- Open Access
Adipose stem cells can secrete angiogenic factors that inhibit hyaline cartilage regeneration
Stem Cell Research & Therapy volume 3, Article number: 35 (2012)
Adipose stem cells (ASCs) secrete many trophic factors that can stimulate tissue repair, including angiogenic factors, but little is known about how ASCs and their secreted factors influence cartilage regeneration. Therefore, the aim of this study was to determine the effects ASC-secreted factors have in repairing chondral defects.
ASCs isolated from male Sprague Dawley rats were cultured in monolayer or alginate microbeads supplemented with growth (GM) or chondrogenic medium (CM). Subsequent co-culture, conditioned media, and in vivo cartilage defect studies were performed.
ASC monolayers and microbeads cultured in CM had decreased FGF-2 gene expression and VEGF-A secretion compared to ASCs cultured in GM. Chondrocytes co-cultured with GM-cultured ASCs for 7 days had decreased mRNAs for col2, comp, and runx2. Chondrocytes treated for 12 or 24 hours with conditioned medium from GM-cultured ASCs had reduced sox9, acan, and col2 mRNAs; reduced proliferation and proteoglycan synthesis; and increased apoptosis. ASC-conditioned medium also increased endothelial cell tube lengthening whereas conditioned medium from CM-cultured ASCs had no effect. Treating ASCs with CM reduced or abolished these deleterious effects while adding a neutralizing antibody for VEGF-A eliminated ASC-conditioned medium induced chondrocyte apoptosis and restored proteoglycan synthesis. FGF-2 also mitigated the deleterious effects VEGF-A had on chondrocyte apoptosis and phenotype. When GM-grown ASC pellets were implanted in 1 mm non-critical hyaline cartilage defects in vivo, cartilage regeneration was inhibited as evaluated by radiographic and equilibrium partitioning of an ionic contrast agent via microCT imaging. Histology revealed that defects with GM-cultured ASCs had no tissue ingrowth from the edges of the defect whereas empty defects and defects with CM-grown ASCs had similar amounts of neocartilage formation.
ASCs must be treated to reduce the secretion of VEGF-A and other factors that inhibit cartilage regeneration, which can significantly influence how ASCs are used for repairing hyaline cartilage.
Adult stem cells, such as adipose stem cells (ASCs) are an emerging clinical option for treating tissue damage and diseases because of their accessibility and ability to differentiate into multiple cell lineages [1, 2]. More recently, ASCs and other adult stem cells have been shown to secrete a wide range of trophic factors that can stimulate regeneration of tissues from multiple lineages . As these cell therapies become more prevalent in different clinical procedures, their secretory profiles need to be more thoroughly investigated in terms of the role stem cell-secreted factors have in tissue regeneration and in possible side effects.
Hyaline cartilage is the most prevalent cartilaginous tissue found in the body, with adult stem cell therapies used to regenerate hyaline cartilage in the knee and trachea of humans [4, 5] and to repair cartilage in the larynx, bronchial stump, and growth plate of animals in preclinical studies [6–8]. Unlike most other tissues, hyaline cartilage is an avascular and aneural tissue that has complex spatial variation in its mechanical properties and composition despite a relatively homogeneous cell population. Therefore, adult stem cell therapies used for repair of chondral defects must secrete factors that stimulate synthesis of specific proteoglycans and collagens without facilitating the infiltration of other tissues, especially blood vessel formation, or enabling hypertrophic differentiation of chondrocytes typical of endochondral ossification.
Although the secretory profile of ASCs for cartilage regeneration has been investigated , an in-depth study determining the role ASC-secreted factors have in chondrocyte proliferation, phenotype, and cartilage regeneration has yet to be conducted. Additionally, techniques such as microencapsulation and differentiation medium treatments have been used to improve the regenerative capacity for mesenchymal stem cells [10–12], but no study has investigated the effects these two parameters have on the secretion of trophic factors from ASCs. Therefore, the overall objective of this study was to determine the role ASC-secreted trophic factors have in cartilage regeneration. The effect of microencapsulation and chondrogenic medium treatment on angiogenic factor production was first determined. Then co-culture and conditioned media studies were conducted to determine how ASC-paracrine signaling and ASC-secreted factors affect chondrocytes. Finally, ASCs were implanted into a chondral defect in the xiphoid to determine the effect ASCs have on hyaline cartilage regeneration.
Materials and methods
For each experiment, ASCs were isolated from inguinal fat pads of six 125-g male Sprague Dawley rats (Harlan Laboratories, Indianapolis, IN, USA) under a protocol approved by the Institutional Animal Care and Use Committee of the Georgia Institute of Technology as described in detail previously . ASCs from the six animals were then combined and cultured in Lonza mesenchymal stem cell growth medium (GM) (Lonza, Walkersville, MD, USA). After one passage, these cells were positive for CD73 and CD271 and negative for CD45 . Non-matching costochondral chondrocytes from the ribs of a different set of six 125-g male Sprague Dawley rats were isolated and combined as described previously . Primary chondrocytes were cultured in DMEM containing 10% fetal bovine serum (FBS) and 50 μg/mL ascorbic acid (Invitrogen) until the fourth passage prior to experimental analysis. These cells continue to express type II collagen, aggrecan, and cartilage oligomeric matrix protein .
Once primary ASCs reached 90% confluence, cells were trypsinized and microencapsulated in 20 mg/mL low molecular weight (approximately 150 kDa) alginate (FMC BioPolymer, Sandvika, Norway) with a high mannuronate to guluronate ratio (40% guluronate) at a concentration of 25 × 106 cells/mL using a Nisco Encapsulator VAR V1 LIN-0043 (Nisco Engineering AG, Zurich, Switzerland) as previously described . The microbeads were washed three times in GM prior to cell culture studies. First passage ASCs were also plated in 6-well plates (Figure 1A).
ASC cell culture
Once first passage ASCs reached 90% confluence (Figure 1A), ASC monolayers and microbeads were then treated for 5 days with either GM or chondrogenic medium (CM) consisting of high-glucose DMEM with 1 mM sodium pyruvate (Mediatech, Manassas, VA, USA), 40 μg/mL proline (Sigma, St. Louis, MO, USA), 50 μg/mL ascorbate-2-phosphate (Sigma), 1% ITS+ (Sigma), 100 nM dexamethasone (Sigma), 10 ng/mL recombinant human transforming growth factor beta-1 (TGF-β1) (R&D Systems, Minneapolis, MN, USA) and 100 ng/mL recombinant human bone morphogenic protein 6 (BMP-6) (PeproTech, Rocky Hill, NJ, USA). Once media were changed on the fifth day, RNA was collected after 8 hours as described below while media and ASCs lysed in 0.05% Triton X-100 were collected after 24 hours. Fourth passage chondrocytes cultured in DMEM, 10% FBS, and 50 μg/mL ascorbic acid and Sprague Dawley-derived clone 9 liver cells (ATCC, Manassas, VA, USA) cultured in F12K medium and 10% FBS served as controls. All media contained 1% penicillin and streptomycin.
Growth factor expression and production
Microbeads were un-cross-linked in 82.5 mM sodium citrate (Sigma), pelleted at 500 g for 10 minutes and washed two more times in sodium citrate to remove any residual alginate. TRIzol reagent (Invitrogen, Grand Island, NY, USA) was added to the resulting cell pellet, homogenized using a QIAshredder (QIAGEN, Valencia, CA, USA), and RNA was isolated using chloroform and an RNeasy Kit (Qiagen) as previously described . Then 1 μg RNA was reverse-transcribed to cDNA using a High Capacity Reverse Transcription cDNA kit (Applied Biosystems, Carlsbad, CA, USA). Gene expressions were quantified as previously described . Primers were designed using Beacon Designer software (Premier Biosoft, Palo Alto, CA, USA) and synthesized by Eurofins MWG Operon (Huntsville, AL, USA) unless otherwise noted (Table 1). Vascular endothelial growth factor (VEGF)-A and fibroblast growth factor (FGF)-2 production over the last 24 hours of culture was quantified using ELISA (R&D Systems) and normalized to DNA content measured with a Quant-iT PicoGreen kit (Invitrogen). Quantified mRNA levels are referred to by the name of the gene (for example, fgf2, vegfa, runx2) whereas quantified protein levels are referred to by the name of the growth factor (for example FGF-2, VEGF-A).
To assess the effects that paracrine signaling between ASCs and chondrocytes have on chondrocyte phenotype, the two cell types were co-cultured in a trans-well system (Figure 2A). Initial studies determined the number of microbeads per insert needed to have the same cell number as ASC-confluent trans-well inserts. ASC monolayers and microbeads were treated with GM or with CM for 5 days in 0.2 μm high density cell culture inserts (BD Biosciences, Franklin Lakes, NJ, USA). ASC cultures and inserts were then washed in DMEM three times and added to wells with confluent chondrocytes. The two cell groups were then cultured in 4.5 mL DMEM + 10% FBS. After 7 days, RNA was isolated from the chondrocytes to quantify chondrogenic gene expression. Microencapsulated clone 9 liver cells served as a control.
Chondrocyte cultures treated with ASC-conditioned media
To assess the effects ASC-secreted factors have on them, chondrocytes were cultured in different ASC-conditioned media (Figure 2C) obtained from T-75 flasks. Initial studies determined the number of microbeads per T-75 needed to have the same cell number as ASC-confluent T-75 flasks. To obtain ASC-conditioned media, ASC monolayers and microbeads were treated with GM or CM for 5 days in T-75s. After the fifth day of treatment, ASC monolayers and microbeads were washed in DMEM three times and 10 mL DMEM + 10% FBS were added to each culture. After 24 hours, media containing the ASC-secreted factors were collected then immediately added to confluent chondrocyte cultures. After 12 hours in ASC-conditioned medium, RNA was isolated from chondrocytes to quantify chondrogenic gene expression. To assess chondrocyte phenotype, apoptosis, and proliferation, the following assays were performed after 24 hours of treatments with ASC-conditioned medium. These time points were selected based upon previous studies investigating the effects of different signaling molecules on chondrocytes [18–20]. Conditioned medium from microencapsulated clone 9 liver cells served as a control.
Incorporation of [3H]- thymidine
DNA synthesis was assayed by measuring [3H]-thymidine incorporation as described previously . Forty%-confluent chondrocytes were treated with DMEM + 1% FBS to induce quiescence. Four hours before harvest, [3H]-thymidine was added to a final concentration of 0.25 μCi/mL. Radioactivity in trichloroacetic acid-insoluble cell precipitates was measured by liquid scintillation spectroscopy.
Incorporation of [35S]- sulfate
Proteoglycan synthesis was assayed by measuring [35S]-sulfate incorporation as previously described . The [35S]-sulfate was added to a final concentration of 18 μCi/mL for the final 4 hours of culture. Only [35S]-sulfate incorporation in the monolayer was measured since less than 15% of total radiolabeled proteoglycan production is secreted into the medium . The [35S]-sulfate incorporation was normalized to protein content measured with a Pierce Macro BCA protein kit (ThermoScientific, Rockford, IL, USA).
Alkaline phosphatase activity
Alkaline phosphatase-specific activity in chondrocyte lysates was measured as a function of release of p-nitrophenol from p-nitrophenylphosphate as previously described  and normalized to protein content measured with a Pierce Macro BCA protein kit (ThermoScientific).
Effects of ASCs on chondrocyte apoptosis
To assess the effects of ASC-secreted factors on DNA fragmentation, confluent chondrocytes were pulsed with [3H]-thymidine for 4 hours prior to treatment with ASC-conditioned medium. Chondrocytes were lysed and centrifuged at 13,000 g for 15 minutes to separate intact DNA from fragmented DNA as previously described . The amount of incorporated [3H]-thymidine was determined in each fraction to establish the total amount of fragmented DNA.
Caspase-3 activity was determined using a colorimetric CaspACE™ Assay System from Promega (Madison, WI, USA) following the manufacturer's protocol, 24 hours after ASC-conditioned media were added to confluent chondrocytes. Caspase-3 activity was normalized to total protein content measured with a Pierce 660 nm protein assay (ThermoScientific).
Effect of secreted factors on angiogenic response
Fibrin gel assay
Angiogenic responses to different ASC-conditioned media were assessed with endothelial cells cultured in a fibrin gel assay as previously described . Human aortic endothelial cells (HAECs) (Lonza) were plated in endothelial cell basal medium (EGM)-2 (Lonza) at 5 × 103 cells/well on fibrin gel and cultured at 37°C for 24 hours. At 24 hours, medium was removed, a second layer of fibrin was added on top, and ASC-conditioned media were added. After 12 hours, images were taken for morphometric analysis and total endothelial tube length was determined using Image Pro Plus.
Role of VEGF-A and FGF-2
To determine the effect exogenous VEGF-A and FGF-2 have on chondrocytes, 1 ng/mL and 20 ng/mL of recombinant human VEGF-A165, and recombinant human FGF-2 (R&D Systems), were added to monolayer cultures of fourth-passage chondrocytes. These concentrations were selected based upon a prior dose-response study on mesenchymal stem cells , and because measured VEGF-A concentrations among the different conditioned media groups ranged from 1 to 20 ng/mL. To determine the effect VEGF-A and FGF-2 secreted by ASCs have on chondrocytes, conditioned medium from GM-treated ASC monolayers was supplemented with 1 μg/mL goat anti rat IgG, 1 μg/mL goat anti-rat VEGF-A neutralizing antibody, or 1 μg/mL goat anti-rat FGF-2 neutralizing antibody (R&D Systems) and added to fourth-passage chondrocyte monolayers as determined by the manufacturer's protocol. After 24 hours, [35S]-sulfate incorporation, caspase-3 activity, and incorporation of [3H]-thymidine were measured as described above. DMEM + 10% FBS and conditioned medium from ASC monolayers treated with CM served as controls.
Xiphoid defect in vivo
To assess if ASCs would inhibit cartilage regeneration, non-critically sized chondral defects were made in the xiphoids of 125-g male Sprague-Dawley rats as previously described . The protocol was approved by the Institutional Animal Care and Use Committee of the Georgia Institute of Technology and each group was tested in seven rats. A full-thickness 1 mm cylindrical defect was made in the center of the xiphoid using a dermal biopsy punch (Mitex, Plainsboro, NJ, USA). This defect size was chosen because cartilage regeneration was previously observed after 35 days and the defect is large enough to contain cell pellets 1 × 106 ASCs in size . ASC monolayers cultured in GM or CM were pelleted at 1 × 106 ASCs/pellet and implanted into the defect. Empty defects and autografts (excised cartilage is re-implanted) served as controls. To maintain groups in the defect and to serve as an adhesion barrier, SepraFilm® (Genzyme, Cambridge, MA, USA) was then placed on the dorsal and ventral sides of the defect. Xiphoids were excised 35 days post-surgery and examined as described below.
Radiographic imaging (Faxitron Bioptics, Lincolnshire, IL, USA) was performed in the coronal plane at a voltage of 22 mV and exposure time of 16 s to visualize soft tissue penetration as previously described . Four observers with experience in examining radiographic images then scored the images blinded, for the presence of soft tissue penetration, with a score of 0 representing no healing, a score of 0.5 representing partial healing, and a score of 1 representing full healing. The average score each observer gave for each group was used for statistical analysis (n = 4).
Equilibrium partitioning of an ionic contrast agent via micro-computed tomography (EPIC-μCT, μCT40, SCANCO Medical, Brüttisellen, Switzerland) was used to visualize the distribution of proteoglycans within the xiphoid defects as previously described [25, 26]. Xiphoids were incubated in 40% Hexabrix (Mallinckrodt, St. Louis, MO, USA) in PBS containing 1% proteinase inhibitor cocktail (CalBiochem, Darmstadt, Germany) overnight and scanned using pre-determined settings . Low x-ray attenuation (green/yellow) of three-dimensional color images corresponded to regions of high proteoglycan concentration; no, or high x-ray attenuation (black and red/orange) indicated regions of low proteoglycan concentration. To determine cartilage volume, user-guided contours corresponding to a 1.1-mm cylinder around the defect were drawn and evaluated at a 100 to 250 threshold range. This contour size was chosen so all cartilage integrity, in-growth, and integration at the defect edge would be taken into account. Thus, all groups had positive cartilage volume since the evaluation volume was larger than the defect volume.
After scanning, samples were washed in PBS for four hours, fixed in 10% phosphate-buffered formalin for 48 hours, and embedded in paraffin. Serial sections, 7-μm thick, were stained with H&E to highlight cells and extracellular matrix on microscope images (DMLB; Leica, Nussloch, Germany).
All in vitro experiments included six independent cultures per treatment group to ensure sufficient power to detect statistically significant differences. All in vitro experiments were conducted multiple times to validate the observations, but only data from a single representative experiment are shown and are expressed as means ± standard error (SE). A power analysis determined that seven samples per group were needed for the in vivo study based on results from a previous study . Statistical analysis was conducted using analysis of variance (ANOVA) with the post hoc Tukey test (GraphPad Prism, La Jolla, CA, USA). Differences in means were considered to be statistically significant if the P-value was less than 0.05.
Angiogenic growth factor production from ASCs
ASC monolayers and microbeads cultured in GM had 1.5 to 3.0 times higher levels of fgf2 and vegfa compared to chondrocytes while CM reduced both vegfa and fgf2 to levels similar to that of chondrocytes (Figure 1B). CM did not influence pdgfa in ASCs, which was half the mRNA level seen in chondrocytes. ASC monolayers and microbeads secreted 10 to 30 times more VEGF-A than chondrocytes, while CM reduced secretion by 3.0- to 3.5-fold (Figure 1C). FGF-2 secretion from ASC cultures and chondrocytes was very low compared to VEGF-A production.
Effect of ASC paracrine signaling and secreted factors on chondrocyte gene expression
Chondrocytes co-cultured with ASC monolayers cultured in GM experienced 3.5- to 4.0-fold reductions in col2, comp, and runx2 compared to chondrocytes with no co-culture (Figure 2B). However, CM-treated ASC monolayers increased acan in chondrocytes and had no effect on col2, comp, and runx2 in chondrocytes compared to the control. GM-cultured ASC microbeads reduced col2 in chondrocytes but CM-treated ASC microbeads reduced col2, comp, and runx2 in chondrocytes compared to control. ASC co-cultures did not affect sox-9 and co-culture with clone 9 liver cell microbeads did not influence chondrocyte gene expression compared to the control.
Conditioned medium from GM-cultured ASC monolayers added to chondrocytes increased sox9 by 50%, acan by 78%, and col2 by 35% compared to control medium added to chondrocytes (Figure 2D). However, conditioned medium from CM-treated ASC monolayers had no effect on chondrogenic mRNA levels compared to control medium. Conditioned medium from GM-cultured ASC microbeads decreased acan, but conditioned medium from CM-treated ASC microbeads had no effect on chondrocyte mRNA levels. Clone 9 liver cell microbeads decreased acan in chondrocytes but had no effect on sox9, col2, comp, or runx2.
Effect of ASC-secreted factors on proliferation, phenotype, and apoptosis
Conditioned media from GM-cultured ASC monolayer and microbeads decreased [35S]-sulfate incorporation by 75% and 60% respectively (Figure 3B), had no effect on alkaline phosphatase activity (Figure 3C), and decreased [3H]-thymidine incorporation by approximately 76% (Figure 3D) compared to chondrocytes treated with control medium. Treating ASC monolayers and microbeads with CM prior to conditioned media collection eliminated the deleterious effects ASC-secreted factors had on chondrocytes (Figure 3B, D). Liver microbead-conditioned medium did not affect [3H]-thymidine incorporation, [35S]-sulfate incorporation, or alkaline phosphatase activity (Figure 3B-D).
Conditioned medium from GM-cultured ASC monolayers increased caspase-3 activity 120%, bax/bcl expression 79%, and DNA fragmentation 114% compared to control medium (Figure 3E-G). Treating ASC monolayers with CM prior to collecting conditioned medium eliminated the apoptotic effects ASC-secreted factors had on chondrocytes. Conditioned medium from ASC microbeads cultured in GM did not increase apoptosis compared to control medium. Conditioned medium from liver microbeads had no effect on caspase-3 activity and bax/bcl, but did increase DNA fragmentation compared to the control (Figure 3E-G).
ASC monolayer and microbead-conditioned media increased endothelial tube length by 2.6- and 2.0-fold respectively (Figure 3G). Treating ASC monolayers and microbeads with CM prior to conditioned media collection eliminated this angiogenic response. Conditioned medium from liver microbeads had no effect on endothelial tube length.
Effect of exogenous VEGF-A and FGF-2 on chondrocytes
The incorporation of 35S-sulfate was reduced by approximately 30% and 50% with the addition of 1 ng/mL and 20 ng/mL of VEGF-A, respectively (Figure 4A). Adding FGF-2 at both 1 and 20 ng/mL alone had no effect on 35S-sulfate incorporation but did eliminate the inhibitory effect rhVEGF-A had on 35S-sulfate incorporation at both concentrations. Addition of VEGF-A at concentrations of 1 ng/mL and 20 ng/mL significantly increased caspase-3 activity by 32% and 84%, respectively (Figure 4B). Adding 1 ng/mL of FGF-2 had no effect on caspase-3 activity and did not reduce the apoptotic effect of VEGF-A compared to the control. However, 20 ng/mL FGF-2 eliminated the apoptotic effect of VEGF-A. VEGF-A and FGF-2 had a more limited effect on chondrocyte proliferation, as only the 20 ng/mL FGF-2 dosage increased [3H]-thymidine incorporation (Figure 4C).
Effect of ASC-secreted VEGF-A and FGF-2 on chondrocytes
ASC-conditioned medium with a goat-anti-rat IgG and FGF-2 neutralizing antibody decreased [35S]-sulfate incorporation by approximately 50% (Figure 5B), and increased caspase-3 activity by approximately 94% (Figure 5C) compared to control medium. Adding VEGF-A neutralizing antibody to ASC-conditioned medium eliminated both its deleterious effect on chondrocyte phenotype and its apoptotic effect. ASC-conditioned medium with or without VEGF-A or FGF-2 neutralizing antibodies all decreased [3H]-thymidine incorporation compared to control medium (Figure 5D). As previously observed, conditioned medium from ASC monolayers treated with CM had no effect on chondrocyte caspase-3 activity, [35S]-sulfate, and [3H]-thymidine incorporation compared to control medium (data not shown).
Effect of ASCs in cartilage defects
Scoring of radiographic images showed that all seven defects with autografts had partial or full healing and three of seven empty defects had partial or full healing; however, no more than two of seven defects with ASC pellets had partial healin, whereas four of seven defects with pellets of ASCs treated with CM had partial or full healing (Figure 6A). Scores for healing for the empty defects, defects with ASCs treated with CM, and defects with autografts were all higher than for defects with ASC pellets. Scores for defects with ASCs treated with CM were not statistically different from scores for the empty defects, and were lower than scores for defects with the autografts (Figure 6A).
Proteoglycan was visible in EPIC-μCT images of empty defects and defects with pellets of CM-treated ASCs but absent from defects with pellets of GM-cultured ASCs (Figure 6B). EPIC-μCT-calculated cartilage volume for defects with ASC pellets was significantly smaller than cartilage volume in both autografts and empty defects. Defects with CM-treated ASCs had more cartilage than defects with GM-cultured ASCs, but were not different from empty defects (Figure 6B).
In histological sections of defects with autografts, early-stage cartilage and infiltrating cells were starting to integrate the graft with the surrounding xiphoid (Figure 6C). Similar tissue deposition and cell infiltration was observed for empty defects and defects with ASCs treated with chondrogenic media. However, defects with ASCs were infiltrated with surrounding epithelial tissue instead and lacked the connective tissue that was observed in empty defects (Figure 6C).
This study is the first to definitively show that ASCs secrete angiogenic factors that are detrimental for chondrocytes and can prevent cartilage regeneration. Specifically, ASCs secrete a relatively large amount of VEGF-A, which can inhibit chondrocyte phenotype and lead to chondrocyte apoptosis. Additionally, ASCs secrete factors that negatively influence chondrocyte proliferation. Finally, ASCs prevent cartilage regeneration in a non-critical, hyaline cartilage defect in vivo. Despite these deleterious effects, treating ASCs with chondrogenic medium can reduce the expression and production of VEGF-A, eliminate the damaging effects ASC-secreted factors have on chondrocytes, and prevent the adverse effects ASCs have on regenerating cartilage in vivo.
In addition to chondrogenic medium, microencapsulation had a significant effect on VEGF-A and FGF-2 secretions. Specifically, microencapsulation had the opposite effect of chondrogenic medium and increased the secretion of these angiogenic factors. Hypoxia due to the high cell density within the microbead may have increased VEGF-A and FGF-2 secretions. Hypoxic conditions can increase VEGF-A and FGF-2 secretion from ASCs  since the genes for these angiogenic factors have hypoxia response elements [28, 29]. Although we did not assay for hypoxic conditions within the microbead, increasing cell concentrations within hydrogels has been shown to increase oxygen tension and gradients . Cell density may therefore be an important variable in controlling growth factor secretion from ASC microbeads.
Previous studies have extensively studied the secretory profiles of bone marrow-derived mesenchymal stem cells (MSCs) and ASCs, showing that they not only secrete several factors that can facilitate cartilage regeneration [9, 31], but that they also secrete a large amount of angiogenic factors [32, 33]. VEGF-A, an important initiator and mediator of angiogenesis [34, 35], was secreted in large quantities by ASC monolayers and microbeads, decreased chondrocyte proteoglycan production, and induced chondrocyte apoptosis in the current study. Although VEGF-A typically elicits anabolic responses from most cell types, this growth factor has catabolic effects on chondrocytes and has been shown to induce matrix metalloproteinase expression in these cells . Although VEGF-A was not responsible for reduced chondrocyte proliferation due to ASC-secreted factors, ASCs also secrete pro-inflammatory factors IL-6, 8, and 11, and TNFα , which may have inhibited chondrocyte proliferation.
Although VEGF-A alone did not prevent chondrocyte proliferation, it mitigated the ability of FGF-2 to stimulate chondrocyte proliferation at a high concentration. Additionally, FGF-2 restored proteoglycan production in chondrocytes treated with VEGF-A, and high concentrations of FGF-2 eliminated the apoptotic effect VEGF-A had on chondrocytes. While both FGF-2 and VEGF-A are important facilitators for angiogenesis [38, 39] and their corresponding mRNA levels in ASCs experienced similar decreases when treated with chondrogenic medium, ASCs secreted at least 10-fold less FGF-2 than VEGF-A. Furthermore, unlike VEGF-A, FGF-2 has previously been shown to enhance the chondrogenic potential of different stem cell sources [40, 41], as well as improve cartilage regeneration [42, 43]. The combination of high VEGF-A secretion and low FGF-2 secretion may be the main reason why ASC-secreted factors have deleterious effects on chondrocytes and subsequent cartilage regeneration.
VEGF enhances catabolic pathways in chondrocytes, and VEGF signaling has been associated with osteophyte formation and progression of osteoarthritis in articular cartilage [44–46]. Moreover, blocking VEGF signaling improves the chondrogenic potential and regenerative capacity of muscle-derived stem cells [47, 48]. Additionally, VEGF-A directs cartilage vascularization in hyaline cartilage and hypertrophic chondrocyte absorption that leads to subsequent ossification [49, 50]. Although chondrocytes exposed to ASC-secreted factors did not have increased mRNA levels corresponding to RUNX2 or increased alkaline phosphatase activity, and cartilage defects with ASC pellets did not have signs of vascularization, hypertrophic differentiation, or bone formation, in vitro conditioned media studies longer than 24 hours or in vivo studies longer than 35 days may have revealed these effects. Additionally, ASCs may secrete trophic factors that prevent hypertrophic differentiation.
In addition to affecting hypertrophic differentiation, the length of exposure to ASC-secreted factors and the time points measured appear to be important variables in regulating chondrocyte phenotype. Twelve hour exposure to ASC-conditioned medium appeared to have the most significant effects on mRNA levels corresponding to SOX9 and aggrecan, which are earlier stage markers of chondrogenesis, whereas 7 days of ASC co-culture exerted the greatest effects on mRNA levels corresponding to RUNX2, a later stage chondrogenic marker . Because these unique phenotypic expression profiles for the different stages of chondrogenesis, the time points measured for the co-cultures, conditioned medium, and subsequent studies may have affected the findings on chondrocyte phenotypic expression, proliferation, proteoglycan synthesis, and apoptosis. However, these time points are consistent with previous studies investigating the effects different signaling molecules have on chondrocytes [18, 19, 21]. Additionally, 7-day co-culture with ASCs treated with chondrogenic medium increased aggrecan expression in chondrocytes, and this increase was not observed in the conditioned media study. Although the different time points between the two studies may explain this discrepancy, the interplay between chondrocyte and ASC signaling may also have a contribution.
Several studies have investigated the effects chondrocyte and stem cell co-cultures and chondrocyte-secreted factors have on stem cell differentiation [47, 52, 53], but few have provided insight into the effects stem cell-mediated paracrine signaling has on chondrocytes. Bian et al. showed that co-culturing chondrocytes with MSCs within the same gel reduced hypertrophy and increased compressive moduli, but it appeared that these improvements were independent of long-range MSC-paracrine signaling . Additionally, results from Hildner et al. suggested that co-culturing ASCs and chondrocytes in the same matrix moderately increased SOX9, aggrecan, and cartilage oligomeric protein mRNA expression when normalized to the initial percentage of chondrocytes, but the findings provided little insight into the role of ASC-secreted factors . Although chondrogenic treatment that included both TGF-β1 and BMP-6 eliminated the deleterious effects that ASC-secreted factors and ASCs had on chondrocytes and cartilage regeneration respectively, ASCs treated with chondrogenic medium did not secrete factors that improved the ability of chondrocytes to produce cartilaginous extracellular matrix in vitro. This absence of improvement over baseline may be due to the short 5-day chondrogenic medium-treatment time as several studies have shown optimal ASC and stem cell chondrogenesis to require at least 2 to 6 weeks of chondrogenic treatment [56, 57]. However, these studies did not investigate the effects that varying the temporal application of chondrogenic medium had on trophic factor production. Additionally, assessing cartilage regeneration at longer time points post-operatively may provide better insight into the therapeutic benefit of this group.
This study showed that ASCs can inhibit cartilage regeneration within a focal hyaline cartilage defect in vivo after 35 days. In vitro, ASC monolayers or microbeads cultured in growth medium secreted a large amount of VEGF-A, which caused chondrocyte apoptosis and reduced proteoglycan synthesis after 24 hours of conditioned media treatments. Additionally, these ASCs secreted factors that reduced chondrogenic gene expression and proliferation after 12 and 24 hours of conditioned media treatments respectively. Treating ASCs with chondrogenic medium for 5 days reduced the secretion of VEGF-A, significantly reduced the deleterious effects ASC-secreted factors have on chondrocytes, and eliminated the inhibitory effect ASCs have on cartilage regeneration. Blocking VEGF-A in ASC-conditioned medium eliminated the deleterious effects ASC-secreted factors had on chondrocyte phenotype and apoptosis after 24 hours. Adding a high concentration of FGF-2 eliminated the apoptotic effect VEGF-A had on chondrocytes, and adding both low and high concentrations of FGF-2 eliminated the detrimental effects VEGF-A had on chondrocyte phenotype after 24 hours. These results have significant implications on how ASCs and possibly other stem cell therapies are used for repairing cartilage. Specifically, these therapies must be pre-treated or modified to reduce the inhibitory effects of VEGF-A and other secreted factors on cartilage regeneration.
- ACAN :
analysis of variance
adipose stem cells
bone morphogenetic protein-6
complementary deoxyribonucleic acid
- COL2 :
- COMP :
cartilage oligomeric matrix protein
enzyme-linked immunosorbent assay
equilibrium partitioning of an ionic contrast agent via micro-computed tomography
fetal bovine serum
fibroblast growth factor-2
mesenchymal stem cells
ribosomal protein S18
- RUNX2 :
runt-related transcription factor 2
- SOX9 :
sex determining region Y-box containing gene 9
transforming growth factor-beta 1
tumor necrosis factor
vascular endothelial growth factor-A.
Gimble JM, Guilak F: Differentiation potential of adipose derived adult stem (ADAS) cells. Curr Top Dev Biol. 2003, 58: 137-160.
Gimble J, Guilak F: Adipose-derived adult stem cells: isolation, characterization, and differentiation potential. Cytotherapy. 2003, 5: 362-369. 10.1080/14653240310003026.
Baraniak PR, McDevitt TC: Stem cell paracrine actions and tissue regeneration. Regen Med. 2010, 5: 121-143. 10.2217/rme.09.74.
Macchiarini P, Birchall M, Hollander A, Mantero S, Conconi MT: Clinical transplantation of a tissue-engineered airway Authors' reply. Lancet. 2009, 373: 718-719.
Mobasheri A, Csaki C, Clutterbuck AL, Rahmanzadeh M, Shakibaei M: Mesenchymal stem cells in connective tissue engineering and regenerative medicine: applications in cartilage repair and osteoarthritis therapy. Histol Histopathol. 2009, 24: 347-366.
Hou N, Cui P, Luo J, Ma R, Zhu L: Tissue-engineered larynx using perfusion-decellularized technique and mesenchymal stem cells in a rabbit model. Acta Otolaryngol. 2011, 131: 645-652. 10.3109/00016489.2010.547517.
Gomez-de-Antonio D, Zurita M, Santos M, Salas I, Vaquero J, Varela A: Stem cells and bronchial stump healing. J Thorac Cardiovasc Surg. 2010, 140: 1397-1401. 10.1016/j.jtcvs.2010.03.009.
McCarty RC, Xian CJ, Gronthos S, Zannettino AC, Foster BK: Application of autologous bone marrow derived mesenchymal stem cells to an ovine model of growth plate cartilage injury. Open Orthop J. 2010, 4: 204-210. 10.2174/1874325001004010204.
Kim BS, Kang KS, Kang SK: Soluble factors from ASCs effectively direct control of chondrogenic fate. Cell Prolif. 2010, 43: 249-261. 10.1111/j.1365-2184.2010.00680.x.
Endres M, Wenda N, Woehlecke H, Neumann K, Ringe J, Erggelet C, Lerche D, Kaps C: Microencapsulation and chondrogenic differentiation of human mesenchymal progenitor cells from subchondral bone marrow in Ca-alginate for cell injection. Acta Biomater. 2010, 6: 436-444. 10.1016/j.actbio.2009.07.022.
Moyer HR, Kinney RC, Singh KA, Williams JK, Schwartz Z, Boyan BD: Alginate microencapsulation technology for the percutaneous delivery of adipose-derived stem cells. Ann Plast Surg. 2010, 65: 497-503. 10.1097/SAP.0b013e3181d37713.
Grellier M, Granja PL, Fricain JC, Bidarra SJ, Renard M, Bareille R, Bourget C, Amedee J, Barbosa MA: The effect of the co-immobilization of human osteoprogenitors and endothelial cells within alginate microspheres on mineralization in a bone defect. Biomaterials. 2009, 30: 3271-3278. 10.1016/j.biomaterials.2009.02.033.
Erdman CP, Dosier CR, Olivares-Navarrete R, Baile C, Guldberg RE, Schwartz Z, Boyan BD: Effects of Resveratrol on Enrichment of Adipose-derived Stem Cells and their Differentiation to Osteoblasts in Two and Three Dimensional Cultures. Journal of Tissue Engineering and Regenerative Medicine.
Boyan BD, Schwartz Z, Swain LD, Carnes DL, Zislis T: Differential expression of phenotype by resting zone and growth region costochondral chondrocytes in vitro. Bone. 1988, 9: 185-194. 10.1016/8756-3282(88)90008-7.
Lee CS, Moyer HR, Gittens RA, Williams JK, Boskey AL, Boyan BD, Schwartz Z: Regulating in vivo calcification of alginate microbeads. Biomaterials. 2010, 31: 4926-4934. 10.1016/j.biomaterials.2010.03.001.
Fitzgerald JB, Jin M, Dean D, Wood DJ, Zheng MH, Grodzinsky AJ: Mechanical compression of cartilage explants induces multiple time-dependent gene expression patterns and involves intracellular calcium and cyclic AMP. J Biol Chem. 2004, 279: 19502-19511. 10.1074/jbc.M400437200.
Olivares-Navarrete R, Hyzy SL, Park JH, Dunn GR, Haithcock DA, Wasilewski CE, Boyan BD, Schwartz Z: Mediation of osteogenic differentiation of human mesenchymal stem cells on titanium surfaces by a Wnt-integrin feedback loop. Biomaterials. 2011, 32: 6399-6411. 10.1016/j.biomaterials.2011.05.036.
Hurst-Kennedy J, Zhong M, Gupta V, Boyan BD, Schwartz Z: 24R,25-Dihydroxyvitamin D3, lysophosphatidic acid, and p53: a signaling axis in the inhibition of phosphate-induced chondrocyte apoptosis. J Steroid Biochem Mol Biol. 2010, 122: 264-271. 10.1016/j.jsbmb.2010.05.010.
Schwartz Z, Schlader DL, Ramirez V, Kennedy MB, Boyan BD: Effects of vitamin D metabolites on collagen production and cell proliferation of growth zone and resting zone cartilage cells in vitro. J Bone Miner Res. 1989, 4: 199-207.
Nasatzky E, Schwartz Z, Boyan BD, Soskolne WA, Ornoy A: Sex-dependent effects of 17-beta-estradiol on chondrocyte differentiation in culture. J Cell Physiol. 1993, 154: 359-367. 10.1002/jcp.1041540220.
O'Keefe RJ, Puzas JE, Brand JS, Rosier RN: Effects of transforming growth factor-beta on matrix synthesis by chick growth plate chondrocytes. Endocrinology. 1988, 122: 2953-2961. 10.1210/endo-122-6-2953.
Schwartz Z, Sylvia VL, Dean DD, Boyan BD: The synergistic effects of vitamin D metabolites and transforming growth factor-beta on costochondral chondrocytes are mediated by increases in protein kinase C activity involving two separate pathways. Endocrinology. 1998, 139: 534-545. 10.1210/en.139.2.534.
Raines AL, Olivares-Navarrete R, Wieland M, Cochran DL, Schwartz Z, Boyan BD: Regulation of angiogenesis during osseointegration by titanium surface microstructure and energy. Biomaterials. 2010, 31: 4909-4917. 10.1016/j.biomaterials.2010.02.071.
Fiedler J, Leucht F, Waltenberger J, Dehio C, Brenner RE: VEGF-A and PlGF-1 stimulate chemotactic migration of human mesenchymal progenitor cells. Biochem Biophys Res Commun. 2005, 334: 561-568. 10.1016/j.bbrc.2005.06.116.
Moyer HR, Wang Y, Farooque T, Wick T, Singh KA, Xie L, Guldberg RE, Williams JK, Boyan BD, Schwartz Z: A new animal model for assessing cartilage repair and regeneration at a nonarticular site. Tissue Eng Part A. 2010, 16: 2321-2330. 10.1089/ten.tea.2009.0245.
Palmer AW, Guldberg RE, Levenston ME: Analysis of cartilage matrix fixed charge density and three-dimensional morphology via contrast-enhanced microcomputed tomography. Proc Natl Acad Sci USA. 2006, 103: 19255-19260. 10.1073/pnas.0606406103.
Lee EY, Xia Y, Kim WS, Kim MH, Kim TH, Kim KJ, Park BS, Sung JH: Hypoxia-enhanced wound-healing function of adipose-derived stem cells: increase in stem cell proliferation and up-regulation of VEGF and bFGF. Wound Repair Regen. 2009, 17: 540-547. 10.1111/j.1524-475X.2009.00499.x.
Spaeth E, Klopp A, Dembinski J, Andreeff M, Marini F: Inflammation and tumor microenvironments: defining the migratory itinerary of mesenchymal stem cells. Gene Ther. 2008, 15: 730-738. 10.1038/gt.2008.39.
Sharp FR, Ran R, Lu A, Tang Y, Strauss KI, Glass T, Ardizzone T, Bernaudin M: Hypoxic preconditioning protects against ischemic brain injury. NeuroRx. 2004, 1: 26-35. 10.1602/neurorx.1.1.26.
Demol J, Lambrechts D, Geris L, Schrooten J, Van Oosterwyck H: Towards a quantitative understanding of oxygen tension and cell density evolution in fibrin hydrogels. Biomaterials. 2011, 32: 107-118. 10.1016/j.biomaterials.2010.08.093.
Polacek M, Bruun JA, Elvenes J, Figenschau Y, Martinez I: The secretory profiles of cultured human articular chondrocytes and mesenchymal stem cells: implications for autologous cell transplantation strategies. Cell Transplant. 2010, 20: 1381-1383.
Rehman J, Traktuev D, Li J, Merfeld-Clauss S, Temm-Grove CJ, Bovenkerk JE, Pell CL, Johnstone BH, Considine RV, March KL: Secretion of angiogenic and antiapoptotic factors by human adipose stromal cells. Circulation. 2004, 109: 1292-1298. 10.1161/01.CIR.0000121425.42966.F1.
Rubina K, Kalinina N, Efimenko A, Lopatina T, Melikhova V, Tsokolaeva Z, Sysoeva V, Tkachuk V, Parfyonova Y: Adipose stromal cells stimulate angiogenesis via promoting progenitor cell differentiation, secretion of angiogenic factors, and enhancing vessel maturation. Tissue Eng Part A. 2009, 15: 2039-2050. 10.1089/ten.tea.2008.0359.
Robinson CJ, Stringer SE: The splice variants of vascular endothelial growth factor (VEGF) and their receptors. J Cell Sci. 2001, 114: 853-865.
Connolly DT, Heuvelman DM, Nelson R, Olander JV, Eppley BL, Delfino JJ, Siegel NR, Leimgruber RM, Feder J: Tumor vascular permeability factor stimulates endothelial cell growth and angiogenesis. J Clin Invest. 1989, 84: 1470-1478. 10.1172/JCI114322.
Pufe T, Harde V, Petersen W, Goldring MB, Tillmann B, Mentlein R: Vascular endothelial growth factor (VEGF) induces matrix metalloproteinase expression in immortalized chondrocytes. J Pathol. 2004, 202: 367-374. 10.1002/path.1527.
Kilroy GE, Foster SJ, Wu X, Ruiz J, Sherwood S, Heifetz A, Ludlow JW, Stricker DM, Potiny S, Green P, Halvorsen YD, Cheatham B, Storms RW, Gimble JM: Cytokine profile of human adipose-derived stem cells: expression of angiogenic, hematopoietic, and pro-inflammatory factors. J Cell Physiol. 2007, 212: 702-709. 10.1002/jcp.21068.
Schweigerer L, Neufeld G, Friedman J, Abraham JA, Fiddes JC, Gospodarowicz D: Capillary endothelial cells express basic fibroblast growth factor, a mitogen that promotes their own growth. Nature. 1987, 325: 257-259. 10.1038/325257a0.
Deckers MM, Karperien M, van der Bent C, Yamashita T, Papapoulos SE, Lowik CW: Expression of vascular endothelial growth factors and their receptors during osteoblast differentiation. Endocrinology. 2000, 141: 1667-1674. 10.1210/en.141.5.1667.
Kim JH, Lee MC, Seong SC, Park KH, Lee S: Enhanced proliferation and chondrogenic differentiation of human synovium-derived stem cells expanded with basic fibroblast growth factor. Tissue Eng Part A. 2011, 17: 991-1002. 10.1089/ten.tea.2010.0277.
Perrier E, Ronziere MC, Bareille R, Pinzano A, Mallein-Gerin F, Freyria AM: Analysis of collagen expression during chondrogenic induction of human bone marrow mesenchymal stem cells. Biotechnol Lett. 2011, 33: 2091-2101. 10.1007/s10529-011-0653-1.
Nishizawa K, Imai S, Mimura T, Kubo M, Araki S, Shioji S, Takemura Y, Matsusue Y: In-advance trans-medullary stimulation of bone marrow enhances spontaneous repair of full-thickness articular cartilage defects in rabbits. Cell Tissue Res. 2010, 341: 371-379. 10.1007/s00441-010-1020-6.
Argun M, Oner M, Guney A, Halici M, Temizyurek O, Canoz O: The healing of full-thickness articular cartilage defects in rabbits: successful results with fibroblast growth factor. Eklem Hastalik Cerrahisi. 2010, 21: 147-152.
Hashimoto S, Creighton-Achermann L, Takahashi K, Amiel D, Coutts RD, Lotz M: Development and regulation of osteophyte formation during experimental osteoarthritis. Osteoarthritis Cartilage. 2002, 10: 180-187. 10.1053/joca.2001.0505.
Pfander D, Kortje D, Zimmermann R, Weseloh G, Kirsch T, Gesslein M, Cramer T, Swoboda B: Vascular endothelial growth factor in articular cartilage of healthy and osteoarthritic human knee joints. Ann Rheum Dis. 2001, 60: 1070-1073. 10.1136/ard.60.11.1070.
Enomoto H, Inoki I, Komiya K, Shiomi T, Ikeda E, Obata K, Matsumoto H, Toyama Y, Okada Y: Vascular endothelial growth factor isoforms and their receptors are expressed in human osteoarthritic cartilage. Am J Pathol. 2003, 162: 171-181. 10.1016/S0002-9440(10)63808-4.
Matsumoto T, Cooper GM, Gharaibeh B, Meszaros LB, Li G, Usas A, Fu FH, Huard J: Cartilage repair in a rat model of osteoarthritis through intraarticular transplantation of muscle-derived stem cells expressing bone morphogenetic protein 4 and soluble Flt-1. Arthritis Rheum. 2009, 60: 1390-1405. 10.1002/art.24443.
Kubo S, Cooper GM, Matsumoto T, Phillippi JA, Corsi KA, Usas A, Li G, Fu FH, Huard J: Blocking vascular endothelial growth factor with soluble Flt-1 improves the chondrogenic potential of mouse skeletal muscle-derived stem cells. Arthritis Rheum. 2009, 60: 155-165. 10.1002/art.24153.
Maes C, Stockmans I, Moermans K, Van Looveren R, Smets N, Carmeliet P, Bouillon R, Carmeliet G: Soluble VEGF isoforms are essential for establishing epiphyseal vascularization and regulating chondrocyte development and survival. J Clin Invest. 2004, 113: 188-199.
Gerber HP, Vu TH, Ryan AM, Kowalski J, Werb Z, Ferrara N: VEGF couples hypertrophic cartilage remodeling, ossification and angiogenesis during endochondral bone formation. Nat Med. 1999, 5: 623-628. 10.1038/9467.
Goldring MB, Tsuchimochi K, Ijiri K: The control of chondrogenesis. J Cell Biochem. 2006, 97: 33-44. 10.1002/jcb.20652.
Ahmed N, Dreier R, Gopferich A, Grifka J, Grassel S: Soluble signalling factors derived from differentiated cartilage tissue affect chondrogenic differentiation of rat adult marrow stromal cells. Cell Physiol Biochem. 2007, 20: 665-678.
Fischer J, Dickhut A, Rickert M, Richter W: Human articular chondrocytes secrete parathyroid hormone-related protein and inhibit hypertrophy of mesenchymal stem cells in coculture during chondrogenesis. Arthritis Rheum. 2010, 62: 2696-2706. 10.1002/art.27565.
Bian L, Zhai DY, Mauck RL, Burdick JA: Coculture of human mesenchymal stem cells and articular chondrocytes reduces hypertrophy and enhances functional properties of engineered cartilage. Tissue Eng Part A. 2011, 17: 1137-1145. 10.1089/ten.tea.2010.0531.
Hildner F, Concaro S, Peterbauer A, Wolbank S, Danzer M, Lindahl A, Gatenholm P, Redl H, van Griensven M: Human adipose-derived stem cells contribute to chondrogenesis in coculture with human articular chondrocytes. Tissue Eng Part A. 2009, 15: 3961-3969. 10.1089/ten.tea.2009.0002.
Diekman BO, Rowland CR, Lennon DP, Caplan AI, Guilak F: Chondrogenesis of adult stem cells from adipose tissue and bone marrow: induction by growth factors and cartilage-derived matrix. Tissue Eng Part A. 2010, 16: 523-533.
Kavalkovich KW, Boynton RE, Murphy JM, Barry F: Chondrogenic differentiation of human mesenchymal stem cells within an alginate layer culture system. In Vitro Cell Dev Biol Anim. 2002, 38: 457-466. 10.1290/1071-2690(2002)038<0457:CDOHMS>2.0.CO;2.
The authors thank Sri Vermula for her assistance with cell culture and Sha'Aqua Ashbury and Elyse A Watkins for their assistance with histology. The authors also thank Dr Andrew Raines, Sharon Hyzy, and Christopher Erdman for their assistance with surgeries and radiographic imaging. Finally, the authors thank Angela Lin and Dr Robert Guldberg for their help in preparing an EPIC-μCT evaluation script to assess cartilage formation in the xiphoid defect. This study was supported by an NSF Graduate Research Fellowship (Lee) and grants from the Department of Defense (W81XWH-11-1-0306) and Children's Healthcare of Atlanta. These funding sources had no involvement in the study design, collection, analysis, or interpretation of data; in the writing of the manuscript; or in the decision to submit the manuscript for publication.
CSD Lee, BD Boyan, and Z Schwartz are co-inventors of the cell culture and microbead technologies described in this research, which is licensed to SpherIngenics, Inc. BD Boyan and Z Schwartz are co-founders and own stock in SpherIngenics, Inc. OA Burnsed, V Raghuram, and J Kalisvaart have no competing interests.
All authors have read and approved the manuscript for publication. Authors have contributed to the conception and design (CSDL, BDB, ZS), collection and assembly of data (CSDL, OAB, VR, JK), data analysis and interpretation (CSDL, OAB, VR, JK), writing (CSDL, ZS), editing (CSDL, BDB), financial and administrative support (BDB), and final approval (BDB, ZS) associated with this manuscript.
Authors’ original submitted files for images
About this article
Cite this article
Lee, C.S., Burnsed, O.A., Raghuram, V. et al. Adipose stem cells can secrete angiogenic factors that inhibit hyaline cartilage regeneration. Stem Cell Res Ther 3, 35 (2012) doi:10.1186/scrt126
- Cartilage Regeneration
- Cartilage Volume
- Chondrocyte Proliferation
- Chondrocyte Apoptosis
- Chondrogenic Medium