Previous in vivo studies have shown that mesenchymal stem cell (MSC) transplantation significantly improves the condition of a number of autoimmune diseases including autoimmune cerebrospinal meningitis, multiple sclerosis, glomerulonephritis and systemic lupus erythematosus.
To investigate the immunoregulatory effect of stem cell transplantation, human umbilical cord MSCs were co-cultured with peripheral blood mononuclear cells (PBMCs) from patients with rheumatoid arthritis (RA). Orphan nuclear receptor gamma (ROR-γ) mRNA and protein expression was detected with real-time PCR and Western blotting. Interleukin (IL)-17, IL-6 and tumor necrosis factor (TNF-α) in the cell culture supernatant were measured using a flow cytometric bead capture method.
After 72 hours of co-culture, the mRNA and protein expression levels of ROR-γ in co-cultured PBMCs were decreased compared with that in PBMC of RA patients cultured alone (p < 0.05). Moreover, the decrement was positively related to the disease activity of RA (p < 0.05). Decreased secretion of IL-17, TNF-α and IL-6 were also found in co-culture supernatants of PBMCs from patients with severe and moderate disease activity, but not in supernatant from PBMCs cultured alone. The decreased cytokine expression levels were positively correlated to the concentrations of MSCs. In contrast, PBMCs from healthy controls or patients with mild RA did not show significant differences in ROR-γ expression or cytokine secretion following co-culture with MSCs as compared with those cultured alone.
In vitro co-culture with MSCs down-regulated the inflammatory response of PBMCs from RA patients with severe disease activity, but had no significant effect on PBMCs from healthy controls or patients with mild disease activity, suggesting that the immunoregulatory role of MSCs may associate with the occurrence of inflammatory mediators.
Rheumatoid arthritis (RA) is a common autoimmune disease, which is usually treated with a combination of anti-rheumatic drugs. However, the clinical remission rate only reaches 40–57% despite serious side effects
. Recently, mesenchymal stem cell (MSC) transplantation has provided an alternative choice for treatment of autoimmune diseases. Animal model studies have found that MSC transplantation significantly improves the autoimmune cerebrospinal meningitis, multiple sclerosis, glomerulonephritis, systemic lupus erythematosus and other autoimmune diseases
[2–5]. Although the mechanism remains largely unknown, MSCs have been shown to play a role in differentiation and proliferation of T lymphocytes
[6, 7]. Recent studies have found that RA patients with joint inflammation have increased helper T lymphocyte cells (Th1) and IL-17 cytokine producing T lymphocytes, which lead to a high level of IL-17 in synovial fluid
. Besides IL-17A and IL-17F, Th17 cells also express IL-6, TNF, IL-21 and IL-26. Results from a collagen-induced arthritis (CIA) animal model indicate that IL-17 receptor signalling is a critical inflammatory regulator
[8, 9]. Thus, overexpression of IL-17 may be associated with the pathogenesis of RA. Orphan nuclear receptor gamma (ROR-γ) is a key transcription factor for the differentiation of Th17 cells and regulates IL-17 expression in vivo and in vitro. ROR-γ knockout mice have shown reduction of Th17 cells and decreased incidence of autoimmune diseases
. Therefore, investigating the interaction between MSCs and Th17 may help to understand the immunological regulation and pathogenesis of RA. In this study, we designed an in vitro co-culture system to observe the immunoregulatory effect of MSCs on Th17 cells of RA patients.
Isolation and culture of umbilical cord MSCs
Umbilical cords were obtained from the Department of Obstetrics & Gynecology at The Second Hospital of Shanxi Medical University. The umbilical cord of related healthy donors were aspirated and was approved by the Ethics Committee of the affiliated the Shanxi Medical University. Umbilical cords from full-term newborn infants were washed with phosphate buffered saline (PBS) under sterile conditions and the blood vessels were carefully removed, leaving only the Wharton gum tissue. MSCs were separated and purified by cell adhesion
[11, 12]. Briefly, the tissue slices were cultured at 37°C in the MSC medium with 5% CO2 and 95% humidity. After 5–7 days, migrated spindle-shaped MSCs were found on the bottom of culture flask. Cells were passaged once 80% confluence was reached. The third-generation of MSCs was detached by 0.25% trypsin, followed by the addition of 10% fetal calf serum (FCS, Phannacia) 3 min later. The cells were centrifuged at 1500 rpm/min for 5 min to remove the supernatant, and resuspened in serum-free medium for cell counting. The cell concentration was adjusted to 2 × 107/mL. Cells were centrifuged at 1500 rpm/min for 5 min and the supernatant was discarded. Cells were diluted with 0.5 ml PBS containing 2% FCS according to the concentrate ratio. The phenotypes of MSCs were assayed by flow cytometry (Beckman Coulter FC500, USA) using the monoclonal antibodies against CD44, CD45, CD34, CD71 and CD105 (BD Pharmingen, USA). Results were analysed using CXP analysis software.
Patient selection and specimen collection
Eighteen RA patients were selected from The Second Hospital of Shanxi Medical University. The study was approved by Shanxi Medical University Ethics Committee, and informed consent was provided to patients according to the Declaration of Helsinki. The patients were grouped according to their disease activity as assessed by the disease active score 28 (DAS28)
1) The low disease activity group contained six patients with DAS28 ≤ 3.2, the moderate group contained six patients with DAS28 >3.2 and ≤5.1, while the severe symptom group had six patients with DAS28 > 5.1. The diagnostic methods were based on the revised 1987 American College of Rheumatology (ACR) diagnostic criteria for RA. RA patients with other chronic diseases, e.g. diabetes, hypertension, coronary heart disease, thyroid disease, or viral hepatitis, were excluded from this study. Of all the patients, three were male and fifteen were females, aged 23–67 years (mean age 38.2 ± 12.2). The healthy control group had six subjects, of which two males and four females were aged 24–56 years (mean age 46.1 ± 11.6). Fifteen millilitres of heparin anti-coagulated blood was drawn from each patient at the morning after a 12-hour fasting period. The blood was diluted 1:1 with Hank’s solution, and peripheral blood mononuclear cells (PBMCs) were separated by gradient centrifugation over Ficoll.
DAS28 ≤ 3.2
3.2 < DAS28 ≤ 5.1
DAS28 > 5.1
(n = 6)
(n = 6)
(n = 6)
(n = 6)
Age, mean ± SD years
38.2 ± 12.2
46.1 ± 11.6
Time duration from diagnosis to inclusion, months
28.2 ± 10.2
30.6 ± 8.2
16.2 ± 6.5
Combination therapy no.
DAS28, * mean ± SD
2.5 ± 0.5
3.6 ± 0.6
5.9 ± 0.7
* DAS28 = Disease Activity Score in 28 joints; See Patients and Methods for description of groups.
Co-culture of PBMCs and MSCs
The PBMCs were resuspended in L-DMEM medium (Sigma company) and were co-cultured with MSCs in different ratios. Firstly, MSC with a cell density of 2 × 107/ml was imbedded in a 6-well plate, and then the numbers of MSCs were counted when they covered around 80% of the area of the cell plate. The average value of the counted number (107) was set as the standard of calculating the number of PBMC in each cell. The settings are as follows: Set I, Umbilical cord MSCs (1 × 107 cells per well) and PBMCs were co-cultured at ratios of 1:1 (1 × 107 cells per well), 1:10 (1 × 108 cells per well) and 1:50 (5 × 108 cells per well); Set II, Umbilical cord MSCs (1 × 107 cells per well) and PBMCs of RA patients in low disease activity group were co-cultured at ratios of 1:1, 1:10 and 1:50 as described above; Set III, Umbilical cord MSCs (1 × 107 cells per well) and PBMCs of moderately active RA patients were co-cultured at ratios of 1:1, 1:10 and 1:50 as described above; Set IV, Umbilical cord MSCs (1 × 107 cells per well) and PBMCs of highly active RA patients were co-cultured at ratios of 1:1, 1:10 and 1:50 as described above. In each set, PMBCs cultured alone (1 × 107 cells per well) were used as the control. Normal control means that MSCs were co-cultured with PBMCs of healthy donor. All culture sets were incubated in 6-well plates in a saturated humidity incubator at 37°C with 5% CO2 for 72 hours. PBMC suspensions were harvested by collecting the supernatant. The cells were collected by centrifugation and the supernatant was kept at −70°C for further analysis.
ROR-γ mRNA expression
Total RNA was extracted from PBMCs using Trizol reagent according to the manufacturer’s instruction, and stored at −70°C. cDNA was synthesized following the procedures of the product operation manual (TaKaRa Code: DRR037S). PCR reactions were set to 20 μL volume containing 10 μL of SYBR®, premix Ex TaqTM II (2 ×) (Fermentas, USA), 7 μL ultra-pure water, 0.5 uL each of sense and anti-sense primers (250 nM, synthesized by Shanghai Biological Engineering Technology Services Limited) and 2 μL of cDNA. PCR was performed in triplicate for each sample and amplification conditions were set as 85°C for 30 sec followed by 40 cycles of 85°C for 5 sec and 56°C for 31 sec. The primer sequences are: ROR-γ sense primer 5′-CAG TGA GAG CCC AGA AGG AC -3′ and anti-sense primer 5′-TCA TCC CAT CCA TTT TTG GT-3′, the product size was 139 bp. The β-actin gene was used as the internal control: the sense primer was 5′- GGC ACC CAG CAC AAT GAA-3′, and the anti-sense primer was 5′-GGA AGG TGG ACA GCG AGG-3′, the product size was 98 bp. All primers were designed using the Primer 3 software.
Western-blotting detection of ROR-γ protein expression
Cell pellets were lysed in 1 mL protein lysate buffer (50 mM Tris, Cl pH 6.8,15 mM NaCl, 5 mM EDTA, 0.5% NP-40, 1 mM PMSF) by repeated pipetting for 100 times using a syringe. The lysates were centrifuged at 10,000 g for 5 min at 4°C. The supernatant was mixed with an equal volume of 2 × SDS buffer (100 mM tris-Cl, 200 mM DTT, 20% glycerol, 0.2% bromophenol blue and 4% SDS) and boiled for 5 min, and then cooled using ice. The supernatant was collected by centrifugation at 10,000 g for 10 minutes at 4°C. The protein was separated by SDS-PAGE and transferred to a PVDF membrane, which was then blocked by 5% BSA at 4°C overnight. The membrane was incubated with a murine anti-human ROR-γ antibody (1:1000; Santa Cruze) and a murine anti-β-actin (1:1000) in Tris-buffered saline containing 0.05% Tween-20 at 4°C overnight, followed by washing and incubation with HRP-labeled anti-mouse Ig secondary antibody (1:10,000; Santa Cruze) for 2 h at room temperature. The membrane was developed with ECL solution and the image was analysed using Gel-Pro Analyzer 4 (Media Cybernetics, USA).
Detection of cytokine secretion
The cytokine levels in the co-culture supernatant were measured and quantitated by multiplex immunoassays using a Cytometric Bead Array (CBA) kit according to the manufacture’s instruction (BD Biosciences, San Jose, CA). The cytometric beads were coated with antibodies against IL-6, TNF-α, IFN-γ and IL-17A used to capture cytokines. Each type of bead had a unique size and fluorescence intensity that can be distinguished by flow cytometry. Cytokines bound to beads were detected by the phycoerythrin (PE) conjugated secondary antibody, which was proportional to the amount of each bound cytokine. Briefly, 50 μL bead suspension and 50 μL of each sample were mixed and incubated at room temperature for 3 h. Followed by the addition of 1 mL washing buffer to each assay tube and centrifugation at 200 g for 5 min, the beads were resuspended with 300 μL washing buffer and analysed by a FACSCalibur flow cytometry (BD Biosciences). Cytokine expressing data was analysed using Flow Cytometric Analysis Program Array software (BD Biosciences).
SPSS 13.0 for Windows was used for statistical analysis and data were presented as mean ± standard deviation (
) or frequency. The one-way ANOVA and post-hoc LSD t-test was used for comparison among groups; meanwhile, post-hoc Dunnett’s T3 method was used for comparison among groups with unequal variance. A P < 0.05 was considered statistically significant.
Phenotype of MSCs
The third passage of isolated human umbilical cord MSCs was analysed by flow cytometry. Results showed that these cells were negative for CD45 and CD34, weak positive for CD71 and positive for CD105, CD44 and CD29 (Figure
Real time PCR detection of mRNA expression for PBMC ROR-γ
Real time-PCR was performed to detect the mRNA expression of PBMC ROR-γ from different groups. All groups showed mRNA expression of ROR-γ. However, compared with PBMCs cultured alone, the ROR-γ mRNA expression was significantly decreased in RA PBMCs co-cultured with MSCs. No statistical difference was found in the mRNA level of ROR-γ from the low (DAS28 ≤ 3.2) and moderate (DAS28 >3.2 and ≤5) RA groups. In the severe RA group (DAS28 > 5.1), following co-culture with different ratios of co-cultured systems, there were significant differences, which was not observed in other groups. Difference was detected in the mRNA expression of PBMC ROR-γ (Figure
Western-blotting detection of PBMC ROR-γ expression
Protein expression of ROR-γ was measured by Western blotting (Figure
2b). The results showed that the ROR-γ protein secretion levels in PBMCs of the severe RA group co-cultured with MSCs were significantly decreased as compared to that in PBMCs cultured alone. This difference was not found in any other groups (Figure
Secretion of pro-inflammatory cytokines
The release of IL-17, TNF-α and IL-6 in culture supernatant was measured using CBA analysis (Figure
3a-c). The results showed that in the severe and moderate RA groups, the releases of IL-17, TNF-α and IL-6 were decreased significantly in co-cultured cells compared with other groups (p < 0.05). The decreased levels of cytokine expression were correlated to the ratio of MSCs and PBMCs, indicating that in vitro secretion of IL-17 by PBMCs from highly activated RA patients was inhibited by MSCs in a dose-dependent manner. In contrast, MSCs did not inhibit cytokine expression of PBMCs from mild RA patients or healthy controls.
This study used an in vitro co-culture system to investigate the interaction between MSCs and Th17 cells in PBMCs of RA patients. The biological function of Th17 cells were inhibited by co-cultured MSCs. IL-17, IL-6 and TNF-α were over-expressed in the highly active RA group, but this over-expression was suppressed to a various extent after being co-cultured with MSCs. Moreover, the inhibitory effect was correlated with the ratio of MSCs and PBMCs in the co-culture. However, the mechanisms are unclear. ROR-γ is a key transcription factor for Th17 cell differentiation and important for IL-17 expression in vivo and in vitro. Our results showed that MSCs played an inhibitory role in regulation of ROR-γ mRNA and protein expression when co-cultured with PBMC from RA patients, especially in highly active RA patients. Therefore it is possible that MSCs inhibit the function of Th17 cells via down-regulation of ROR-γ.
Interestingly, the dose-dependent inhibitory effect of MSCs was only found in high active group, MSCs in the low disease activity group and the healthy control group did not inhibit the secretion of IL-17 or other cytokines. Thus, the immune regulatory role of MSCs may depend on an inflammatory environment as activated RA patients are closely associated with high inflammatory response. On the other hand, the inhibitory effect of MSCs may be primed by a pro-inflammatory stimulus, such as lipopolysaccharide or IFN-γ. A recent study has shown that IFN-γ enhances the immune regulatory effect of MSCs, leading to promising results for the treatment of graft-versus-host disease
. Thus, transplantation of primed MSCs may have therapeutic potential for the treatment of RA.
In this study, we found that in vitro co-culture with MSCs down-regulated the inflammatory response of PBMCs from RA patients with severe disease activity, suggesting that the immunoregulatory role of MSCs may associate with the occurrence of inflammatory mediators. Further study on how MSCs regulate Th17 cells in an inflammatory microenvironment may pave a road to a new therapeutic strategy for RA.
This study was supported by the Innovation Fund of the Education Department of Shanxi Province (Grant No.2010030).
Branch hospital in Fengxian of shanghai No. 6 people’s hospital, Shanghai Fengxian Center Hospital
The Second Hospital Affiliated of Shanxi Medical University
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