Background
Rheumatoid arthritis (RA) is a systemic, autoimmune, and chronic inflammatory disease which causes pain and dysfunction and leads to the destruction of joints [
1]. The major inflammatory tissue is the synovium, the thin tissue that lines the joint. Immune cells, such as neutrophils, lymphocytes, and monocytes, produce inflammatory cytokines including interleukin (IL)-1, tumor necrosis factor-α (TNF-α), IL-6, and granulocyte-macrophage colony-stimulating factor (GM-CSF) [
2], and are involved in the development of inflammation. It is well-known that peripheral blood monocytes are derived from precursors in the bone marrow, migrate into synovial tissue, and differentiate into macrophages that produce pro-inflammatory cytokines [
3]. Macrophages involved in synovial inflammation transform into osteoclasts, which cause joint destruction in RA [
2,
4]. Osteoclasts are also derived from CD14+ monocytes under the influence of pro-inflammatory cytokines [
5]. Circulating CD14+ monocytes serve as precursors of endothelial cells and contribute to the process of angiogenesis in the tissue [
6]. Based on this background, the identification and classification of peripheral monocytes responsible for the disease is indispensable to understanding the pathogenesis of RA.
CD16 is a receptor for immunoglobulin (Ig) gamma Fc region III (FcγRIII). Fcγ receptors (FcγRs) are expressed on most of the cells involved in the immune system, including circulating monocytes, and they regulate immune responses through interaction with antibodies [
7]. According to these previous studies, immune complexes formed by anti-cyclic citrullinated peptide antibody (ACPA) and citrullinated peptide seem to bind to FcγRs and stimulate immune cell activation and release of inflammatory cytokines in patients with RA [
8]. Therefore, FcγRIII is one of the molecules possibly associated with the pathogenesis of RA. It has been reported that aberrant expression of FcγRIII, or the presence of allelic variants, can contribute to the pathogenesis of RA [
9]. However, the regulatory mechanisms of FcγRIII in RA are not fully understood.
Until now, circulating human monocytes have been classified into CD14+ CD16- (classical) and CD14+ CD16+ subsets according to their expression levels of CD14 and CD16 [
10,
11]. It had been reported that CD14+ CD16+ monocytes are increased in patients with RA [
12]. Recently, a new third monocyte subpopulation, CD14
brightCD16+ monocytes, was defined. According to the new classification system, the CD14+ CD16+ population is classified into CD14
brightCD16+ (intermediate) and CD14
dimCD16+ (non-classical) monocytes, depending on the level of CD14 expression [
13]. The CD14
brightCD16- (classical) monocyte is the major subset, while the CD14
brightCD16+ and CD14
dimCD16+ subsets occur in lower numbers than classical monocytes [
11].
It has been shown that the CD14
brightCD16+ monocyte population increases in inflammatory or infectious conditions and, upon lipopolysaccharide stimulation [
14,
15], produces TNF-α, IL-1β, IL-6, and IL-10. This newly classified CD14
brightCD16+ monocyte population has been reported to be increased in patients with RA, whereas the CD14
dimCD16+ monocyte population is not increased [
14]. It has been suggested that CD14
brightCD16+ monocytes may migrate into the synovium from peripheral blood and differentiate into M1 or M2 macrophages in the tissue [
16]. However, the role of each subset in RA has not been fully clarified.
In this study, we sought to investigate the involvement of CD14brightCD16+ monocytes in the pathogenesis of RA, and possible mechanisms of the enhanced expression of CD16 on monocytes in patients with RA.
Methods
Subjects and study design
Patients with RA (n = 35) (mean age ± SD 59.8 ± 12.6 years, 82.9% female) who met the 2010 American College of Rheumatology/European League Against Rheumatism Classification criteria, and 14 healthy volunteers (mean age 49.2 ± 10.8 (range 30–72), 12 female) were enrolled into the study. All patients visited Keio University Hospital between January 2013 and May 2014 and had never been treated with methotrexate (MTX) or biological agents. They were considered to have moderate or high disease activity (scoring ≥3.2 on the 28-joint disease activity score based on erythrocyte sedimentation rate (DAS28-ESR). All participants gave written informed consent in accordance with the Declaration of Helsinki. MTX was initiated at an oral dose of 4–16 mg weekly. Monocyte subsets from peripheral blood samples were taken at baseline and after 12 weeks of MTX treatment in the patients. Clinical parameters including C-reactive protein (CRP), ESR, matrix metalloproteinase-3 (MMP-3), ACPA, and rheumatoid factor (RF) titers were obtained by routine clinical laboratory methods. DAS28-ESR scores, DAS28-CRP score, clinical disease activity index (CDAI), and simplified disease activity index (SDAI) were also determined at baseline and after 12 weeks of MTX treatment. Clinical characteristics of the patients were retrospectively collected from their medical records.
Monocyte subset determination
Heparinized whole blood was stained with phycoerythrin-Cy7 (PE-Cy7)-conjugated anti-CD14 (clone M5E2, BD Pharmingen, San Diego, CA, USA) and V450-conjugated anti-CD16 antibodies (clone 3G8, BD Horizon, San Jose, CA, USA), and analyzed using a flow cytometer with built-in software (MACSQuant Analyzer® and MACSQuantify® software, Miltenyi Biotec, Bergisch Gladbach, Germany). Monocyte subsets were identified on the basis of forward scatter/side scatter characteristics and CD14-positive gating. Subpopulations of CD14
brightCD16-, CD14
brightCD16+, and CD14
dimCD16+ monocytes were distinguished by their surface expression pattern of CD14 and CD16 according to a previous report [
11] and the proportion of each monocyte subset was determined.
Serum immunoassays
Serum samples were collected at baseline and stored at -80 °C. Serum levels of GM-CSF, interferon-γ (IFN-γ), IL-1β, IL-10, IL-12p70, IL-2, IL-6, IL-8, and TNF-α were measured by multiplex electrochemiluminescence assay (Meso Scale Discovery SECTOR Imager 2400 platform®, Meso Scale Discovery, Rockville MD, USA). Serum macrophage colony-stimulating factor (M-CSF) levels were assessed by enzyme-linked immunosorbent assay (ELISA) (Quantikine® ELISA, Human M-CSF Immunoassay, R&D Systems Inc., Minneapolis MN, USA) and calculated using the manufacturer’s software. Values are expressed in pg/mL and presented as median with interquartile range (IQR).
Stimulation of peripheral monocytes in vitro
Peripheral blood mononuclear cells (PBMCs) were isolated from five healthy volunteers by density gradient centrifugation (Ficoll-Paque®, GE Healthcare, Uppsala, Sweden). To isolate monocyte subsets, cells were stained with phycoerythrin (PE)-conjugated anti-CD14 (clone MφP9, BD Pharmingen) and BV421-conjugated anti-CD16 antibodies (clone 3G8, BD Horizon) and sorted according to their CD14/CD16 expression using a cell sorter (BD Aria III®, BD Biosciences, San Jose CA, USA). CD14brightCD16- monocytes were cultured at 2.5 × 105/500 μL in Roswell Park Memorial Institute medium (RPMI-1640®, ATCC, Manassas, VA, USA) with 10% heat-inactivated fetal bovine serum (MP Biomedicals, Santa Ana CA, USA). They were then stimulated for 14 hours with either 100 ng/mL M-CSF, 1-100 (1, 10, 25, 50, or 100) ng/mL IL-10, 100 ng/mL IL-6, or 20 ng/mL IL-8 at 37 °C in a humidified atmosphere containing 5% CO2. The stimulated monocytes were stained with PE-conjugated anti-CD14, BV421-conjugated anti-CD16, and allophycocyanin (APC)-conjugated anti-HLA (human leukocyte antigen)-DR (clone LN3, eBioscience, San Diego CA, USA) antibodies and we analyzed the proportion of CD16+ monocytes using a flow cytometer.
Detection of IL-10 receptor expression
Heparinized whole blood cells from four healthy volunteers were stained with PE-Cy7-conjugated anti-CD14 (clone M5E2, BD Pharmingen), V450-conjugated anti-CD16 (clone 3G8, BD Horizon), and APC-conjugated anti-IL-10 receptor antibodies (clone 3F9, Biolegend, San Diego CA, USA), and the expression levels of IL-10 receptor on the CD14brightCD16- monocyte subset was evaluated.
IL-10 neutralization assay
CD14brightCD16- monocytes (2.5 × 105/500 μL) from the peripheral blood of four healthy volunteers were incubated with 25 ng/mL IL-10. In some experiments, anti-IL-10 receptor antibody (5 μg/mL) (clone 3F9, Biolegend) or rat IgG2aκ (5 μg/mL) to an irrelevant antigen (clone RTK2758, Biolegend) was added to the cultures. CD16 expression on monocytes was then measured.
Statistical analysis
We used commercial statistical software (JMP 11 system®, SAS Institute Inc., Cary NC, USA). The Wilcoxon rank sum test was used to assess the statistical significance of differences between groups. Correlation between two continuous variables was analyzed using Spearman’s rank correlation coefficient. Dunn’s test was used for multiple comparison procedures. A p value <0.05 was considered statistically significant.
Discussion
In this study, we demonstrate that circulating CD14brightCD16+ monocytes are increased in patients with RA in the active phase and decrease after MTX treatment in a manner that correlates with decreasing disease activity. Moreover, this monocyte subset is associated with expression of inflammatory cytokines in peripheral blood, and the cytokine IL-10, which is increased in patients with RA, induces CD16 expression on monocytes. These results suggest that CD14brightCD16+ monocytes play a role in the pathogenesis of RA, and that IL-10 is a key cytokine in the regulation of CD16 expression.
Although an increase in CD14
brightCD16+ monocytes in patients with RA has been reported [
14], the possibility of correlation between CD14
brightCD16+ monocytes and cytokines in untreated patients with active RA has not yet been investigated. Previous studies have not ruled out any influence of treatment on cytokine and disease activity, because the patients with RA in these studies were not treatment-naïve. Our results support previous observations [
14] and show that the proportion of CD14
brightCD16+ monocytes is increased in treatment-naïve patients with active RA compared to healthy controls, and is positively correlated with disease activity in these patients.
We further showed that the CD14brightCD16- population was negatively correlated with RA disease activity. Notably, the proportion of CD14brightCD16+ monocytes decreased and that of CD14brightCD16- monocytes increased when the patients received MTX treatment.
Though the function of CD14
brightCD16+ monocytes in RA is not still clarified, this population may be involved in the pathogenesis of RA in accordance with our findings that CD14
brightCD16+ monocytes decreased after MTX treatment. It has been shown that MTX inhibits inflammatory cytokine production [
19] and cell proliferation in vitro, and to induce apoptosis of immune cells [
20], but it has not been found to inhibit a specific subset of monocytes. One of the reasons for the decreased proportion of CD14
brightCD16+ monocytes after MTX treatment was probably secondary to a phenomenon derived from the improvement in RA disease activity.
It is reported that M-CSF plays an important role in the introduction of CD14
brightCD16+ monocytes. Anti-M-CSF antibody caused a decrease in circulating CD14
brightCD16+ and CD14
dimCD16+ monocytes in a clinical trial in two patients with active RA [
17]. Moreover, M-CSF and IFN-γ therapy has been found to induce CD16 expression on circulating monocytes in patients with cancer or lymphoma [
21]. CD16 expression has been shown to be induced in monocytes with culture of whole PBMCs with M-CSF or IL-10 on CD14
brightCD16- monocytes in vitro [
12]. Although this report may indicate a possible direct role for cytokines, it did not exclude interactions with other cell subsets among the PBMCs. In our study, using highly purified CD14
brightCD16- monocytes, we clearly showed that IL-10, but not M-CSF, directly induces CD16 expression in CD14
brightCD16- monocytes. In addition, we proved that the enhancement of CD16 expression on CD14
brightCD16- monocytes required the interaction with IL-10 and IL-10 receptor by a neutralization assay with anti-IL-10 receptor antibody.
It is well-known that IL-10 plays a crucial role, such as anti-inflammatory and/or pro-inflammatory roles in the pathogenesis of RA. IL-10 has been shown to inhibit production of IL-6, TNF-α, and GM-CSF from immune cells [
22], and to enhance B cell differentiation to cells secreting IgG, IgM, and IgA [
23,
24], resulting in increased RF and IgG-RF production by B cells in peripheral blood. Moreover, IL-10 is localized to the synovial membrane lining layer, the site of monocyte migration, and inhibits pro-inflammatory cytokines in RA [
25]. In this study, we demonstrated that serum IL-10 in patients with RA was significantly elevated compared with healthy volunteers, and was correlated with disease activity.
IL-10 is secreted by many kinds of cells such as T-cells, B-cells, macrophages, dendritic cells, natural killer cells, and monocytes themselves [
26‐
28]. It is reported that CD16 expression on monocytes is maintained by IL-10 production by human naïve CD4+ T cells [
29]. The function of CD14
brightCD16+ monocytes may be regulated by these cells producing IL-10. IL-10 tended to decrease in patients with RA with decreasing CD14
brightCD16+ monocytes after 12 weeks of treatment. IL-10 may play a role in the induction of CD16 on monocytes in patients with RA.
We note two limitations to our study. First, the number of patients was relatively small, albeit large enough to provide statistically significant data. Second, we did not show that CD14
brightCD16+ monocytes are directly associated with inflammatory cytokines in RA in vivo. Production of IL-6 and TNF-α in CD14
brightCD16+ monocytes was not higher than that in CD14
brightCD16-monocytes (Additional file
1). We thought that CD14
brightCD16+ monocytes could exert both inflammatory and anti-inflammatory effects, and which effect’s dominance would depend on cells producing IL-10. The functions of these monocytes in RA will need to be clarified in future studies.
Acknowledgements
The authors sincerely thank Ms Harumi Kondo and Ms Mayumi Ota for helping with the acquisition of clinical information.
Competing interests
MT and KYo have conflicts of interest to declare. NS has received research grants from Chugai Pharmaceutical Co., Ltd., Mitsubishi Tanabe Pharma Co., Ono Pharmaceutical Co., Ltd. and Nippon Kayaku Co., Ltd. KS has received research grants from Eisai Co., Ltd., and Bristol-Myers Squibb. KYa has received consultant fees from Pfizer, Chugai Pharmaceutical Co., Ltd, Mitsubishi-Tanabe Pharma Co., and Abbvie, and received honoraria from Pfizer, Chugai Pharmaceutical Co., Ltd, Mitsubishi-Tanabe Pharma Co., Bristol-Myers Squibb, Takeda Industrial Pharma, GlaxoSmithkline, Nippon Shinyaku, Eli lilly, Janssen Pharma, Eisai Pharma, Astellas Pharma, and Acterlion Pharmaceuticals and received research support from Chugai Pharma and Mitsubishi-Tanabe Pharma. TT has received lecture fees or research grants from Abbott Japan Co., Ltd., Astellas Pharma, Bristol-Myers K.K., Chugai Pharmaceutical Co, Ltd., Daiichi Sankyo Co., Ltd., Eisai Co., Ltd., Janssen Pharmaceutical K.K., Mitsubishi Tanabe Pharma Co., Pfizer Japan Inc., Sanofi-Aventis K.K., Santen Pharmaceutical Co., Ltd., Teijin Pharma Ltd., Asahikasei Pharma Corp., Taisho Toyama Pharmaceutical Co., Ltd., Janssen Pharmaceutical K.K., Astra Zeneca K.K., Eli Lilly Japan K.K., Novartis Pharma K.K., and Abbvie GK.