- Research article
- Open Access
Skewed distribution of proinflammatory CD4+CD28nullT cells in rheumatoid arthritis
Arthritis Research & Therapyvolume 9, Article number: R87 (2007)
Expanded populations of CD4+ T cells lacking the co-stimulatory molecule CD28 (CD4+CD28null T cells) have been reported in several inflammatory disorders. In rheumatoid arthritis, increased frequencies of CD4+CD28null T cells in peripheral blood have previously been associated with extra-articular manifestations and human cytomegalovirus (HCMV) infection, but their presence in and contribution to joint manifestations is not clear. In the present article we investigated the distribution of CD4+CD28null T cells in the synovial membrane, synovial fluid and peripheral blood of RA patients, and analysed the association with erosive disease and anti-citrullinated protein antibodies. CD4+CD28null T cells were infrequent in the synovial membrane and synovial fluid, despite significant frequencies in the circulation. Strikingly, the dominant TCR-Vβ subsets of CD4+CD28null T cells in peripheral blood were often absent in synovial fluid. CD4+CD28null T cells in blood and synovial fluid showed specificity for HCMV antigens, and their presence was clearly associated with HCMV seropositivity but not with anti-citrullinated protein antibodies in the serum or synovial fluid, nor with erosive disease. Together these data imply a primary role for CD4+CD28null T cells in manifestations elsewhere than in the joints of patients with HCMV-seropositive rheumatoid arthritis.
T cells are likely to play an important role in the pathogenesis of rheumatoid arthritis (RA) (reviewed in ). In the synovial joint, infiltrating T cells are predominantly of the CD4+ phenotype and are often found in the proximity of B cells and macrophages. These T cells could either represent cells potentiating the function of infiltrating leukocytes or represent suppressive regulatory T cells. Neither specific autoantigens nor autoreactive T cells have so far been conclusively demonstrated in RA. However, a distinct population of oligoclonally expanded proinflammatory CD4+ T cells is found with increased frequencies in peripheral blood in RA patients compared with healthy control individuals [2–4]. These cells display a proinflammatory phenotype, are terminally differentiated, express a variety of NK cell-related receptors and lack the co-stimulatory molecule CD28; the cells are therefore often referred to as CD4+CD28null T cells [5, 6].
The presence of these CD4+CD28null T cells in peripheral blood has been associated with human cytomegalovirus (HCMV) seropositivity, extra-articular manifestations and cardiovascular disease in RA patients [7–9]. Despite increased frequencies of CD4+CD28null T cells in the circulation of RA patients, however, their contribution to erosive disease is still unclear: while studies from Pawlik and colleagues and Goronzy and colleagues found associations between circulating CD4+CD28null T cells and erosive disease [4, 10], Martens and colleagues and Gerli and colleagues did not observe such associations [3, 9].
We had a unique opportunity to investigate the presence of these CD4+CD28null T cells in the synovial membrane, the synovial fluid and peripheral blood from the same patients in a large cohort of RA patients. The association with erosive disease and the levels of antibodies to citrullinated peptides/antigens was examined. Furthermore, CD4+CD28null T cells isolated from the synovial fluid were investigated with regard to antigen specificity and selective recruitment to the joint.
Materials and methods
One hundred and twenty-eight patients with RA were enrolled in the study. All fulfilled the American College of Rheumatology criteria for RA and attended the Rheumatology Clinic at Karolinska University Hospital, Stockholm, Sweden for corticosteroid injections of inflamed joints . Before the corticosteroid injections, synovial fluids were acquired from the knee joints (n = 128), the elbow (n = 1) or the shoulder joints (n = 2). Eighty per cent of the patients were women, median age of 56 years (range, 25–82 years) and a median disease duration of 9 years (range, 0–45 years).
Assessment of erosive disease was performed by radiographic evaluations of the ankle joints or wrist joints by the same two rheumatologists. Radiographic changes in one or more joints were found in 51 out of 70 (73%) patients included in these analyses. The majority of the patients were treated either with nonsteroidal anti-inflammatory drugs, with systemic or local corticosteroid treatment, with methotrexate alone or in combination with corticosteroids (prednisolone), or with TNF blockers alone or in combination with methotrexate. Some patients were untreated.
This study was approved in compliance with the Helsinki Declaration by the Ethics Committee of the Karolinska University Hospital, and all patients and healthy subjects gave informed consent.
Arthroscopy and synovial biopsies
Knee joint synovial biopsies were acquired according to a previously described procedure . Biopsies were taken at the site of inflammation, either close to cartilage or not close to cartilage, defined as either less than 1.5 cm or more than 1.5 cm from cartilage, respectively.
Three-colour immunofluorescence microscopy
Frozen unfixed synovial biopsy sections were fixed with acetone. Sections were incubated overnight with the cocktail of primary antibodies – CD244 (R&D Systems, Minneapolis, MN, USA), CD4 (Becton Dickinson, San Jose, CA, USA), CD3 (DakoCytomation, Glostrup, Denmark) – or the isotype control antibodies – goat IgG (Caltag Laboratories, Burlingame, CA, USA), mouse IgG1 (DakoCytomation) and rabbit immunoglobulin (DakoCytomation). Excess of antibodies were washed away before incubation with the secondary antibodies – anti-sheep/goat immunoglobulin-biotin (The Bidning Site, Birmingham, UK), avidin-Oregon Green 488 (Molecular Probes, Eugene, OR, USA), anti-mouse IgG-Rhodamine RedTM-X (Jackson ImmunoResearch Laboratories, West Grove, PA, USA) and anti-rabbit IgG-AMCA (Jackson ImmunoResearch).
Stained tissue sections were examined with a Leica DM RXA2 microscope (Leica Microsystems, Wetzlar, Germany) equipped with a Leica DC 300F (Leica Microsystems DI, Cambridge, UK) digital colour video camera connected to a PC computer. Photographs were analysed with Leica IM500 software (Leica Microsystems, Heerbrugg, Switzerland).
CD4+CD28null T cells were identified by morphologically cell-like structures with co-localized immunostainings of CD3, CD4 and CD244, and were manually quantified in independent analyses performed by two persons. CD4dim macrophages/monocytes and NK cells , which also might express CD244, could be excluded using the combination of CD3 and CD4 in the three-colour stainings to identify CD4+ T cells. The density of CD4+CD28null T cells were calculated by dividing the number of CD4+CD28null T cells by the total area of infiltrating T cells, measured with Image J software version 1.34s (National Institutes of Health, Bethesda, MD, USA).
The frequency of CD4+CD28null T cells in peripheral blood and synovial fluid was analysed by four-colour flow cytometry (FACSCalibur instrument; Becton Dickinson Immunocytometry Systems, San Jose, CA, USA) in peripheral blood mononuclear cells and synovial fluid mononuclear cells after Ficoll separation (Ficoll-Paque Plus; GE Healthcare Biosciences AB, Uppsala, Sweden). The antibodies used were CD3-FITC, CD28-APC (Pharmingen; Becton Dickinson, San Diego, CA, USA), CD4-PerCP (Becton Dickinson, San Jose) and CD244-PE (Immunotech, Marseille, France).
The TCR-Vβ usage was determined by the IOTest1 Beta Mark kit (Beckman Coulter, Marseille, France). The TCR-Vβ stainings were combined with antibodies to CD4 and CD28 (see above) to identify CD4+CD28null T cells and CD4+CD28+ T cells.
Peripheral blood mononuclear cells and synovial fluid mononuclear cells stimulated with HCMV antigens (see below) were analysed by flow cytometry after immunostaining with IFNγ-FITC, CD28-PE, CD3-APC and CD14-APC-Cy7 (all from Becton Dickinson, San Diego, CA, USA) and CD4-PerCp (Becton Dickinson, San Jose, CA, USA).
Flow cytometric data were analysed with CellQuest software (Becton Dickinson, Franklin Lakes, NJ, USA) or FlowJo software (Tree Star Inc., Ashland, OR, USA). The frequency of CD4+CD28null T cells was calculated as the percentage of CD28-negative cells in the gated CD3+CD4+ population.
The functional capacity of CD4+CD28null T cells from the synovial fluid and peripheral blood were assessed by IFN-γ production. Two million peripheral blood mononuclear cells and synovial fluid mononuclear cells from eight patients were either stimulated with plate-bound anti-CD3 antibodies (OKT-3) at 0 or 0.1 μg/ml for 4 hours, or by 2 μg/ml pp65 and immediate early HCMV antigens (JPT Peptide Technologies GmbH, Berlin, Germany) for 8 hours.
Activated cells were either detected by secretion (MACS Secretion Assay; Miltenyi Biotec, Bergisch Gladbach, Germany) or by upregulation of intracellularly stored IFN-γ (Becton Dickinson, San Diego, CA, USA) according to the manufacturers' protocols. The frequency of IFN-γ secreting CD3+CD4+CD28null T cells was analysed by flow cytometry (see above).
Enzyme-linked immunosorbent assay
The anti-CCP2 test (Immunoscan RA, Mark 2; Euro-Diagnostica, Arnhem, The Netherlands) was used to determine the levels of anti-citrullinated peptide/protein antibodies (ACPA) in the serum and synovial fluid. A cutoff value of 25 U/ml was used according to the manufacturer's instructions. Serum and synovial fluid samples were diluted equally (1:50) and were analysed on the same plate.
The presence of anti-HCMV IgG and IgM antibodies in the serum and the synovial fluid, from the same time point as the screening of CD4+CD28null T cells, was tested in an enzygnost anti-HCMV/IgG ELISA and an enzygnost anti-HCMV/IgM ELISA (Dade Behring, Marburg, Germany). Sera from HCMV-seronegative patients were further examined for detection of IgG against HCMV using antigens prepared from a HCMV clinical isolate (C6) using an ELISA as previously described by Rahbar and colleagues . Control antigen was prepared from uninfected fibroblasts.
Comparisons of nonparametrically distributed data in two independent groups or compartments were performed by the Mann–Whitney test. The Spearman test for correlation was used for analyses of covariation of two nonparametrically distributed data.
CD4+CD28nullT cells are scarce in the synovial membrane
To investigate the presence of CD4+CD28null T cells in the synovial membrane, we used three-colour immunofluorescence microscopy. This technique utilizes our findings of CD244 expression by CD4+ T cells as a specific marker for the CD28null subset in peripheral blood of patients with RA and muscle tissue of patients with myositis (Figure 1) (Fasth et al., submitted).
CD244 is hitherto mainly described as a receptor regulating activation of NK cells after interaction with its ligand CD48 . CD244 might have similar functions on T cells, but this is not yet fully understood . Instead of detecting T cells lacking CD28, CD4+CD28null T cells in synovial membrane biopsies were identified by co-expression of CD244, CD3 and CD4 (Figure 1). Two patient groups were analysed: patients having less than 0.5% and patients having more than 7% of circulating CD4+CD28null T cells (Table 1). In all 11 patients, as expected, CD3-positive cells were abundant in the synovial membrane, and a majority of the CD3-positive cells also expressed CD4 (Figure 1). Only small numbers of CD4+CD28nullCD244+ T cells were found. They were evenly distributed and without correlation with the size of the T-cell infiltrates, the frequencies of CD4+CD28null T cells in peripheral blood or with ongoing medication. From these results we conclude that the vast majority of CD4+CD28null T cells do not home specifically to the synovial membrane despite significant frequencies in the circulation.
CD4+CD28nullT cells are restricted to HCMV-seropositive patients and are less frequent in synovial fluid than in peripheral blood
We then analysed the presence of CD4+CD28null T cells in the synovial fluid by screening synovial fluid samples from 128 patients by flow cytometry. CD4+CD28null T cells could be detected in synovial fluid at a median frequency of 1.9% (range 0–27%). These percentages, however, were significantly lower than in paired peripheral blood samples (median, 4.4%; range, 0–50%; P < 0.001) (Figure 2a). Despite significant differences in the two compartments, patients with the largest population of CD4+CD28null T cells in the synovial fluid still tended to have the highest frequencies in peripheral blood (r = 0.47, P < 0.0001) (Figure 2b).
Analysis of 14 patients with two simultaneous synovial fluid samples demonstrated that the presence of CD4+CD28null T cells in one inflamed joint reflects the occurrence also in other affected joints (Figure 2c). Patient groups undergoing different medical treatments (untreated, nonsteroidal anti-inflammatory drug, methotrexate or TNF blockade) did not have different frequencies of CD4+CD28null T cells in the peripheral blood or the synovial fluid (data not shown).
Increased frequencies of circulating CD4+CD28null T cells in patients with RA have been associated with HCMV infection; whether this is also valid for synovial CD4+CD28null T cells is not known. Strikingly, we found significant CD4+CD28null T-cell populations only in the synovial fluid of HCMV-seropositive individuals (P < 0.01) (Figure 2d). Comparative analysis of the frequencies of CD4+CD28null T cells in the synovial fluid and peripheral blood of HCMV IgG-seropositive patients clearly showed that CD4+CD28null T cells were less frequent in synovial fluid compared with peripheral blood also in this subset of patients (P < 0.0001) (Figure 2f). The serum titres of anti-HCMV IgG correlated with the levels in the synovial fluid (r = 0.87, P < 0.0001; data not shown). Seven patients (15%) displayed both anti-HCMV IgM and anti-HCMV IgG antibodies, indicating a recent or ongoing infection, but the frequency of CD4+CD28null T cells in the circulation and synovial fluid was similar to IgG-seropositive patients lacking IgM (data not shown).
These data demonstrate that CD4+CD28null T cells are only present in the synovial fluid and peripheral blood of RA patients seropositive for HCMV, and demonstrate that, despite significant frequencies in peripheral blood, CD4+CD28null T cells are infrequent in the synovial compartment.
CD4+CD28nullT cells from synovial fluid are functional and reactive to HCMV antigens
We have previously reported that CD4+CD28null T cells from the peripheral blood rapidly respond to low TCR stimulation mimicked by a low concentration of anti-CD3 antibodies . To investigate whether CD4+CD28null T cells in the synovial fluid displayed the same hyperresponsiveness, we measured the frequency of IFN-γ-secreting CD4+CD28null T cells in mononuclear cells from synovial fluid. Indeed, these cells showed a similar response as CD4+CD28null T cells from the peripheral blood (Figure 3, upper panel), indicating that CD4+CD28null T cells in the synovial compartment have a capacity to function as local effector T cells.
With the strong association between CD4+CD28null T cells and HCMV seropositivity we also investigated whether IFN-γ production could be provoked from CD4+CD28null T cells in peripheral blood and synovial fluid, after stimulation by the HCMV-derived pp65 and immediate early antigens. Interestingly, synovial fluid-derived CD4+CD28null T cells from all investigated patients showed specificity for these antigens (Figure 3, lower panel). These results indicate that HCMV-derived peptides can activate at least a subset of CD4+CD28null T cells to function as effector T cells.
Selected subsets of CD4+CD28nullT cells have access to the inflamed joint
Hitherto we have shown that CD4+CD28null T cells are less frequent in the synovial fluid compared with peripheral blood. We next investigated whether there was a selective recruitment of certain subsets of CD4+CD28null T cells to the joint. Using antibodies detecting 24 different TCR-Vβ chains, we could identify TCR-Vβ subsets of the CD4+CD28null T-cell population in both peripheral blood and synovial fluid. Two distinct patterns of TCR-Vβ distribution were found in the joint.
In six of the 13 patients analysed, the dominant TCR-Vβ within the CD4+CD28null T-cell population in peripheral blood was also present in the joint. In one such representative patient, with total frequencies of 7%, 1% and 1.5% CD4+CD28null T cells in the circulation, in the left knee synovial fluid and in the right knee synovial fluid respectively, 29–36% of the CD4+CD28null T cells in all three compartments expressed TCR-Vβ13.1 (Figure 4a). In contrast, synovial fluid from five patients displayed a clear exclusion of the dominant CD4+CD28null T cells from peripheral blood. In the most prominent case, a patient with total frequencies of 9% CD4+CD28null T cells in peripheral blood and 4% in the synovial fluid, 71.5% of the CD4+CD28null T cells in the circulation expressed Vβ20 but only 4.5% of the cells in the joint expressed Vβ20. In contrast, there was an enrichment of TCR-Vβ5.1-expressing CD4+CD28null T cells in the joint (Figure 4b). Patients with the restricted pattern did not display lower overall frequencies of synovial fluid CD4+CD28null T cells as compared with patients with the same TCR-Vβ dominance in peripheral blood and synovial fluid. Neither did different medical treatments co-segregate with either pattern of TCR-Vβ distribution (data not shown). Interestingly, in one patient displaying two TCR-Vβ subsets covering more than 75% of the circulating CD4+CD28null population, one of the subsets had access to, and was even significantly enriched in, the synovial fluid, while the other dominant subset was clearly restricted (Figure 4c). Two patients did not display any of these distinct patterns of TCR-Vβ distribution.
In all 13 patients, the distribution of TCR-Vβ subsets in the conventional CD4+CD28+ T-cell population was not dramatically different in the synovial fluid from that in peripheral blood, as illustrated in Figure 4a–c. These results suggest that the access of CD4+CD28null T cells to the joint is restricted to certain TCR-Vβ subsets, and that RA patients can be divided into two distinct groups with regard to different access of CD4+CD28null T-cell subsets to the joint.
Associations between CD4+CD28nullT cells, ACPA and erosive disease
The presence of ACPA is RA specific and is an early predictor of an aggressive disease course [17, 18]. We therefore analysed whether the frequencies of CD4+CD28null T cells in the circulation and in the synovial fluid were associated with the presence of ACPA in these compartments. We found no differences in the frequencies of circulating or synovial CD4+CD28null T cells in patients with or without ACPA in these locations (Figure 5a,b).
To investigate the association between CD4+CD28null T cells and erosive disease, we allocated patients into two clearly distinguishable groups of either significant erosive disease (n = 21) or no signs of erosive disease (n = 16) according to radiographic evaluations. We had access to longitudinal follow-up data on patients without erosions up to 10 years after disease onset; therefore, patients allocated to the erosive group also had a disease duration of a maximum 10 years. Since subgroups of patients with different treatment did not display different frequencies of CD4+CD28null T cells either in peripheral blood or in synovial fluid, treatment was not considered a parameter to stratify for in this analysis. The results indicated that CD4+CD28null T cells were not specifically enriched in the joint or peripheral blood of patients with erosive disease (Figure 5c,d), which is in accordance with the lack of correlation with ACPA levels.
Increased frequencies of CD4+CD28null T cells have been associated with extra-articular manifestations [3, 4]. Three cases of such manifestations were reported in our cohort. One patient, rheumatoid factor-positive and HLA-B27-positive, with iritis had no CD4+CD28null T cells either in blood or the synovial fluid. In contrast, two patients with pleurisy had 31% and 33% CD4+CD28null T cells in peripheral blood and 2.3% and 6.4% in the synovial fluid, respectively. Despite only two patients, these observations are in line with the notion of an association between CD4+CD28null T cells and extra-articular manifestations in RA.
Taken together, our data from peripheral blood and the inflamed synovial joint show no association between the presence of CD4+CD28null T cells and joint destruction.
Herein we demonstrate that only minor populations of CD4+CD28null T cells were present in the inflamed joints of RA patients, despite significant percentages in peripheral blood. The presence of CD4+CD28null T cells in peripheral blood and the synovial fluid was strongly associated with HCMV IgG seropositivity, but not with ACPA or erosive disease.
Our results on the presence of CD4+CD28null T cells in the synovial fluid were based on screening for CD3+CD4+CD28- cells. It was therefore important to consider the stability of the CD28-negative phenotype. Data from in vitro experiments indicate that cytokines such as TNF and IL-12 in synovial fluid can modify CD28 expression, complicating the analyses of CD4+CD28null T cells in the joint [19, 20]. We believe our data, however, not to be biased by the cytokines present in the synovial fluid since there was no over-representation of synovial CD4+CD28+ T cells expressing the TCR-Vβ chains preferentially expressed by peripheral blood CD4+CD28null T cells (Figure 4). Interestingly, previous studies have shown a reduction in the frequency of CD4+CD28null T cells in peripheral blood after TNF blockade [9, 21–23]. In our cohort, neither TNF blockade nor any of the other most frequently used medical treatments (untreated, nonsteroidal anti-inflammatory drug, methotrexate) was associated with the distribution of CD4+CD28null T cells in the synovial fluid, peripheral blood and synovial tissue. It is therefore likely that the effect of TNF blockade on CD4+CD28null T cells is primarily seen when comparing the same patients before and after treatment, rather than comparing heterogeneous groups of patients with and without this treatment.
CD4+CD28null T cells from both peripheral blood and synovial fluid demonstrated reactivity to HCMV-derived antigens. That the frequency of responding CD4+CD28null T cells was higher in the synovial fluid compared with the peripheral blood does not necessarily mirror an accumulation of HCMV-reactive CD4+CD28null T cells in this compartment, since the same effect was seen for CD4+CD28+ T cells (data not shown). These differences might instead be due to a different status of accessory cells from the two compartments. We also analysed the HCMV specificity of the dominant TCR-Vβ subsets of CD4+CD28null T cells from two patients comprising 20% and 29% of the total CD4+CD28null population in both peripheral blood and synovial fluid. Interestingly, the TCR-Vβ dominant CD4+CD28null T-cell subsets did not respond either to pp65 or to immediate early antigens, indicating that the TCR-Vβ dominant subsets might be reactive to antigens other than those considered immunodominant for HCMV (data not shown). This might be explained by a hypothesis suggested by Davenport and colleagues, who demonstrate that during chronic Esptein–Barr virus infections T-cell clones reactive to the most dominant epitopes rapidly decrease after primary infection and that clonotypes reactive to less dominant epitopes control the recurrent infections . At present, however, we can not exclude that some of the CD4+CD28null T cells with access to the joint have specificity for cartilage-derived and/or citrullinated candidate antigens.
It is intriguing that only certain subsets of CD4+CD28null T cells reach the synovial fluid. Since we were not able to detect all possible TCR-Vβ chains, we cannot exclude that there is an even more pronounced discrimination of CD4+CD28null T cells expressing nondetectable TCR-Vβ chains. The reason for this skewed distribution of CD4+CD28null T cells in peripheral blood and synovial fluid, both with regard to subsets of CD4+CD28null T cells and to the size of whole populations, can with present knowledge only be speculated upon. Owing to the strong association of CD4+CD28null T cells to HCMV seropositivity, it is tempting to assume that the location or status of the HCMV infection plays an important role. Because of the increased frequencies in peripheral blood and exclusion from the synovial fluid, it is probable that tissues other than the rheumatic joint are the primary homing sites for CD4+CD28null T cells in these patients. The few CD4+CD28null T cells found in the joint could instead be a consequence of general patrolling initiated by infection in other tissues. A widespread distribution of virus-specific T cells in a site other than the actual site of virus infection has previously been demonstrated in mouse models . Further investigations considering the expression of chemokine receptors/integrins, antigen specificity, location of the HCMV infection and the presentation of HCMV antigens are needed to clarify this issue. The frequency of CD4+CD28null T cells in the synovial fluid does not necessarily reflect the situation in the inflamed synovia, although in our cohort the low CD4+CD28null T-cell frequencies in the synovial fluid were in agreement with the modest numbers in the inflamed synovial membrane.
CD4+CD28null T cells isolated from the synovial fluid could function as effector T cells by rapid secretion of IFN-γ. Interestingly, IFN-γ is only scarcely found in the T-cell infiltrates of the rheumatic synovial membrane and has therefore not been considered a key cytokine in the pathogenesis of RA . Several reports instead indicate the importance of IL-17, and recent publications have further shown that IFN-γ counteracts the differentiation of IL-17-producing T cells [27–29]. Since CD4+CD28null T cells produce IFN-γ but not IL-17 [6, 30], it is possible that CD4+CD28null T cells, if activated in the joint by secretion of IFN-γ, might even inhibit the synovial inflammation in RA.
The limited presence of CD4+CD28null T cells in the synovial fluid, despite increased frequencies in peripheral blood and their equal distribution in patients with and patients without erosive disease, indicates no significant role for CD4+CD28null T cells in the local inflammation driving joint destruction. Instead, these data indirectly support the previously suggested role for these cells in extra-articular manifestations and cardiovascular disease. That is, CD4+CD28null T cells are exclusively present in HCMV IgG-seropositive RA patients and are reactive to HCMV antigens (present study and ), CD4+CD28null T cells only have limited access to the inflamed joint despite increased frequencies in the circulation (present study), increased frequencies of CD4+CD28null T cells do not correlate with erosive disease (present study and [3, 9]), RA patients with high frequencies of circulating CD4+CD28null T cells display increased risk for cardiovascular events compared with patients lacking CD4+CD28null T cells [9, 31], CD4+CD28null T cells have been found in atherosclerotic plaques and can mediate lysis of endothelial cells in vitro [32, 33], HCMV is frequently found in atherosclerotic and nonatherosclerotic vascular walls , and HCMV increases the thrombogenicity of endothelial cells .
CD4+CD28null T cells and HCMV might not be the only mediators of cardiovascular events in RA, but these studies together strongly link CD4+CD28null T cells and HCMV infection to cardiovascular events, which is found with increased prevalence and is the major cause of death in patients with RA.
In the present study we have shown that CD4+CD28null T cells in RA only are present in HCMV-seropositive patients and display a skewed distribution in the inflamed joint compared with that in peripheral blood. Consistent with the limited number of CD4+CD28null T cells in the joints, these cells were not associated with joint destruction indicated by radiographic analyses or ACPA antibodies predictive of erosive disease.
= anti-citrullinated protein antibodies
= enzyme-linked immunosorbent assay
= human cytomegalovirus
= rheumatoid arthritis
= T-cell receptor
= tumour necrosis factor.
Lundy SK, Sarkar S, Tesmer LA, Fox DA: Cells of the synovium in rheumatoid arthritis. T lymphocytes. Arthritis Res Ther. 2007, 9: 202-212. 10.1186/ar2107.
Schmidt D, Martens PB, Weyand CM, Goronzy JJ: The repertoire of CD4+ CD28- T cells in rheumatoid arthritis. Mol Med. 1996, 2: 608-618.
Martens PB, Goronzy JJ, Schaid D, Weyand CM: Expansion of unusual CD4+ T cells in severe rheumatoid arthritis. Arthritis Rheum. 1997, 40: 1106-1114. 10.1002/art.1780400615.
Pawlik A, Ostanek L, Brzosko I, Brzosko M, Masiuk M, Machalinski B, Gawronska-Szklarz B: The expansion of CD4+CD28- T cells in patients with rheumatoid arthritis. Arthritis Res Ther. 2003, 5: R210-R213. 10.1186/ar766.
Warrington KJ, Takemura S, Goronzy JJ, Weyand CM: CD4+,CD28- T cells in rheumatoid arthritis patients combine features of the innate and adaptive immune systems. Arthritis Rheum. 2001, 44: 13-20. 10.1002/1529-0131(200101)44:1<13::AID-ANR3>3.0.CO;2-6.
Fasth AE, Cao D, van Vollenhoven R, Trollmo C, Malmström V: CD28nullCD4+ T cells – characterization of an effector memory T-cell population in patients with rheumatoid arthritis. Scand J Immunol. 2004, 60: 199-208. 10.1111/j.0300-9475.2004.01464.x.
Hooper M, Kallas EG, Coffin D, Campbell D, Evans TG, Looney RJ: Cytomegalovirus seropositivity is associated with the expansion of CD4+CD28- and CD8+CD28- T cells in rheumatoid arthritis. J Rheumatol. 1999, 26: 1452-1457.
Fletcher JM, Vukmanovic-Stejic M, Dunne PJ, Birch KE, Cook JE, Jackson SE, Salmon M, Rustin MH, Akbar AN: Cytomegalovirus-specific CD4+ T cells in healthy carriers are continuously driven to replicative exhaustion. J Immunol. 2005, 175: 8218-8225.
Gerli R, Schillaci G, Giordano A, Bocci EB, Bistoni O, Vaudo G, Marchesi S, Pirro M, Ragni F, Shoenfeld Y, Mannarino E: CD4+CD28- T lymphocytes contribute to early atherosclerotic damage in rheumatoid arthritis patients. Circulation. 2004, 109: 2744-2748. 10.1161/01.CIR.0000131450.66017.B3.
Goronzy JJ, Matteson EL, Fulbright JW, Warrington KJ, Chang-Miller A, Hunder GG, Mason TG, Nelson AM, Valente RM, Crowson CS, et al: Prognostic markers of radiographic progression in early rheumatoid arthritis. Arthritis Rheum. 2004, 50: 43-54. 10.1002/art.11445.
Arnett FC, Edworthy SM, Bloch DA, McShane DJ, Fries JF, Cooper NS, Healey LA, Kaplan SR, Liang MH, Luthra HS, et al: The American Rheumatism Association 1987 revised criteria for the classification of rheumatoid arthritis. Arthritis Rheum. 1988, 31: 315-324. 10.1002/art.1780310302.
Baeten D, Van den Bosch F, Elewaut D, Stuer A, Veys EM, De Keyser F: Needle arthroscopy of the knee with synovial biopsy sampling: technical experience in 150 patients. Clin Rheumatol. 1999, 18: 434-441. 10.1007/s100670050134.
Bernstein HB, Plasterer MC, Schiff SE, Kitchen CM, Kitchen S, Zack JA: CD4 expression on activated NK cells: ligation of CD4 induces cytokine expression and cell migration. J Immunol. 2006, 177: 3669-3676.
Rahbar AR, Sundqvist VA, Wirgart BZ, Grillner L, Söderberg-Naucler C: Recognition of cytomegalovirus clinical isolate antigens by sera from cytomegalovirus-negative blood donors. Transfusion. 2004, 44: 1059-1066. 10.1111/j.1537-2995.2004.03292.x.
Bryceson YT, March ME, Ljunggren HG, Long EO: Synergy among receptors on resting NK cells for the activation of natural cytotoxicity and cytokine secretion. Blood. 2006, 107: 159-166. 10.1182/blood-2005-04-1351.
Assarsson E, Kambayashi T, Persson CM, Chambers BJ, Ljunggren HG: 2B4/CD48-mediated regulation of lymphocyte activation and function. J Immunol. 2005, 175: 2045-2049.
Rönnelid J, Wick MC, Lampa J, Lindblad S, Nordmark B, Klareskog L, van Vollenhoven RF: Longitudinal analysis of citrullinated protein/peptide antibodies (anti-CP) during 5 year follow up in early rheumatoid arthritis: anti-CP status predicts worse disease activity and greater radiological progression. Ann Rheum Dis. 2005, 64: 1744-1749. 10.1136/ard.2004.033571.
Machold KP, Stamm TA, Nell VP, Pflugbeil S, Aletaha D, Steiner G, Uffmann M, Smolen JS: Very recent onset rheumatoid arthritis: clinical and serological patient characteristics associated with radiographic progression over the first years of disease. Rheumatology (Oxford). 2007, 46: 342-349. 10.1093/rheumatology/kel237.
Bryl E, Vallejo AN, Weyand CM, Goronzy JJ: Down-regulation of CD28 expression by TNF-alpha. J Immunol. 2001, 167: 3231-3238.
Warrington KJ, Vallejo AN, Weyand CM, Goronzy JJ: CD28 loss in senescent CD4+ T cells: reversal by interleukin-12 stimulation. Blood. 2003, 101: 3543-3549. 10.1182/blood-2002-08-2574.
Pawlik A, Ostanek L, Brzosko I, Brzosko M, Masiuk M, Machalinski B, Szklarz BG: Therapy with infliximab decreases the CD4+CD28- T cell compartment in peripheral blood in patients with rheumatoid arthritis. Rheumatol Int. 2004, 24: 351-354. 10.1007/s00296-003-0374-4.
Bryl E, Vallejo AN, Matteson EL, Witkowski JM, Weyand CM, Goronzy JJ: Modulation of CD28 expression with anti-tumor necrosis factor alpha therapy in rheumatoid arthritis. Arthritis Rheum. 2005, 52: 2996-3003. 10.1002/art.21353.
Rizzello V, Liuzzo G, Brugaletta S, Rebuzzi A, Biasucci LM, Crea F: Modulation of CD4(+)CD28null T lymphocytes by tumor necrosis factor-alpha blockade in patients with unstable angina. Circulation. 2006, 113: 2272-2277. 10.1161/CIRCULATIONAHA.105.588533.
Davenport MP, Fazou C, McMichael AJ, Callan MF: Clonal selection, clonal senescence, and clonal succession: the evolution of the T cell response to infection with a persistent virus. J Immunol. 2002, 168: 3309-3317.
Masopust D, Vezys V, Usherwood EJ, Cauley LS, Olson S, Marzo AL, Ward RL, Woodland DL, Lefrançois L: Activated primary and memory CD8 T cells migrate to nonlymphoid tissues regardless of site of activation or tissue of origin. J Immunol. 2004, 172: 4875-4882.
Smeets TJ, Dolhain R, Miltenburg AM, de Kuiper R, Breedveld FC, Tak PP: Poor expression of T cell-derived cytokines and activation and proliferation markers in early rheumatoid synovial tissue. Clin Immunol Immunopathol. 1998, 88: 84-90. 10.1006/clin.1998.4525.
Chabaud M, Durand JM, Buchs N, Fossiez F, Page G, Frappart L, Miossec P: Human interleukin-17: a T cell-derived proinflammatory cytokine produced by the rheumatoid synovium. Arthritis Rheum. 1999, 42: 963-970. 10.1002/1529-0131(199905)42:5<963::AID-ANR15>3.0.CO;2-E.
Park H, Li Z, Yang XO, Chang SH, Nurieva R, Wang YH, Wang Y, Hood L, Zhu Z, Tian Q, Dong C: A distinct lineage of CD4 T cells regulates tissue inflammation by producing interleukin 17. Nat Immunol. 2005, 6: 1133-1141. 10.1038/ni1261.
Harrington LE, Hatton RD, Mangan PR, Turner H, Murphy TL, Murphy KM, Weaver CT: Interleukin 17-producing CD4+ effector T cells develop via a lineage distinct from the T helper type 1 and 2 lineages. Nat Immunol. 2005, 6: 1123-1132. 10.1038/ni1254.
van Bergen J, Thompson A, van der Slik A, Ottenhoff TH, Gussekloo J, Koning F: Phenotypic and functional characterization of CD4 T cells expressing killer Ig-like receptors. J Immunol. 2004, 173: 6719-6726.
Warrington KJ, Kent PD, Frye RL, Lymp JF, Kopecky SL, Goronzy JJ, Weyand CM: Rheumatoid arthritis is an independent risk factor for multi-vessel coronary artery disease: a case control study. Arthritis Res Ther. 2005, 7: R984-R991. 10.1186/ar1775.
Liuzzo G, Goronzy JJ, Yang H, Kopecky SL, Holmes DR, Frye RL, Weyand CM: Monoclonal T-cell proliferation and plaque instability in acute coronary syndromes. Circulation. 2000, 101: 2883-2888.
Nakajima T, Schulte S, Warrington KJ, Kopecky SL, Frye RL, Goronzy JJ, Weyand CM: T-cell-mediated lysis of endothelial cells in acute coronary syndromes. Circulation. 2002, 105: 570-575. 10.1161/hc0502.103348.
Kilic A, Onguru O, Tugcu H, Kilic S, Guney C, Bilge Y: Detection of cytomegalovirus and Helicobacter pylori DNA in arterial walls with grade III atherosclerosis by PCR. Pol J Microbiol. 2006, 55: 333-337.
Rahbar A, Söderberg-Naucler C: Human cytomegalovirus infection of endothelial cells triggers platelet adhesion and aggregation. J Virol. 2005, 79: 2211-2220. 10.1128/JVI.79.4.2211-2220.2005.
The authors would like to thank Dr Cecilia Söderberg-Naucler for helpful discussion in HCMV-related issues, Dr Florian Kern and Charlotte Tammik for providing the protocol and reagents for the HCMV reactivity assay, Eva Jemseby for organizing sampling, storage and administration of biomaterial, and Marianne Engström for technical support with the immunofluorescence microscopy stainings. This study was supported by Alex and Eva Wallstrom, Borje Dahlin, Tore Nilsson, Magn. Bergvall, Nanna Svartz, and Åke Wiberg Foundations, the Swedish Association againt Rheumatism, the Swedish Medical Association, the King Gustaf the V:s 80 year Foundation, the Swedish Research Council and the EU FP6 project, AutoCure LSHB CT-2006-018661, 2. This publication reflects only the author's views; the European Community is not liable for any use that may be made of the information herein.
The authors declare that they have no competing interests.
AERF was responsible for the study design, performed laboratory work (preparation of blood and synovial fluid samples, flow cytometry analyses, development, analyses of the immunofluorescence microscopy, and HCMV reactivity assays), statistical analyses, interpretation of the data, and drafted the manuscript. OS performed and interpreted data from in vitro stimulation assays as well as ACPA ELISAs of serum and synovial fluid. AATJ performed and analysed the immunofluorescence stainings. BN contributed to the clinical evaluation of the patient cohort together with EaK, who also performed the arthroscopies. AR carried out and evaluated the results from the HCMV ELISAs. NKB set up the flow cytometric assays for investigation of the CD244 expression. A-KU was responsible for the biobank of arthroscopic biopsies and participated in the development of immunofluorescence stainings. RvV contributed to the clinical evaluations of patients and manuscript preparation. VM and CT were the principle investigators and participated equally in the planning and coordination of the study, interpretation of data, and drafting the manuscript. All authors read and approved the final manuscript.
Vivianne Malmström and Christina Trollmo contributed equally to this work.