8932–8937 (2002).
Zhao, K. et al. Immunomodulation effects of mesenchymal stromal cells on acute graft-versus-host disease after hematopoietic stem cell transplantation. Biol. Blood Marrow Transplant. 21, 97–104 (2015).
Chen, J. et al. Correlation of in vivo bone formation capability and in vitro differentiation of human bone marrow stromal cells. J. Med. Dent. Sci. 52, 27–34 (2005).
Siddappa, R., Licht, R., van Blitterswijk, C. & de Boer, J. Donor variation and loss of multipotency during in vitro expansion of human mesenchymal stem cells for bone tissue engineering. J. Orthop. Res. 25, 1029–1041 (2007).
Koh, Y. G., Kwon, O. R., Kim, Y. S., Choi, Y. J. & Tak, D. H. Adipose-derived mesenchymal stem cells with microfracture versus microfracture alone: 2-year follow-up of a prospective randomized trial. Arthroscopy 32, 97–109 (2016).
Yoon, D. S. et al. Interleukin-6 induces the lineage commitment of bone marrow-derived mesenchymal multipotent cells through down-regulation of Sox2 by osteogenic transcription factors. FASEB J. 28, 3273–3286 (2014).
Yoon, D. S., Choi, Y., Choi, S. M., Park, K. H. & Lee, J. W. Different effects of resveratrol on early and late passage mesenchymal stem cells through beta-catenin regulation. Biochem. Biophys. Res. Commun. 467, 1026–1032 (2015).
Lee, S. et al. microRNA-495 inhibits chondrogenic differentiation in human mesenchymal stem cells by targeting Sox9. Stem Cells Dev. 23, 1798–1808 (2014).
Park, K. W. et al. Inhibition of microRNA-449a prevents IL-1beta-induced cartilage destruction via SIRT1. Osteoarthr. Cartil. 24, 2153–2161 (2016).
Yoon, D. S. et al. Cell recruiting chemokine-loaded sprayable gelatin hydrogel dressings for diabetic wound healing. Acta Biomater. 38, 59–68 (2016).
Lee, Y. et al. In situ forming gelatin-based tissue adhesives and their phenolic content-driven properties. J. Mater. Chem. B 1, 2407–2414 (2013).
Yoon, D. S. et al. Synergistic action of IL-8 and bone marrow concentrate on cartilage regeneration through upregulation of chondrogenic transcription factors. Tissue Eng. Part A 22, 363–374 (2016).
Choi, M. Y. et al. Engineered extracellular microenvironment with a tunable mechanical property for controlling cell behavior and cardiomyogenic fate of cardiac stem cells. Acta Biomater. 50, 234–248 (2017).
O’Driscoll, S. W., Keeley, F. W. & Salter, R. B. Durability of regenerated articular cartilage produced by free autogenous periosteal grafts in major full-thickness defects in joint surfaces under the influence of continuous passive motion. A follow-up report at one year. J. Bone Joint Surg. Am. 70, 595–606 (1988).
This study was supported by Basic Science Research Program through the National Research Foundation of Korea (NRF) funded by the Ministry of Education (No. NRF-2016R1D1A1B03933182), and from the NRF grant funded by the Korea government (MSIP) (NRF-2018R1A2B2004529).
Conflict of interest
The authors declare that they have no conflict of interest.
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Edited by D. Aberdam
Electronic supplementary material
About this article
Cite this article
Choi, S.M., Lee, K., Ryu, S.B. et al. Enhanced articular cartilage regeneration with SIRT1-activated MSCs using gelatin-based hydrogel. Cell Death Dis 9, 866 (2018). https://doi.org/10.1038/s41419-018-0914-1
A comprehensive review on polymeric hydrogel and its composite: Matrices of choice for bone and cartilage tissue engineering
Journal of Industrial and Engineering Chemistry (2020)
ACS Applied Materials & Interfaces (2020)
Materials Science and Engineering: R: Reports (2020)
Overexpression of Pitx1 attenuates the senescence of chondrocytes from osteoarthritis degeneration cartilage–A self-controlled model for studying the etiology and treatment of osteoarthritis