CD90 serves as differential modulator of subcutaneous and visceral adipose-derived stem cells by regulating AKT activation that influences adipose tissue and metabolic homeostasis
Stem Cell Research & Therapy volume 10, Article number: 355 (2019)
White adipose tissue includes subcutaneous and visceral adipose tissue (SAT and VAT) with different metabolic features. SAT protects from metabolic disorders, while VAT promotes them. The proliferative and adipogenic potentials of adipose-derived stem cells (ADSCs) are critical for maintaining adipose tissue homeostasis through driving adipocyte hyperplasia and inhibiting pathological hypertrophy. However, it remains to be elucidated the critical molecules that regulate different potentials of subcutaneous and visceral ADSCs (S-ADSCs, V-ADSCs) and mediate distinct metabolic properties of SAT and VAT. CD90 is a glycosylphosphatidylinositol-anchored protein on various cells, which is also expressed on ADSCs. However, its expression patterns and differential regulation on S-ADSCs and V-ADSCs remain unclear.
S-ADSCs and V-ADSCs were detected for CD90 expression. Proliferation, colony formation, cell cycle, mitotic clonal expansion, and adipogenic differentiation were assayed in S-ADSCs, V-ADSCs, or CD90-silenced S-ADSCs. Glucose tolerance test and adipocyte hypertrophy were examined in mice after silencing of CD90 in SAT. CD90 expression and its association with CyclinD1 and Leptin were analyzed in adipose tissue from mice and humans. Regulation of AKT by CD90 was detected using a co-transfection system.
Compared with V-ADSCs, S-ADSCs expressed high level of CD90 and showed increases in proliferation, mitotic clonal expansion, and adipogenic differentiation, together with AKT activation and G1-S phase transition. CD90 silencing inhibited AKT activation and S phase entry, thereby curbing proliferation and mitotic clonal expansion of S-ADSCs. In vivo CD90 silencing in SAT inhibited S-ADSC proliferation, which caused adipocyte hypertrophy and glucose intolerance in mice. Furthermore, CD90 was highly expressed in SAT rather than in VAT in human and mouse, which had positive correlation with CyclinD1 but negative correlation with Leptin. CD90 promoted AKT activation through recruiting its pleckstrin homology domain to plasma membrane.
CD90 is differentially expressed on S-ADSCs and V-ADSCs, and plays critical roles in ADSC proliferation, mitotic clonal expansion, and hemostasis of adipose tissue and metabolism. These findings identify CD90 as a crucial modulator of S-ADSCs and V-ADSCs to mediate distinct metabolic features of SAT and VAT, thus proposing CD90 as a valuable biomarker or target for evaluating ADSC potentials, monitoring or treating obesity-associated metabolic disorders.
Excess fat accumulation in adipose tissue causes obesity, which increases the risks of diabetes, steatohepatitis, stroke, cardiovascular disease, or even cancer [1, 2]. White adipose tissue (WAT) including subcutaneous and visceral adipose tissue (SAT and VAT) stores surplus energy to regulate metabolic balance. Both SAT and VAT expand during adiposity but with distinct metabolic functions. The accumulation of VAT is associated with metabolic disorders including insulin resistance, diabetes mellitus, hypertension, dyslipidemia, and atherosclerosis, while SAT improves insulin action and metabolism [3,4,5]. Studies from humans and animal models provided evidences for the protective effects of SAT but adverse effects of VAT on metabolism. Removal of visceral fat in aging rats or omentectomy in obese subjects improved their metabolic profiles, while transplantation of subcutaneous fat into intra-abdominal site decreased body weight and fat mass, and improved insulin sensitivity in recipient mice [6,7,8].
WAT expands via adipocyte hyperplasia and hypertrophy, characterized by increases in number of new adipocytes or size of existing adipocytes, respectively [9,10,11,12]. Adipocyte hyperplasia indicates de novo adipogenesis from progenitors in response to metabolic demands. It has been demonstrated that hyperplasic expansion of SAT protected the mice against obesity-induced insulin resistance, whereas loss of hyperplasic potential caused pathological hypertrophic expansion of SAT that led to adipose tissue dysfunction, inflammation, and systemic insulin resistance in animals and humans [10, 13,14,15]. A recent study also substantiated that de novo adipocyte differentiation protected against pathologic visceral adipose expansion in obesity and resulted in improvements in glucose homeostasis , suggesting the beneficial roles of adipocyte hyperplasia in WAT and metabolic homeostasis. Currently, there are still some controversy over de novo adipogenesis in SAT and VAT . Joe and colleagues concluded that SAT expanded mostly by hyperplasia, whereas VAT by hypertrophy, as SAT had more proliferating adipogenic progenitors than VAT in mice fed on high-fat diet . Conversely, another study showed that VAT had higher capacity of adipogenesis by hyperplasia than SAT in response to high-fat diet feeding using an in vivo adipogenesis tracking mouse model, though the stromal vascular fraction (SVF) from SAT was easier to differentiate into adipocytes in vitro than that from VAT . In addition, Macotela et al. reported that CD34- and SCA1-positive adipocyte precursor cells from SAT had higher capacity for adipogenic differentiation in vitro than those from VAT in mice . So, the balance between adipocyte hyperplasia and hypertrophy in SAT and VAT especially related regulatory mechanisms remains to be clarified.
Adipose-derived stem cells (ADSCs) expressing mesenchymal stem cell (MSC) markers like CD44, CD105, CD90, and CD73 are the main progenitors in WAT, which can differentiate into multiple cell types in vitro including adipocytes, osteoblasts, and chondrocytes. Due to their capacities for self-renewal and multipotent differentiation, ADSCs play pivotal roles in supporting WAT homeostasis under pathophysiological conditions and have broad prospects in tissue repair and regeneration [21,22,23,24,25]. ADSCs are essential progenitors for adipocyte hyperplasia, which links cell proliferation with differentiation during adipogenic differentiation . In the initial phase of adipogenesis, growth-arrested preadipocytes (ADSCs committed to adipocyte lineage) reenter cell cycle to undergo several rounds of cell division, known as mitotic clonal expansion, which is a prerequisite for adipogenic differentiation [12, 26,27,28]. Reagents blocking cell cycle reentry or proliferation significantly impaired adipocyte differentiation through inhibiting clonal expansion [12, 29, 30], confirming the proliferative potential of ADSCs in determining adipogenic differentiation. Considering the differences between SAT and VAT, key molecules and mechanisms for regulating the proliferative potentials and differences between subcutaneous and visceral ADSCs (S-ADSCs, V-ADSCs) require to be clarified.
CD90, also known as Thy-1, is a typical glycosylphosphatidylinositol (GPI)-anchored protein, which functions differently in various cells including regulating cell proliferation, apoptosis, survival, adhesion, and migration [31,32,33,34]. The effects of CD90 on cell proliferation have been studied in several types of tumor cells, fibroblasts, and hematopoietic stem cells, which either promotes or inhibits proliferation depending on different cell types in various contexts [32, 33, 35,36,37]. Several studies also showed the differential impacts of CD90 on differentiation of MSCs based on their different species or tissue sources [38,39,40]. As one of the MSC markers, CD90 is also expressed on ADSCs, but its expression patterns and differential impacts on S-ADSCs and V-ADSCs remain unclear. A recent study showed an important role of CD90 in AKT activation in human cytomegalovirus-infected cells . AKT activation is involved in the survival or proliferation of various cells and can promote the proliferation of human and mice ADSCs by upregulating cell cycle protein CyclinD1 [42,43,44,45,46]. However, it remains largely unknown whether CD90 regulates ADSC potentials via AKT and whether CD90 produces different impacts on S-ADSCs and V-ADSCs to influence adipose tissue and metabolic homeostasis. In the present study, we demonstrated that CD90 had different expression profiles on S-ADSCs and V-ADSCs, which differentially regulated proliferation and mitotic clonal expansion of S-ADSCs and V-ADSCs through modulating AKT activation, thereby producing distinct impacts on WAT homeostasis and metabolism. This study proposes CD90 as a critical target for regulating ADSCs, which has potential prospects in therapy for obesity-associated metabolic disorders.
C57BL/6 male mice were provided by Vital River Laboratory Animal Technology Co. Ltd. (Beijing, China). All animal studies were approved by the Ethical Committee of Qilu Hospital of Shandong University, and all experimental procedures were performed in accordance with the institutional guidelines for animal care and utilization.
Isolation and culture of ADSCs
S-ADSCs and V-ADSCs were isolated from inguinal and epididymal WAT of C57BL/6 male mice at the age of 10–12 weeks. Briefly, fat pads were digested with 2 mg/mL collagenase (Worthington, Lakewood, NJ) in Krebs-Ringer Bicarbonate buffer at 37 °C for about 50 min. The SVF passed through a 100-μm filter was incubated overnight in complete Dulbecco’s modified Eagle’s medium (DMEM) containing 10% fetal bovine serum (Invitrogen, Carlsbad, CA) and 5 ng/mL basic fibroblast growth factor (Peprotech, Rocky Hill, NJ). After removal of non-adherent cells, the adherent cells were cultured as ADSCs. The third to fifth passages were used for the experiments.
Assay for proliferation, mitotic clonal expansion, colony formation, and cell cycle
The growth curve of ADSCs was examined using Cell Counting Kit (CCK)-8 (Dojindo, Tokyo, Japan), and optical density (OD) value was measured at 450 nm to evaluate viability of the cells. For EdU incorporation assay, ADSCs were cultured in 96-well plates at 37 °C, 5%CO2 overnight, and then were incubated with EdU (10 μM) for additional 6 h before harvest. EdU incorporation was detected by Cell-Light EdU Apollo567 Cell Tracking Kit (RiboBio, Guangzhou, China) according to the manufacturer’s instruction. Mitotic clonal expansion was examined in ADSCs subjected to 16 h of adipogenic induction by EdU incorporation assay. For colony formation assay, ADSCs were cultured in 6-well plates at 37 °C, 5% CO2 for 7 days, and then were stained with crystal violet for colony counting after fixed with 100% methanol. For cell cycle assay, ADSCs were fixed with ice-cold 70% ethanol at 4 °C overnight and then incubated with propidium iodide (PI) at 4 °C for 30 min. The cells were acquired and analyzed with Cytomics FC500 (Beckman Coulter, Pasadena, CA). In some experiments, S-ADSCs were transfected with CD90 siRNA (siCD90, Sigma-Aldrich, San Francisco, CA) using Jet-PRIME (Polyplus, Berkeley, CA) and then used for the above assays. The sequences of siCD90 were listed (Additional file 1: Table S1).
ADSCs were cultured to over confluence and further induced using adipogenic differentiation medium (Cyagen Biosciences, Guangzhou, China) according to the manufacturer’s instruction. The adipogenic differentiation was evaluated by Oil Red O staining (Sigma-Aldrich) after 18 days of induction, and OD value was measured at 500 nm after eluting Oil Red O with 100% isopropanol. In some experiments, S-ADSCs infected with shRNA CD90 (shCD90) or control shRNA (shControl) recombinant lentivirus (GenePharma, shanghai, China) were subjected to adipogenic induction. The sequences of shCD90 were listed (Additional file 1: Table S1).
ADSCs were incubated with Fc block and then stained with fluorescein isothiocyanate (FITC)-labeled antibody (Ab) against mouse CD90 (clone: 30-H12), phycoerythrin (PE)-labeled Ab against mouse CD105 (clone: MU7/18), and PE-cyanine5 (PE-cy5)-labeled Ab against mouse CD44 (clone: IM7) (eBioscience, San Diego, CA). The cells were acquired using CytoFLEX S, and data were analyzed by CytExpert (Beckman Coulter).
In vivo lentiviral infection
Male mice at the age of 8 weeks were anesthetized, and the bilateral inguinal fat pads were exposed and injected with shCD90 or shControl lentivirus (Genechem, Shanghai, China) (Additional file 1: Table S1). The mice were maintained under standard conditions after surgery, and glucose tolerance test (GTT) was conducted 3 weeks later. Briefly, mice were fasted overnight and blood glucose levels were determined at different time points after intraperitoneal injection of glucose (2 g/kg body weight, Sigma-Aldrich). Four weeks later, inguinal adipose tissue was collected from the mice. The average sizes of adipocytes were measured in adipose tissue section after hematoxylin and eosin (H&E) staining using Image-Pro Plus 6.0. ADSCs isolated from inguinal adipose tissue were examined for CD90 expression and proliferative potential.
CD90 expression and its correlation with CyclinD1 and Leptin were analyzed in mice and human adipose tissue using GEO databases. The following databases were included in the study: (1) gene expression profiles of inguinal and axillary SAT, and epididymal and mesenteric VAT from age-matched C57BL/6 male mice fed on normal diet (GSE53307); (2) gene expression profiles of epididymal and mesenteric VAT from C57BL/6 mice fed on normal or high-fat diet for 2, 4, 8, 20, and 24 weeks (GSE39549); (3) gene expression of epididymal VAT including adipocyte and stromal vascular cell (SVC) fractions from male C57BL/6 mice fed on normal or high-fat diet for 0, 3, and 7 days (GSE65557); (4) gene expression of abdominal SAT from subjects (body mass index, BMI, 16.7–50.2) with normal or impaired glucose tolerance, or type 2 diabetes (GSE27951); (5) gene expression of SAT and omental VAT from BMI-matched, morbidly obese patients who were insulin sensitive or resistant (GSE15773); and (6) gene expression of SAT and omental VAT from BMI-matched, obese patients who were insulin sensitive or resistant (GSE20950).
Plasmid transfection and immunofluorescence
Plasmids carrying genes encoding human active pleckstrin homology (PH) domain of AKT (pcDNA3-AKT-PH-GFP) or mutant AKT-PH domain (pcDNA3-AKT-PHR25C-GFP) were kindly provided by Dr. Craig Montell from Johns Hopkins University via addgene (Cambridge, MA) . Plasmids pENTER (Mock) and pENTER-THY1(CD90)-Flag were purchased from ViGene BioScieneces (Jinan, China). HEK-293T cells planted in 24-well chamber slides were co-transfected with pcDNA3-AKT-PH-GFP (or pcDNA3-AKT-PHR25C-GFP) and pENTER-CD90-Flag (or Mock) for 24 h. After fixed in 4% paraformaldehyde for 30 min and blocked with 5% bovine serum albumin (BSA) for 1 h, the cells were incubated with anti-Flag (DDDDK) Ab (MBL, Woburn, MA) at 4 °C overnight, followed by incubation with Alexa Fluor 594-conjucted secondary Ab (Proteintech Group, Chicago, IL) at 37 °C for 1 h. The nuclei were stained with 4,6-diamidino-2-phenylindole (Beyotime Biotechnology, Shanghai, China). Fluorescent signals were analyzed with laser scanning confocal microscope (Zeiss, Jena, Germany).
Total RNA was extracted from cells or tissues using RNAfast200 (Fastagen, Shanghai, China) or Trizol (TIANGEN BIOTECH, Beijing, China), and reversely transcripted into cDNA with ReverTra Ace qPCR RT Kit (TOYOBO Life Science, Shanghai, China). qPCR was carried out using SYBR Green Master Mix (CWbiotech, Beijing, China). The relative mRNA levels of interested genes were evaluated using 2-△△Ct method, using 18 s rRNA or GAPDH as internal control. The primers were listed (Additional file 1: Table S2).
Equal amounts of proteins from cell or tissue lysates were loaded on SDS-PAGE gels. After electrophoresis, proteins were transferred to PVDF membranes. After blocked with 5% BSA for 3 h, the membranes were blotted with Abs against mouse AKT, phosphor (p)-AKT, CyclinD1 (Cell Signaling Technology, Beverly, MA), CD90 (Biolegend, San Diego, CA), GAPDH, or Tubulin (Proteintech Group) at 4 °C overnight, followed by incubation with HRP-conjugated secondary Ab (ZSGB-BIO, Beijing, China) for 1 h. The signals were detected by SuperSignal West Pico Chemiluminescent Substrate (Pierce Biotechnology, Rockford, IL).
Data were expressed as mean ± SEM. Statistical differences were evaluated using Student’s t test, one- or two-way ANOVA, or non-parametric test, respectively. P < 0.05 was considered significant.
S-ADSCs show higher potential in proliferation than V-ADSCs through promoting AKT activation
The proliferation of S-ADSCs and V-ADSCs was examined by EdU incorporation assay. Compared with V-ADSCs, S-ADSCs showed significant increase in EdU-positive cells (red in nuclear indicates cells in S phase), suggesting that S-ADSCs proliferate more rapidly than V-ADSCs (Fig. 1a, b). Accordingly, S-ADSCs formed more clones than V-ADSCs in colony formation assay (Fig. 1c, d). Cell cycle profiles showed that S-ADSCs had a marked decrease in G1 phase but increase in S phase compared to V-ADSCs (Fig. 1e, f). The expression levels of stemness genes Nanog, Oct4, and Sox2 were markedly upregulated in S-ADSCs compared with those in V-ADSCs (Fig. 1g). Importantly, S-ADSCs showed significant increase in AKT phosphorylation compared with V-ADSCs, together with CyclinD1 upregulation that drives G1-S phase transition (Fig. 1h). While in the presence of AKT inhibitor MK2206, the upregulation of CyclinD1 in S-ADSCs was obviously impaired after blockade of AKT phosphorylation (Fig. 1i). These data suggest that AKT activation may contribute to effective proliferation of S-ADSCs through driving G1-S phase transition.
S-ADSCs show higher potential in adipogenic differentiation than V-ADSCs through promoting mitotic clonal expansion
Considering the differences in proliferation and stemness between S-ADSCs and V-ADSCs, the adipogenic differentiation between S-ADSCs and V-ADSCs was further compared. After 18 days of adipogenic induction, S-ADSCs were fully differentiated into adipocytes with numerous lipid droplets, while V-ADSCs showed poor ability to differentiate into adipocytes, with only a few lipid droplets in them. These observations were further confirmed by quantification of lipid contents (Fig. 2a, b). Correspondingly, the mRNA levels of white adipocyte markers PPAR-γ, C/EBPα, αP2, and Adiponectin were dramatically increased in S-ADSCs after 4, 8, or 12 days of adipogenic induction, which were significantly higher than those in differentiating V-ADSCs (Fig. 2c). These data indicate that S-ADSCs have higher adipogenic potential than V-ADSCs.
Since the initial events determining adipogenic efficiency are cell cycle reentry and mitotic clonal expansion, we further compared the mitotic clonal expansion between S-ADSCs and V-ADSCs in the early stage of adipogenic differentiation. Both S-ADSCs and V-ADSCs showed obvious growth arrest before adipogenic induction. After 16 h of adipogenic induction, EdU-positive cells were observed in both S-ADSCs and V-ADSCs. Differently, S-ADSCs had a significant increase in EdU-positive cells compared with V-ADSCs upon adipogenic induction, suggesting that S-ADSCs had higher capacity for S phase entry and mitotic clonal expansion than V-ADSCs in response to adipogenic induction (Fig. 2d, e).
CD90 is highly expressed on S-ADSCs rather than V-ADSCs
To clarify the possible reasons for differences in proliferation and mitotic clonal expansion between S-ADSCs and V-ADSCs, we examined the expression profiles of stem cell-related markers on ADSCs. As expected, both S-ADSCs and V-ADSCs positively expressed CD90, CD105, and CD44. Differently, S-ADSCs expressed higher level (both percentage and intensity) of CD90 than V-ADSCs (Fig. 3a, b), while no obvious differences were observed in CD105 expression between S-ADSCs and V-ADSCs (Fig. 3c, d); though there is a slight increase in CD44 percentage on S-ADSCs compared with V-ADSCs, both of them express high levels of CD44 (Fig. 3e, f). Consistently, high levels of CD90 mRNA and protein in S-ADSCs rather than in V-ADSCs were confirmed by qPCR and western blot (Fig. 3g, h). These findings demonstrate that S-ADSCs and V-ADSCs have different expression profiles of CD90, which may serve as an important modulator of their distinct biological behaviors.
CD90 silencing inhibits proliferation of S-ADSCs by attenuating AKT activation
To explore the roles of CD90 in proliferation of S-ADSCs, we knocked down the expression of CD90 in S-ADSCs and found marked reductions in AKT phosphorylation and CyclinD1 expression (Fig. 4a, b). Different from the rapid response on AKT phosphorylation in the control group, insulin failed to induce the increase of AKT phosphorylation in CD90-silenced S-ADSCs, confirming that CD90 exerts an indispensable role in AKT activation in S-ADSCs (Additional file 1: Figure S1). Accordingly, CD90 silencing caused significant G1 phase arrest together with S phase inhibition in S-ADSCs (Fig. 4c, d). Consequently, CD90-silenced S-ADSCs showed obviously reduced proliferation as suggested by decreases in growth curve and EdU-positive cells (Fig. 4e–g). Consistently, significant decreases in the mRNA levels of Nanog, Oct4, and Sox2 were observed in CD90-silenced S-ADSCs (Fig. 4h). These findings indicate that CD90 promotes ADSC proliferation and stemness through activating AKT pathway and driving CyclinD1-mediated G1-S phase transition.
CD90 silencing inhibits mitotic clonal expansion of S-ADSCs that influences adipocyte differentiation
Next, S-ADSCs were efficiently infected with GFP-tagged shCD90 or shControl lentivirus (Additional file 1: Figure S2). Compared with shControl, shCD90 led to a marked reduction in CD90 expression in S-ADSCs (Fig. 5a). Although adipogenic induction caused increase of EdU-positive cells in both shControl- and shCD90-treated S-ADSCs, there were much less EdU-positive cells in shCD90-treated S-ADSCs than those in shControl-treated S-ADSCs, indicating that CD90 silencing obviously inhibits mitotic clonal expansion and cell division of S-ADSCs during the early phase of adipogenic differentiation (Fig. 5b, c). Accordingly, after 18 days of adipogenic induction, shCD90-treated S-ADSCs showed obvious reduction in lipid droplets compared with shControl-treated S-ADSCs, which was verified by quantification of lipid contents (Fig. 5d, e). Meanwhile, shCD90 markedly inhibited the mRNA levels of white adipocyte markers PPAR-γ, C/EBPα, αP2, and Adiponectin in differentiating S-ADSCs (Fig. 5f). These findings suggest that CD90 promotes the mitotic clonal expansion of S-ADSCs, thereby facilitating their adipogenic differentiation.
CD90 silencing causes glucose intolerance and adipocyte hypertrophy in mice
To evaluate the influence of CD90 on WAT and systemic metabolism, we knocked down CD90 in inguinal SAT of the mice using recombinant lentivirus. After determining the efficiencies of lentiviral infection and CD90 silencing by shCD90 in S-ADSCs in vitro (Fig. 6a, b), the efficiency of lentiviral infection was examined in vivo. The results showed that GFP signals were clearly observed in inguinal S-ADSCs from the mice 2 weeks after injection with lentivirus, which lasted until 4 weeks (Fig. 6c). Compared with control mice, shCD90-treated mice showed no significant alterations in body weight and WAT weight till the end of the experiment (Fig. 6d and Additional file 1: Figure S3). However, shCD90 treatment led to a significant glucose intolerance in mice, as evidenced by difficulty in decreasing glucose levels at 30, 45, and 60 min after glucose injection and elevation in area under the curve during GTT (Fig. 6e, f). Importantly, shCD90-treated mice showed a marked increase in adipocyte size in SAT compared with shControl-treated mice (Fig. 6g, h). The mRNA level of Leptin, which has been proved to be positively correlated with adipocyte size , was also elevated in this fat depot from shCD90-treated mice (Fig. 6i). As expected, S-ADSCs from shCD90-treated mice, which had reduced expression of CD90, showed significant decrease in proliferation compared with those from shControl-treated mice (Fig. 6j–l). These data suggest that CD90 silencing in SAT results in adipocyte hypertrophy and glucose intolerance in mice through suppressing ADSC proliferation.
CD90 is positively correlated with CyclinD1 but negatively with Leptin in mouse and human WAT
To further verify the effects of CD90 on WAT homeostasis, we analyzed the mRNA level of CD90 in mouse and human WAT using GEO database. In mice fed on normal diet, CD90 was highly expressed in inguinal SAT compared with that in epididymal VAT, which was consistent with the expression profiles on S-ADSCs and V-ADSCs. CD90 expression was positively correlated to proliferation-related CyclinD1 expression, but negatively correlated to adipocyte hypertrophy-related Leptin expression in WAT (inguinal, axillary SAT and epididymal, mesenteric VAT) from these mice (Fig. 7a–c and Additional file 1: Figure S4A–C). A highly positive correlation of CD90 with CyclinD1 but a negative correlation with Leptin were also observed in epididymal and mesenteric VAT from mice fed on normal or high-fat diet for different time periods (Fig. 7d, e). Similarly, the correlations of CD90 with CyclinD1 or Leptin were found in epididymal VAT (adipocytes and SVCs) from mice fed on short term of normal or high-fat diet (Fig. 7f, g and Additional file 1: Figure S4D, E). It should be noted that CD90 is highly expressed on SVCs that contained amounts of ADSCs, rather than on adipocytes (Fig. 7h). CD90 on SVCs but not on adipocytes had a positive correlation with CyclinD1 (Fig. 7i, j), indicating the predominant expression of CD90 on ADSCs is the primary contributor to CyclinD1 regulation and WAT homeostasis.
In human subjects with normal or impaired glucose tolerance, or type 2 diabetes, CD90 expression in abdominal SAT was positively correlated with CyclinD1 expression, as well as the BMI of the subjects (Fig. 7k, l). The positive correlation of CD90 with CyclinD1 was also found in WAT (SAT and omental VAT) from obese patients with insulin sensitivity or resistance (Fig. 7m). In particular, results from obese patients who were insulin sensitive or resistant showed that CD90 was highly expressed in SAT compared with that in omental VAT, which was positively correlated to CyclinD1 expression (Fig. 7n, o and Additional file 1: Figure S4F). Especially in insulin-resistant obese patients, CD90 expression had a tightly negative correlation with Leptin expression in VAT (Fig. 7p). These observations from human WAT further confirmed the positive regulation of CD90 on CyclinD1 and WAT homeostasis.
CD90 recruits AKT-PH domain to plasma membrane to promote AKT activation
The initial activation of AKT requires binding lipid messengers on plasma membrane with its active PH domain [47, 49, 50]. To clarify how CD90 regulated AKT activation, HEK-293T cells were co-transfected with pcDNA3-AKT-PH-GFP (or pcDNA3-AKT-PHR25C-GFP) and pENTER-CD90-Flag (or Mock), and the translocation of AKT-PH domain was detected. As shown in Fig. 8a, AKT-PHR25C-GFP was retained inside the cells and had no translocation to plasma membrane in either the presence or the absence of exogenous CD90-Flag, indicating that mutant AKT-PHR25C domain loses the ability to bind to plasma membrane. A small amount of AKT-PH-GFP had a translocation to plasma membrane in the absence of exogenous CD90-Flag, indicating the basal level of endogenous CD90 may recruit AKT-PH domain in HEK-293T cells. Importantly, enhanced expression of CD90-Flag caused an obvious accumulation of AKT-PH-GFP in a raft-like structure, which had an apparent colocalization with CD90-Flag on plasma membrane, while AKT-PH-GFP inside the cells was accordingly reduced. Consistent with these observations, the overexpression of CD90 in ADSCs caused significant increases in AKT phosphorylation and CyclinD1 expression, which were obviously inhibited by MK2206 (Additional file 1: Figure S5). Thus, the overexpression of CD90 caused an obvious translocation of AKT-PH domain to plasma membrane, suggesting that CD90 promotes AKT activation by recruiting its PH domain to plasma membrane.
ADSCs play important roles in maintaining WAT homeostasis. The differences between S-ADSCs and V-ADSCs may influence the balance of hyperplasia and hypertrophy of adipocytes, which contributes to different metabolic profiles between SAT and VAT. In this study, we showed that S-ADSCs had higher proliferative potential than V-ADSCs, supported by increased expression of stemness genes Nanog, Oct4, and Sox2. Compared with V-ADSCs, S-ADSCs showed marked increases in AKT activation, CyclinD1 expression, and G1-S phase transition. Consistent with previous studies showing the critical role of AKT activation in promoting proliferation of cancer cells and ADSCs [45, 46, 51], we demonstrated that AKT activation in S-ADSCs may promote their proliferation via S phase entry driven by CyclinD1, thereby facilitating their self-renewal in SAT. Although there is still controversy over adipogenesis of SAT and VAT [18,19,20], our findings showed that S-ADSCs had higher efficiency in adipogenesis than V-ADSCs, indicating that S-ADSCs are more prone to adipocyte hyperplasia than V-ADSCs. Several recent studies showed that adipocyte differentiation was influenced by regulating mitotic clonal expansion, substantiating the indispensability of mitotic clonal expansion in adipogenesis [12, 26,27,28, 52, 53]. Our study provided evidences that S-ADSCs possessed high potential in mitotic clonal expansion, which may vest them with high capacity for adipogenic differentiation. Thus, S-ADSCs may exert important roles in maintaining WAT homeostasis due to their high potential of adipocyte hyperplasia.
Previous studies have reported that CD90 promoted the proliferation of hepatocellular carcinoma cells and hematopoietic stem cells, but inhibited the proliferation of ovarian cancer cells and nasopharyngeal carcinoma cells, or even displayed opposite effects on the proliferation of fibroblasts from different tissues [31, 33, 35, 36, 54,55,56]. Our study showed that CD90 was highly expressed on S-ADSCs but moderately on V-ADSCs. CD90 on S-ADSCs is essential for AKT activation and CyclinD1 upregulation, which may promote the proliferation and stemness of S-ADSCs via G1-S phase transition, and promote the mitotic clonal expansion of S-ADSCs and their terminal adipogenic differentiation. CD90 has been identified as a cancer stem cell marker involved in tumorigenicity in several types of cancers such as hepatocellular carcinoma [57,58,59]. By contrast, our findings revealed that CD90 on ADSCs served as an AKT activator to promote ADSC potentials and functions, suggesting CD90 may play beneficial or undesirable effects depending on its expression on different tissues or cells.
The potential link between CD90 engagement and activation of PI3K/AKT pathway was reported in human cytomegalovirus-infected cells, whereas the underlying mechanisms remain to be clarified . The initiation of AKT activation requires binding to lipid messengers PtdIns(4,5)P2/PtdIns(3,4,5)P3 on plasma membrane through its active PH domain, which enables subsequent AKT phosphorylation [47, 49, 50, 60]. Our study showed the direct contribution of CD90 to AKT activation, as suggested by the translocation of AKT-PH domain from cytosol to plasma membrane caused by CD90 overexpression. Lipid rafts act as dynamic microdomains on plasma membrane and function in various membrane signaling pathways [61, 62]. Several studies have reported the critical roles of membrane raft microdomains in AKT activation [63,64,65,66]. As a GPI-anchored protein, CD90 has been verified to be incorporated into lipid raft and involved in signal transduction in various cells [62, 67, 68]. We showed that both exogenous AKT-PH domain and CD90 were exactly colocalized in a membrane raft-like structure, indicating that CD90 may act as an important trigger of membrane raft to promote the recruitment and translocation of AKT via PH domain, finally driving AKT phosphorylation and activation.
Based on its critical roles in ADSC proliferation and mitotic clonal expansion, CD90 exerts pivotal function in vivo in maintaining homeostasis of WAT and systemic metabolism. CD90 silencing in inguinal SAT led to significant glucose intolerance in mice, though no significant alterations were observed in body weight and WAT weight. The metabolic change could be attributed to attenuations in ADSC self-renewal and adipocyte hyperplasia under physiological conditions, which eventually resulted in pathological adipocyte hypertrophy and consequent metabolic disorders. On some degree, this metabolic change can partially support a previous study showing increases in body weight and serum resistin level in CD90-null mice fed on high-fat diet . However, different from the inhibitory effect of ectopic CD90 on the adipogenesis of 3T3-L1 cells, which influenced the whole process of adipogenic differentiation , we revealed an unrecognized role of CD90 in promoting mitotic clonal expansion, which influenced the early phase of adipogenic differentiation of ADSCs. Notably, although CD90 on S-ADSCs contributed to their proliferation and mitotic clonal expansion, a gradual loss of CD90 was observed during the process of adipogenic differentiation, which was consistent with the change of CD90 expression in differentiating 3T3-L1 cells [69, 70]. These data indicate that CD90 may play essential roles in maintaining the stemness of ADSCs, which determines their capacities for self-renewal and initiation of adipogenic differentiation in response to metabolic demands. After mitotic clonal expansion, the decrease of CD90 may drive the switch of ADSCs from proliferation toward terminal differentiation. Depending on the different expression levels, CD90 can differentially regulate the proliferation of S-ADSCs and V-ADSCs via AKT/CyclinD1 pathway, thus mediating distinct metabolic profiles of SAT and VAT. These findings were further supported by data from human and mouse WAT, as evidenced by the predominant expression of CD90 in SAT rather than in VAT, and its positive correlation with AKT downstream CyclinD1 but negative correlation with adipocyte hypertrophy-related Leptin. However, to validate the application potentials of CD90 in clinic, it is still necessary to expand animal or human samples in future investigations. It is also helpful to extend this study to gender differences, as both male and female have fat pads with different distributions and metabolic features. Furthermore, there was an increase of exogenous CD90 after blockade of AKT activation (Additional file 1: Figure S5), indicating a possible feedback regulation of CD90 by AKT signaling pathway in ADSCs or some influence of AKT signaling on the efficiencies of lentiviral infection or gene expression, which need to be further explored.
This study provides evidences that CD90 is highly expressed on S-ADSCs rather than on V-ADSCs, which promotes AKT activation, CyclinD1 upregulation, and G1-S phase transition, thus empowering S-ADSCs with high potentials in proliferation, mitotic clonal expansion, and adipocyte differentiation. As consequence, high level of CD90 on S-ADSCs may contribute to metabolic homeostasis via preventing adipocyte hypertrophy in SAT, while VAT is prone to mediate metabolic disorder due to a reduction of CD90 on V-ADSCs (Fig. 8b). Therefore, CD90 acts not only as a valuable biomarker for evaluating ADSC potentials or monitoring metabolic status of WAT, but also as a potential target for treating obesity-associated metabolic disorders. It should be noted that more evidences are still required to elaborate the detailed functions of CD90 in ADSCs, WAT, and metabolism as well as the underlying mechanisms.
Availability of data and materials
All data generated or analyzed during this study are included in this published article and its supplementary information files.
Subcutaneous adipose tissues
Visceral adipose tissues
Adipose-derived stem cells
White adipose tissue
Stromal vascular fraction
Mesenchymal stem cell
Dulbecco’s modified Eagle’s medium
Glucose tolerance test
Hematoxylin and eosin
Bovine serum albumin
Ogden CL, Carroll MD, Kit BK, Flegal KM. Prevalence of childhood and adult obesity in the United States, 2011-2012. JAMA. 2014;311(8):806–14.
Wang YC, McPherson K, Marsh T, Gortmaker SL, Brown M. Health and economic burden of the projected obesity trends in the USA and the UK. Lancet. 2011;378(9793):815–25.
Badimon L, Cubedo J. Adipose tissue depots and inflammation: effects on plasticity and resident mesenchymal stem cell function. Cardiovasc Res. 2017;113(9):1064–73.
Jeffery E, Wing A, Holtrup B, Sebo Z, Kaplan JL, Saavedra-Pena R, et al. The adipose tissue microenvironment regulates depot-specific adipogenesis in obesity. Cell Metab. 2016;24(1):142–50.
Gil A, Olza J, Gil-Campos M, Gomez-Llorente C, Aguilera CM. Is adipose tissue metabolically different at different sites? Int J Pediatr Obes. 2011;6(Suppl 1):13–20.
Tran TT, Yamamoto Y, Gesta S, Kahn CR. Beneficial effects of subcutaneous fat transplantation on metabolism. Cell Metab. 2008;7(5):410–20.
Thorne A, Lonnqvist F, Apelman J, Hellers G, Arner P. A pilot study of long-term effects of a novel obesity treatment: omentectomy in connection with adjustable gastric banding. Int J Obes Relat Metab Disord. 2002;26(2):193–9.
Gabriely I, Ma XH, Yang XM, Atzmon G, Rajala MW, Berg AH, et al. Removal of visceral fat prevents insulin resistance and glucose intolerance of aging: an adipokine-mediated process? Diabetes. 2002;51(10):2951–8.
Walker GE, Marzullo P, Ricotti R, Bona G, Prodam F. The pathophysiology of abdominal adipose tissue depots in health and disease. Horm Mol Biol Clin Investig. 2014;19(1):57–74.
Gustafson B, Hedjazifar S, Gogg S, Hammarstedt A, Smith U. Insulin resistance and impaired adipogenesis. Trends Endocrinol Metab. 2015;26(4):193–200.
Haczeyni F, Bell-Anderson KS, Farrell GC. Causes and mechanisms of adipocyte enlargement and adipose expansion. Obes Rev. 2018;19(3):406–20.
Fajas L. Adipogenesis: a cross-talk between cell proliferation and cell differentiation. Ann Med. 2003;35(2):79–85.
Kim JY, van de Wall E, Laplante M, Azzara A, Trujillo ME, Hofmann SM, et al. Obesity-associated improvements in metabolic profile through expansion of adipose tissue. J Clin Invest. 2007;117(9):2621–37.
Kim SM, Lun M, Wang M, Senyo SE, Guillermier C, Patwari P, et al. Loss of white adipose hyperplastic potential is associated with enhanced susceptibility to insulin resistance. Cell Metab. 2014;20(6):1049–58.
Gustafson B, Gogg S, Hedjazifar S, Jenndahl L, Hammarstedt A, Smith U. Inflammation and impaired adipogenesis in hypertrophic obesity in man. Am J Physiol Endocrinol Metab. 2009;297(5):E999–E1003.
Shao M, Vishvanath L, Busbuso NC, Hepler C, Shan B, Sharma AX, et al. De novo adipocyte differentiation from Pdgfrbeta(+) preadipocytes protects against pathologic visceral adipose expansion in obesity. Nat Commun. 2018;9(1):890.
Pellegrinelli V, Carobbio S, Vidal-Puig A. Adipose tissue plasticity: how fat depots respond differently to pathophysiological cues. Diabetologia. 2016;59(6):1075–88.
Joe AW, Yi L, Even Y, Vogl AW, Rossi FM. Depot-specific differences in adipogenic progenitor abundance and proliferative response to high-fat diet. Stem Cells. 2009;27(10):2563–70.
Wang QA, Tao C, Gupta RK, Scherer PE. Tracking adipogenesis during white adipose tissue development, expansion and regeneration. Nat Med. 2013;19(10):1338–44.
Macotela Y, Emanuelli B, Mori MA, Gesta S, Schulz TJ, Tseng YH, et al. Intrinsic differences in adipocyte precursor cells from different white fat depots. Diabetes. 2012;61(7):1691–9.
Cawthorn WP, Scheller EL, MacDougald OA. Adipose tissue stem cells meet preadipocyte commitment: going back to the future. J Lipid Res. 2012;53(2):227–46.
Park KW, Halperin DS, Tontonoz P. Before they were fat: adipocyte progenitors. Cell Metab. 2008;8(6):454–7.
Lv FJ, Tuan RS, Cheung KM, Leung VY. Concise review: the surface markers and identity of human mesenchymal stem cells. Stem Cells. 2014;32(6):1408–19.
Bateman ME, Strong AL, Gimble JM, Bunnell BA. Concise review: using fat to fight disease: a systematic review of nonhomologous adipose-derived stromal/stem cell therapies. Stem Cells. 2018;36(9):1311–28.
Czapla J, Matuszczak S, Kulik K, Wisniewska E, Pilny E, Jarosz-Biej M, et al. The effect of culture media on large-scale expansion and characteristic of adipose tissue-derived mesenchymal stromal cells. Stem Cell Res Ther. 2019;10(1):235.
Tang QQ, Lane MD. Adipogenesis: from stem cell to adipocyte. Annu Rev Biochem. 2012;81:715–36.
Tang QQ, Otto TC, Lane MD. CCAAT/enhancer-binding protein beta is required for mitotic clonal expansion during adipogenesis. Proc Natl Acad Sci U S A. 2003;100(3):850–5.
Tang QQ, Otto TC, Lane MD. Mitotic clonal expansion: a synchronous process required for adipogenesis. Proc Natl Acad Sci U S A. 2003;100(1):44–9.
Patel YM, Lane MD. Mitotic clonal expansion during preadipocyte differentiation: calpain-mediated turnover of p27. J Biol Chem. 2000;275(23):17653–60.
Yeh WC, Bierer BE, McKnight SL. Rapamycin inhibits clonal expansion and adipogenic differentiation of 3T3-L1 cells. Proc Natl Acad Sci U S A. 1995;92(24):11086–90.
Rege TA, Hagood JS. Thy-1, a versatile modulator of signaling affecting cellular adhesion, proliferation, survival, and cytokine/growth factor responses. Biochim Biophys Acta. 2006;1763(10):991–9.
Rege TA, Hagood JS. Thy-1 as a regulator of cell-cell and cell-matrix interactions in axon regeneration, apoptosis, adhesion, migration, cancer, and fibrosis. FASEB J. 2006;20(8):1045–54.
Schmidt M, Gutknecht D, Simon JC, Schulz JN, Eckes B, Anderegg U, et al. Controlling the balance of fibroblast proliferation and differentiation: impact of Thy-1. J Invest Dermatol. 2015;135(7):1893–902.
Craig W, Kay R, Cutler RL, Lansdorp PM. Expression of Thy-1 on human hematopoietic progenitor cells. J Exp Med. 1993;177(5):1331–42.
Cheng BQ, Jiang Y, Zhu Q, Lin WG. Wnt/beta-catenin aids in regulating the proliferation of hepG2 cells mediated by thy-1. Genet Mol Res. 2014;13(3):5115–27.
Takeda H, Yamamoto M, Morita N, Tanizawa T. Relationship between Thy-1 expression and cell-cycle distribution in human bone marrow hematopoietic progenitors. Am J Hematol. 2005;79(3):187–93.
Bradley JE, Ramirez G, Hagood JS. Roles and regulation of Thy-1, a context-dependent modulator of cell phenotype. Biofactors. 2009;35(3):258–65.
Picke AK, Campbell GM, Bluher M, Krugel U, Schmidt FN, Tsourdi E, et al. Thy-1 (CD90) promotes bone formation and protects against obesity. Sci Transl Med. 2018;10(453):eaao6806.
Moraes DA, Sibov TT, Pavon LF, Alvim PQ, Bonadio RS, Da Silva JR, et al. A reduction in CD90 (THY-1) expression results in increased differentiation of mesenchymal stromal cells. Stem Cell Res Ther. 2016;7(1):97.
Saalbach A, Anderegg U. Thy-1: more than a marker for mesenchymal stromal cells. FASEB J. 2019;33(6):6689–96.
Li Q, Wilkie AR, Weller M, Liu X, Cohen JI. THY-1 cell surface antigen (CD90) has an important role in the initial stage of human cytomegalovirus infection. PLoS Pathog. 2015;11(7):e1004999.
Wang W, Shen T, Dong B, Creighton CJ, Meng Y, Zhou W, et al. MAPK4 overexpression promotes tumor progression via noncanonical activation of AKT/mTOR signaling. J Clin Invest. 2019;129(3):1015–29.
Chang MY, Rhee YH, Yi SH, Lee SJ, Kim RK, Kim H, et al. Doxycycline enhances survival and self-renewal of human pluripotent stem cells. Stem Cell Reports. 2014;3(2):353–64.
Knapp DJ, Hammond CA, Aghaeepour N, Miller PH, Pellacani D, Beer PA, et al. Distinct signaling programs control human hematopoietic stem cell survival and proliferation. Blood. 2017;129(3):307–18.
Shen H, Zhou E, Wei X, Fu Z, Niu C, Li Y, et al. High density lipoprotein promotes proliferation of adipose-derived stem cells via S1P1 receptor and Akt, ERK1/2 signal pathways. Stem Cell Res Ther. 2015;6:95.
Bai Y, Shang Q, Zhao H, Pan Z, Guo C, Zhang L, et al. Pdcd4 restrains the self-renewal and white-to-beige transdifferentiation of adipose-derived stem cells. Cell Death Dis. 2016;7:e2169.
Kwon Y, Hofmann T, Montell C. Integration of phosphoinositide- and calmodulin-mediated regulation of TRPC6. Mol Cell. 2007;25(4):491–503.
Guo KY, Halo P, Leibel RL, Zhang Y. Effects of obesity on the relationship of leptin mRNA expression and adipocyte size in anatomically distinct fat depots in mice. Am J Physiol Regul Integr Comp Physiol. 2004;287(1):R112–9.
Fayngerts SA, Wu J, Oxley CL, Liu X, Vourekas A, Cathopoulis T, et al. TIPE3 is the transfer protein of lipid second messengers that promote cancer. Cancer Cell. 2014;26(4):465–78.
Franke TF. Direct regulation of the Akt proto-oncogene product by phosphatidylinositol-3,4-bisphosphate. Science. 1997;275(5300):665–8.
Wang L, Cao XX, Chen Q, Zhu TF, Zhu HG, Zheng L. DIXDC1 targets p21 and cyclin D1 via PI3K pathway activation to promote colon cancer cell proliferation. Cancer Sci. 2009;100(10):1801–8.
Chen Q, Hao W, Xiao C, Wang R, Xu X, Lu H, et al. SIRT6 is essential for adipocyte differentiation by regulating mitotic clonal expansion. Cell Rep. 2017;18(13):3155–66.
Wang X, Wu H, Yu W, Liu J, Peng J, Liao N, et al. Hepatocyte nuclear factor 1b is a novel negative regulator of white adipocyte differentiation. Cell Death Differ. 2017;24(9):1588–97.
Abeysinghe HR, Pollock SJ, Guckert NL, Veyberman Y, Keng P, Halterman M, et al. The role of the THY1 gene in human ovarian cancer suppression based on transfection studies. Cancer Genet Cytogenet. 2004;149(1):1–10.
Lung HL, Bangarusamy DK, Xie D, Cheung AK, Cheng Y, Kumaran MK, et al. THY1 is a candidate tumour suppressor gene with decreased expression in metastatic nasopharyngeal carcinoma. Oncogene. 2005;24(43):6525–32.
Mizoguchi F, Slowikowski K, Wei K, Marshall JL, Rao DA, Chang SK, et al. Functionally distinct disease-associated fibroblast subsets in rheumatoid arthritis. Nat Commun. 2018;9(1):789.
Yang ZF, Ho DW, Ng MN, Lau CK, Yu WC, Ngai P, et al. Significance of CD90+ cancer stem cells in human liver cancer. Cancer Cell. 2008;13(2):153–66.
Shu X, Liu H, Pan Y, Sun L, Yu L, Sun L, et al. Distinct biological characterization of the CD44 and CD90 phenotypes of cancer stem cells in gastric cancer cell lines. Mol Cell Biochem. 2019;459(1–2):35–47.
Buishand FO, Arkesteijn GJ, Feenstra LR, Oorsprong CW, Mestemaker M, Starke A, et al. Identification of CD90 as putative cancer stem cell marker and therapeutic target in insulinomas. Stem Cells Dev. 2016;25(11):826–35.
Choi S, Hedman AC, Sayedyahossein S, Thapa N, Sacks DB, Anderson RA. Agonist-stimulated phosphatidylinositol-3,4,5-trisphosphate generation by scaffolded phosphoinositide kinases. Nat Cell Biol. 2016;18(12):1324–35.
Averaimo S, Assali A, Ros O, Couvet S, Zagar Y, Genescu I, et al. A plasma membrane microdomain compartmentalizes ephrin-generated cAMP signals to prune developing retinal axon arbors. Nat Commun. 2016;7:12896.
Suzuki KG, Kasai RS, Hirosawa KM, Nemoto YL, Ishibashi M, Miwa Y, et al. Transient GPI-anchored protein homodimers are units for raft organization and function. Nat Chem Biol. 2012;8(9):774–83.
Lasserre R, Guo XJ, Conchonaud F, Hamon Y, Hawchar O, Bernard AM, et al. Raft nanodomains contribute to Akt/PKB plasma membrane recruitment and activation. Nat Chem Biol. 2008;4(9):538–47.
Reis-Sobreiro M, Roue G, Moros A, Gajate C, de la Iglesia-Vicente J, Colomer D, et al. Lipid raft-mediated Akt signaling as a therapeutic target in mantle cell lymphoma. Blood Cancer J. 2013;3:e118.
Ryu JM, Han HJ. L-threonine regulates G1/S phase transition of mouse embryonic stem cells via PI3K/Akt, MAPKs, and mTORC pathways. J Biol Chem. 2011;286(27):23667–78.
Gao X, Lowry PR, Zhou X, Depry C, Wei Z, Wong GW, et al. PI3K/Akt signaling requires spatial compartmentalization in plasma membrane microdomains. Proc Natl Acad Sci U S A. 2011;108(35):14509–14.
Dietrich C, Volovyk ZN, Levi M, Thompson NL, Jacobson K. Partitioning of Thy-1, GM1, and cross-linked phospholipid analogs into lipid rafts reconstituted in supported model membrane monolayers. Proc Natl Acad Sci U S A. 2001;98(19):10642–7.
Paulick MG, Bertozzi CR. The glycosylphosphatidylinositol anchor: a complex membrane-anchoring structure for proteins. Biochemistry. 2008;47(27):6991–7000.
Woeller CF, O’Loughlin CW, Pollock SJ, Thatcher TH, Feldon SE, Phipps RP. Thy1 (CD90) controls adipogenesis by regulating activity of the Src family kinase. Fyn FASEB J. 2015;29(3):920–31.
Flores EM, Woeller CF, Falsetta ML, Susiarjo M, Phipps RP. Thy1 (CD90) expression is regulated by DNA methylation during adipogenesis. FASEB J. 2019;33(3):3353–63.
The authors thank the Microscopy Characterization Facility, Shandong University, China, for performing microscopy imaging.
This study is supported by the National Natural Science Foundation of China (81770838, 81471065, 81970733), Shandong Major Research Program (2016GSF201005, 2017GSF218094), and Shandong Provincial Natural Science Foundation (ZR2017BH074).
Ethics approval and consent to participate
All animal studies and sample collection were approved by the Ethical Committee of Qilu Hospital of Shandong University (KYLL-2017(KS)-394). All experimental procedures were performed in accordance with the institutional guidelines for animal care and utilization.
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The authors declare that they have no competing interests.
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Sequences of siCD90 and shCD90. Table S2. Primer pairs used in qPCR. Figure S1. Inhibitory effect of CD90 silencing on AKT activation. Figure S2. Infection of S-ADSCs with GFP-tagged shControl or shCD90 lentivirus. Figure S3. Influence of shCD90 lentivirus on WAT weight. Figure S4. Expression of CyclinD1 and Leptin in adipose tissue. Figure S5. Contribution of CD90 overexpression to AKT activation in ADSCs.
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Pan, Z., Zhou, Z., Zhang, H. et al. CD90 serves as differential modulator of subcutaneous and visceral adipose-derived stem cells by regulating AKT activation that influences adipose tissue and metabolic homeostasis. Stem Cell Res Ther 10, 355 (2019). https://doi.org/10.1186/s13287-019-1459-7