pERK-dependent defective TCR-mediated activation of CD4+ T cells in end-stage renal disease patients
Immunity & Ageingvolume 14, Article number: 14 (2017)
Patients with end-stage renal disease (ESRD) have an impaired immune response with a prematurely aged T-cell system. Mitogen-activated protein kinases (MAPKs) including extracellular signal-regulated kinase (ERK) and p38, regulate diverse cellular programs by transferring extracellular signals into an intracellular response. T cell receptor (TCR)-induced phosphorylation of ERK (pERK) may show an age-associated decline, which can be reversed by inhibiting dual specific phosphatase (DUSP) 6, a cytoplasmic phosphatase with substrate specificity to dephosphorylate pERK. The aim of this study was to assess whether ESRD affects TCR-mediated signaling and explore possibilities for intervening in ESRD-associated defective T-cell mediated immunity.
An age-associated decline in TCR-induced pERK-levels was observed in the different CD4+ (P < 0.05), but not CD8+, T-cell subsets from healthy individuals (HI). Interestingly, pERK-levels of CD4+ T-cell subsets from young ESRD patients were in between young and elderly HI. A differentiation-associated decline in TCR-induced ERK and p38 phosphorylation was observed in T cells, although TCR-induced p38 phosphorylation was not significantly affected by age and/or ESRD. Frequencies of TCR-induced CD69-expressing CD4+ T cells declined with age and were positively associated with pERK. In addition, an age-associated tendency of increased expression of DUSP6 was observed in CD4+ T cells of HI and DUSP6 expression in young ESRD patients was similar to old HI. Inhibition of DUSP6 significantly increased TCR-induced pERK-levels of CD4+ T cells in young and elderly ESRD patients, and elderly HI.
TCR-mediated phosphorylation of ERK is affected in young ESRD patients consistent with the concept of premature immunological T cell ageing. Inhibition of DUSP6 specific for pERK might be a potential intervention enhancing T-cell mediated immunity in ESRD patients.
ESRD patients have a defective T-cell mediated immune system that is clinically characterized by an increased risk of a variety of infections [1, 2] and impaired response of vaccination [3,4,5,6,7]. Infections are the second leading cause of mortality following cardiovascular disease and a major cause of morbidity in ESRD patients .
Uremia-associated T-cell defects closely resemble premature immunological T-cell ageing . ESRD patients have a discrepancy of 15–20 years between the immunological T-cell age and their chronological age . Declined thymic output, more differentiated memory T cells, T cells lacking co-stimulatory molecules like CD28, skewed T cell receptor (TCR) Vβ repertoire diversity and shorter telomere length are observed in ESRD patients compared to age-matched healthy individuals (HI) .
TCR-induced signaling mediates clonal (positive or negative) selection of thymocytes in the thymus and initiates T cell immune responses in the periphery, consisting of T cell proliferation and differentiation . The mitogen-activated protein kinase (MAPK) pathway is one of the major pathways induced upon TCR stimulation . Activation of MAPK is mediated by phosphorylation of MAPK and downregulated by MAPK phosphatase resulting in inactive MAPK . In particular, the extracellular signal-regulated kinase (ERK) pathway is one of the important MAPK pathways. Phosphorylation of ERK can reduce sensitivity of cells to apoptosis and promote cell proliferation . ERK activity controls the positive feedback loop in the TCR-induced activation cascade and reduced ERK activity affects signal strength and activation of T cells [16, 17]. Reduced phosphorylation of ERK is associated with decreased interleukin-2 (IL-2) production  and vice versa . Dual specific phosphatases (DUSPs) represents a family of phosphatases that dephosphorylate phosphor-threonine and phosphor-tyrosine residues on MAPK and that are pivotal regulators of MAPK activities. DUSP6 is a cytoplasmic phosphatase with substrate specificity to dephosphorylate pERK . Ageing is also associated with defective signaling pathways [21, 22]. Recently it was shown that decreased phosphorylation of ERK in naive CD4+ T cells from elderly HI was associated with more time to build up the required signaling strength following stimulation compared to those from young HI. This decreased phosphorylation of ERK can be overcome by inhibiting DUSP6 .
P38 is another pivotal protein in the MAPK pathway  and of interest with respect to age-related changes is T cell activation. Most stimuli, including engagement of TCR, costimulatory receptors, inflammation, stress, growth factors, as well as DNA damage induce phosphorylation of p38 by various pathways [24, 25]. Although phosphorylation of ERK and p38 from T cells share some upstream molecules after triggering of TCR, such as phosphorylation of CD3 zeta-chain associated protein kinase of 70 kDa (ZAP70) , they each have their unique upstream MAPK kinases (MKKs) . Highly differentiated CD4+ T cells lacking expression of CD28 are accumulated in elderly healthy individuals , patients with ESRD , following chronic viral infection , and also in patients suffering from autoimmune disease . Senescent CD27−CD28−CD4+ T cells employ an MKK-independent mechanism for phosphorylating p38 and depend on 5′ adenosine monophosphate-activated protein kinase (AMPK) and transforming growth factor-β-activated protein kinase 1(TAK1)-binding protein 1(TAB1) ex vivo .
Little is known as to how MAPK signaling pathways in ESRD patients. Understanding MAPK signaling in ESRD patients may increase knowledge about mechanisms of uremia-associated impaired T-cell mediated immunity and offer possibilities for intervention. Here, we demonstrate that TCR-induced phosphorylation of ERK, and not p38, in CD4+ T cells decreases with age and T cell differentiation. This pathway is specifically affected in young ESRD patients and at the level of elderly healthy individuals, compatible with the concept of premature immunological T cell ageing in patients with renal failure. In addition, inhibition of DUSP6 may offer a potential intervention for improving T-cell mediated immunity in ESRD patients.
In line with our previous studies, young and elderly patients groups were defined based on their chronological age [32, 33]. Twenty-four stable ESRD patients, defined as having a glomerular filtration rate of ≤15 ml/min with or without renal replacement therapy (RRT; i.e. dialysis) and 24 HI were included (Study population characteristics are described in Table 1) at the outpatient clinic. Patients with any clinical or laboratory evidence of acute bacterial or viral infection, malignancy, immunosuppressive drug treatment within 28 days prior to transplantation (except for glucocorticoids) were excluded. Lithium-heparinized blood was drawn of ESRD patients and healthy kidney donors. All individuals included gave informed consent and the local medical ethical committee approved the study (METC number: 2012–022). It was conducted according to the principles of Declaration of Helsinki and in compliance with International Conference on Harmonization/Good Clinical Practice regulations.
Peripheral blood mononuclear cells (PBMCs) were isolated from peripheral blood from HI and ESRD patients as described previously  and then cryopreserved for further analysis.
Phosphorylation-specific flow cytometry
PBMCs were stained with eFluor-450-labeled anti-CD7 (eBioscience, Vienna, Austria), allophycocyanin-Cy7 (APC-Cy7)-labeled anti-CD8 (BD, Erembodegem, Belgium), Brilliant Violet (BV)-510-labeled anti-CD16 (BD) and fluorescein isothiocyanate (FITC)-labeled anti-CCR7 (R&D system, Uithoorn, the Netherlands) for 30 min at room temperature. Then 1 million PBMCs/50 μl were prepared for stimulation by labeling cells with 20 μg/ml mouse anti-human CD3 (BD) and mouse anti-human CD28 (BD) each on ice for 20 min, followed by an incubation with goat-anti mouse IgG (BD) for cross-linking on ice for 20 min. Stimulation was initiated by transferring cells to a 37 °C water bath for 10 min. Cells were fixed using Cytofix (BD) at 37 °C for 10 min and then permeabilized in 70% methanol at -20 °C for 30 min. Subsequently, cells were stained with peridinin chlorophyll (PerCP)-labeled anti-CD4 (BD), phycoerythrin (PE)-Cy7-labeled anti-CD45RO (BioLegend, Uithoorn, Netherlands), PE-labeled anti-phospho-p38MAPK (pT180/pY182) (BD), and Alexa Fluor (AF) 647-labeled anti-phospho-ERK1/2 (pThr202/pTyr204) (BD). Phosphorylation was measured on a BD FACSCanto II flow cytometer (BD) and data were analyzed by Kaluza™ software (Beckman Coulter, Woerden, Netherlands). Median fluorescence intensity (MFI) of phosphorylated ERK or p38, generated by Kaluza™, were multiplied by 256 to make them comparable to the data analyzed by FACS Diva software (linear value instead of log-transformed value) (BD). The MFI obtained for anti-CD3/anti-CD28-stimulation were corrected by subtracting the MFI of the unstimulated condition.
CD69 and IL-2 measurement
PBMCs were either not or stimulated with anti-CD3/anti-CD28 T-cell expander beads (Invitrogen Dynal, Oslo, Norway) at different ratios, i.e. 1 cell / 0.1 bead, 1 cell / 0.5 bead, 1 cell / 1 bead for 6 h in human culture medium (HCM; RPMI-1640 with GlutaMAX, 10% heat-inactivated pooled human serum and 1% penicillin and streptomycin) (Lonza, Breda, Netherlands) with Golgistop (BD). Then cells were stained with AmCyan-labeled anti-CD3 (BD), Pacific Blue-labeled anti-CD4 (BD), APC-Cyanin 7 (APC-Cy7)-labeled anti-CD8 (BD), APC-labeled anti-CD45RO (BD) and PE-Cy7-labeled anti-CCR7 (R&D Systems) antibodies and a live–dead marker ViaProbe (7-aminoactinomycin D; 7AAD; BD). Upon fixation with FACS lysing solution (BD) and permeabilization using FACS permeabilizing solution 2 (BD), cells were stained intracellular using PE-labeled anti-CD69 (BD) and FITC-labeled anti-IL-2 (BD). Percentages CD69-expressing and IL-2 producing CD4+ T cell subsets were evaluated upon measuring the samples on a BD FACSCanto II flow cytometer (BD). Data were analyzed by Kaluza™ software (Beckman Coulter).
PBMCs were pre-incubated in HCM including 50 μM (E)-2-benzylidene-3-(cyclohexylamino)-2, 3-dihydro-1 H-inden-1-one (BCI) (Merck – Millipore, Amsterdam, Netherlands) at 37 °C for 1 h. BCI has been shown to be an inhibitor of DUSP6 and DUSP1 activity. PBMCs were subsequently washed 3 times and then stimulated by CD3/CD28 antibodies (as described previously) for 10 mins and then MFI of pERK of BCI-pretreated T cells was measured by Phosphorylation-specific flow cytometry as described previously.
PBMCs were stained with AmCyan-labeled anti-CD3 (BD), Pacific Blue-labeled anti-CD4 (BD), APC-Cy7-labeled anti-CD8 (Biolegend); APC-labeled anti-CD45RO (BD) and PE-Cy7-labeled anti-CCR7 (R&D Systems) antibodies and 7-AAD for 30 min at 4 °C. Upon fixation and permeabilization using Fix/Perm buffer (eBioscience), 1% bovine serum albumin (Zwijndrecht, Netherlands) was used to block Fc receptors. Then cells were further stained with AF647-labeled anti-DUSP6 (Santa Cruz Biotechnology, Heidelberg, Germany) and PE-labeled anti-DUSP1 (Santa Cruz Biotechnology) for 30 min at 4 °C. MFI of DUSP6 and DUSP1 was measured on a BD FACSCanto II flow cytometer (BD) and data were analyzed using FACS Diva software version 6.1.2 (BD).
Data were analyzed by Graphpad Prism 6 (GraphPad Software, CA, USA). Comparison between two groups (non-parametric data) were using Mann Whitney test. Comparison in multiple groups were using Friedman test followed by Dunn’s Multiple Comparison T test or repeated ANOVA test followed by Bonferroni’s multiple comparison test. Comparison between DUSP6-treated and non-treated conditions was done by Paired T- test. All reported P-values are two-sided and were considered statistically significant when P < 0.05.
The demographic and clinical characteristics of the study population are given in Table 1. Twelve patients were within the young group (age 22–44 years) and 12 patients belonged to the elderly group (age 66–78 years). Age- and cytomegalovirus (CMV)-matched HI, i.e. 13 young (age 21–40 years) and 11 elderly (age 65–74 years) HI were included for comparison. Approximately half of the ESRD patients received RRT (dialysis) with a median dialysis time of 22 months.
Decreased ERK phosphorylation in young ESRD patients
A typical flow cytometric example for analysis of ERK phosphorylation is given in Fig. 1. First, we compared phosphorylation of ERK and p38 between young and elderly HI or young and elderly ESRD patients. A significant age-related lower TCR-mediated phosphorylation of ERK was observed within all CD4+ T cell subsets from HI (Fig. 2a–d). For example, the median of MFI value of CD4+ phosphorylated ERK (pERK) was 658 in young HI, which was significantly higher than 535 in elderly HI (p = 0.015) (Fig. 2a). This trend consistently existed between young and elderly HI when we compared MFI value of pERK in CD4+ naive (median 722 vs. 612, p = 0.022) (Fig. 2b), CM (median 666 vs. 489, p = 0.021) (Fig. 2c) and EM subsets (517 vs. 364, p = 0.018) (Fig. 2d). Due to the almost absent EMRA subset within the CD4+ T cells, phosphorylation of ERK and p38 within this subset was not evaluated.
However, no significant differences in expression levels of pERK in total CD4+ T cells or the subsets were found comparing young and elderly ESRD patients (Fig. 2a–c &d). For example, the median (interquartile range)) MFI value of CD4+ pERK in young patients was 613 (490–664) and 541 (413–801) in elderly patients (p = 0.51). The median MFI value for CD4+ pERK in young patients was in between the MFI values of young HI 658 (485–1212)) and elderly HI (535 (305–620)) but did not significantly differ from either group (respectively p = 0.13 and p = 0.06). This age-associated decline in pERK was not found for CD8+ T cell subsets (Fig. 2e–h & i). In addition, an age-related decline in TCR-mediated phosphorylation of p38, was absent in CD4+ T cells (Fig. 3a–c & d) as well as CD8+ T cells (Fig. 3e–h & i) of both HI and ESRD patients. In conclusion, ESRD patients have a defective ERK, but not p38, phosphorylation in CD4+ T cells, that is independent of age and at a level similar to aged HI.
Phosphorylation of ERK is associated with T-cell differentiation status
Next, we compared phosphorylation of ERK and p38 within different T cell subsets to assess whether differentiation-associated effects exist in the study groups. In all groups, a gradual decrease in TCR-induced phosphorylation capacity was seen with increasing CD4+ T cell differentiation. Phosphorylation of ERK was highest in naive CD4+ T cells of young HI, followed by that in the CM and EM subsets of the memory compartment (Fig. 4a). Median MFI dropped from 722 to 666 and 517 in the naive, CM and EM T cell subset, respectively. Interestingly, in elderly HI as well as both groups of ESRD patients (Fig. 4b, c & d), pERK levels were still highest within naive CD4+ T cells compared to the more differentiated EM T cell subset, but the difference with that observed within CM T cells disappeared. ERK phosphorylation within CM is higher than that within the EM compartment in young and elderly HI (Fig. 4a & b), as well as in young patients (Fig. 4c), but not in elderly patients (Fig. 4d). Differences for the various CD8+ T-cell subsets with respect to TCR-mediated phosphorylation of ERK between naive and CM compartment, or between EM and EMRA were less outspoken and not significantly different in HI (Fig. 4e & f) and patients (Fig. 4g & h). Similar to ERK, phosphorylation of p38 showed a similar trend to decrease with increasing differentiation status but no significant decline in phosphorylation of p38 from naive to CM in CD4+ in HI and patients (Fig. 5a–c & d). In CD8+ T cells, p38 phosphorylation was decreased in highly differentiated EMRA compared to CM in HI and patients (Fig. 5e–g & h). In conclusion, a differentiation-associated decrease in anti-CD3/CD28-induced phosphorylation of ERK and p38 in T cells was present in HI and patients.
Auto-phosphorylation (baseline) of ERK was associated with ageing in HI and increased according to differentiation status in CD4+ T cells
Baseline phosphorylation of ERK (i.e. auto-phosphorylation) was significantly lower for total and naive CD4+T cells in young HI compared with elderly HI, however, this trend was not observed in patients (Fig. 6a & b). Baseline levels of pERK were significantly lower in the CD8+ memory compartment (CM, EM and EMRA) when comparing young to elderly HI, but no age-related differences were observed for patients (Fig. 6g, h & i). Baseline phosphorylation of ERK was lower in the naive CD4+ T cells when compared to CM and/or EM in HI (Fig. 7 a & b) and patients (Fig. 7c & d). Naive CD8+ T cells also had lower baseline pERK when compared to EMRA in elderly HI (Fig. 7f), CM and EM in young patients (Fig. 7g), and EM in elderly patients (Fig. 7h). Naive CD4+ T cells had lower baseline phosphorylated p38 compared to CM or EM in elderly HI (Additional file 1: Fig. S1b), and lower p38 phosphorylation compared to EM in young patients (Additional file 1: Figure S1c). In CD8+ T cells, p38 auto-phosphorylation in naive compartment was significantly lower than that of EMRA in young and elderly HI (Additional file 1: Figure S1e & f), but this trend was not observed in the patient population (Additional file 1: Figure S1 g & h). To summarize, an age- as well as differentiation-related increase in baseline levels of pERK was observed for CD4+ T cells.
Neither CMV-serostatus nor RRT significantly influenced ERK or p38 phosphorylation
CMV-seropositivity may promote immunological T-cell ageing and was therefore analyzed for its association with MAPK pathway activation. However, ERK or p38 phosphorylation within T cells showed no significant difference comparing CMV-seropositive individuals to their CMV- seronegative counterparts in healthy individuals and ESRD patients respectively (Additional file 1: Figure S2 & S3). Moreover, in ESRD patients, ERK or p38 phosphorylation was not significantly different between the patients receiving RRT (i.e. dialysis) and those without RRT (Additional file 1: Fig. S4 & S5). In conclusion, neither CMV-serostatus nor RRT significantly influenced TCR-stimulation induced phosphorylation of ERK or p38.
Age-related decline in anti-CD3/CD28-induced CD69-expressing CD4+ T cells positively associated with phosphorylation of ERK
A typical flow cytometric example for analysis of frequencies of CD69-expressing and IL-2 producing CD4+ T cells after CD3/CD28 stimulation was given in Additional file 1: Figure S6. Higher frequencies of CD69-expressing CD4+ T cells were observed in young HI compared to that in elderly HI when stimulated with different ratios of anti-CD3/CD28 beads to cells (Fig. 8a). This age-related decline in CD69-expressing cells was observed for naive CD4+ T cells in the healthy population at a ratio of 1:0.1 (Fig. 8b) and at 1:0.1 and 1:1 ratios for memory CD4+ T cells (Fig. 8c). Percentages of IL-2 producing CD4+ T cells did not reveal an age-associated decline in our study population (Fig. 8d, e & f). Percentages of CD69-expressing CD4+ T cells following stimulation with anti-CD3/CD28 beads (at ratios 1:0.5 and 1:1) were associated with ERK phosphorylation, presented as the fold increase in MFI dividing the MFI from stimulated samples by that of unstimulated samples (Fig. 8g). Percentages of IL-2 producing CD4+ T cells were not associated with pERK (Fig. 8h). In addition, frequencies of CD69-expressing CD4+ T cells were significantly higher in the naive subset compared to CM or EM (Fig. 8i). In short, an age-related decline in anti-CD3/CD28-induced percentages of CD69-expressing CD4+ T cells was observed and percentages of CD69-expressing CD4+ T cells were positively associated with phosphorylation of ERK.
BCI promoted TCR-mediated phosphorylation of ERK
BCI is known to inhibit DUSP6 but also decrease levels of DUSP1 (product document, Merck – Millipore). BCI did not significantly enhance phosphorylation of ERK in young HI; in contrast, in elderly HI and both young and elderly ESRD patients, the pERK level was significantly upregulated in all CD4+ T cell subsets pretreated with BCI compared to that without (Fig. 9a–c & d). The average fold increase in pERK levels in naive CD4+ T cell subsets were 3.8, 2.5, and 2.1 in elderly HI, young and elderly ESRD patients, respectively. This was not observed for CD8+ T cells (Additional file 1: Figure S7). In short, BCI promoted TCR-mediated phosphorylation of ERK in CD4+ T cells of both elderly HI as well as young and old ESRD patients.
DUSP6 and DUSP1 expression in CD4+ T cells
In an attempt to unravel whether effects of BCI on pERK levels were mediated by interfering with DUSP6 and/or DUSP1, we measured DUSP6 and DUSP1 levels within CD4+ T cells in a small fraction of our study cohort. Due to limited availability of materials only 10 HI (4 young and 6 elderly) and 9 ESRD patients (4 young and 5 elderly) could be included. A typical flow cytometric example for analysis of DUSP6 and DUSP1 is given in Additional file 1: Figure S8. An age-associated trend of increased levels of DUSP6 was noted for total and naive CD4+ T cells in HI (Fig. 10a & b). The opposite was present comparing young to old ESRD patients (Fig. 10a, b & c). Levels of DUSP6 in young ESRD patients were similar to old HI. Like observed for pERK, a significant differentiation-associated increase in DUSP6 levels was observed (Fig. 10 d). Interestingly, DUSP1 expression in CD4+ T cells was quite comparable between both young and elderly HI and patients (Fig. 10e, f, & g). To conclude, an age-related tendency of increased levels of DUSP6, but not DUSP1, was observed for HI. Moreover, DUSP6 expression was significantly associated with T-cell differentiation status in CD4+ T cells.
The main observation of this study was that TCR-mediated phosphorylation of ERK in CD4+ T cells of young patients was in between young and old HI. Phosphorylation of ERK decreased in highly differentiated T-cell subsets compared to naive T cells. This defective TCR-mediated phosphorylation was specific as it could be restored by addition of a DUSP6 inhibitor. TCR-induced p38 phosphorylation was comparable between ESRD patients and HI.
Beyond midlife, the immune system shows age-related features and its defensive capabilities becomes impaired . The uremia-associated inflammatory environment present in ESRD patients accelerates this age-related immune senescence process. In addition to declined thymic output, accumulation of highly differentiated T cells, short telomere length [10, 33, 36] and narrowed TCR-Vβ repertoire diversity , this study indicates that young ESRD patients also have a defective CD4+ TCR activation judging from the reduced capacity to phosphorylate ERK upon TCR-triggering. ERK activity is critical for TCR threshold calibration, as it controls positive feedback loops in TCR-induced activation . Reduced ERK activity impairs TCR signal strength and activation, and favors T cells with higher affinity to antigen to be activated, leading to a contracted immune response to a given antigen . The ERK phosphorylation upregulation of early activation marker CD69 on T cells ensures a proper inducing activation of T cells in the lymph node , and also play an important role in T cell proliferation  and IL-2 production [39, 40]. In addition, ERK activation impacts cellular apoptosis as it inhibits Fas-mediated apoptosis in T cells . Evaluating ERK phosphorylation is a valuable tool to study more upstream molecules in the defective T-cell mediated immune system from ESRD patients. T cells from rheumatoid arthritis (RA) patients exhibit several defects which can also be viewed as premature immunological ageing . However, ERK phosphorylation in CD4+ T cells of RA patients selectively increased . This increased ERK activation lowers the TCR threshold in T cells of RA patients to respond to self-antigens, which may partly explain the adaptive immune system of RA patients to exhibit abnormalities that go beyond the local inflammatory response in the synovium .
DUSP6 is a cytoplasmic phosphatase with substrate specificity for phosphorylated ERK. In elderly individuals, silencing of DUSP6 increased the expression of T cell activation markers, such as CD69 and CD25, IL-2 production as well as proliferative response . Inhibition of DUSP6 could be a potential intervention to increase CD4+ TCR-sensitivity by enhancing ERK phosphorylation in ESRD patients. BCI (an inhibitor of DUSP6 and 1) enhanced TCR-induced pERK in CD4+ T cells from elderly HI, young and elderly ESRD patients, but not young HI, implying a role for DUSP6 and/or DUSP1 in regulation of ERK phosphorylation. Based on the age- as well as differentiation-related expression of DUSP6, but not DUSP1, in our HI, a potential role for DUSP6 may be present in defective TCR-induced ERK phosphorylation, especially in elderly HI and young patients. This needs to be confirmed in a larger cohort. Furthermore, use of siRNA specific for DUSP6 is required to draw a more definite conclusion with respect to the role of DUSP6 in defective TCR-induced phosphorylation of ERK in ESRD patients. The lack of age-related effects on pERK in CD8+ T cells of ESRD patients and HI, the latter confirming observations done by another study , as well as absence of effects of BCI on pERK levels in CD8+ T cells, indicates a different role for DUSP6 in CD8+ T cells compared to CD4+ T cells. We did not observe an association between DUSP6 expression and ERK phosphorylation in CD4+ T cells in ESRD patients. This could be due to the small cohort size or imply other DUSPs (e.g. 2, 4 or 5) [45,46,47,48,49] or upstream signaling molecules to contribute to this defective TCR-induced ERK phosphorylation in ESRD patients.
ERK over-phosphorylation might be as bad as defective ERK phosphorylation. ERK over-activation from kidney cells occurs in the physiologic setting in some chronic kidney diseases, such as compensatory kidney hypertrophy and in pathologic conditions for example glomerular disease . Increased ERK phosphorylation in T cells predisposes for autoimmunity for example rheumatoid arthritis . Over-expression of DUSP6 is also reported to impair T-cell function in chronic viral infections such as hepatitis C virus infection . Therefore, more research is warranted evaluating inhibition of DUSP in the setting of defective T-cell mediated immunity in ESRD patients.
We analyzed the effect of latency for CMV as it represents chronic antigenic stimulation of T cells, but ERK- or p38-activation of CD4+ or CD8+ T cells was not different between the CMV-IgG seropositive population and CMV-IgG seronegative population following CD3/CD28 stimulation. Highly differentiated memory CD4+ and CD8+ T cells may accumulate in CMV seropositive individuals and are functional CMV-specific T cells [29, 52, 53]. The results of our study show that non-specific TCR stimulation does not identify a defect p38 and ERK signaling associated with CMV seropositivity. In accordance with the results of a previous study, uremia is the major determinant affecting MAPK pathway parameters in ESRD patients and not RRT [9, 11, 33].
In the present study, we induced phosphorylation of p38 in T cells via triggering CD3  and CD28 . Lack of CD28 may only partly explain the decreased p38 activation in more differentiated CD4+ T cells. In addition to that, senescent human CD27−CD28− CD4+ T cells lack several essential upstream components including ZAP70 and the loss of TCR signaling machinery in those cells was associated with a defective calcium influx , which may indicate the decreased response of TCR-mediated activation in the more differentiated T cells. Interestingly, in contrast to the p38 activation following CD3/CD28 stimulation, baseline levels (spontaneous phosphorylation) of p38 increased during T cells differentiation . This might be caused by DNA damage in these more differentiated T cells and mediated by TAB1 (MKK-independent molecule), a key molecule involved in this auto-phosphorylation .
We have described for the first time a uremia-mediated defect in TCR-induced phosphorylation of ERK which may contribute to the impaired T-cell mediated immune response in ESRD patients. Inhibition of DUSP6 specific for pERK can restore defective p-ERK-mediated activation of CD4+ T cells in ESRD patients.
5′ adenosine monophosphate-activated protein kinase
(E)-2-benzylidene-3-(cyclohexylamino)-2, 3-dihydro-1 H-inden-1-one
Dual specific phosphatase
Highly differentiated effector T cells
Extracellular signal-regulated kinase
End-stage renal disease
Human culture medium
mitogen-activated protein kinases
Median fluorescence intensity
Peripheral blood mononuclear cells
Phosphorylation of ERK
Renal replacement therapy
TAK1-binding protein 1
Transforming growth factor-β-activated protein kinase 1
T cell receptor
CD3 zeta-chain associated protein kinase of 70 kDa
Dalrymple LS, Go AS. Epidemiology of acute infections among patients with chronic kidney disease. Clin J Am Soc Nephrol. 2008;3(5):1487–93.
Betjes MG. Immune cell dysfunction and inflammation in end-stage renal disease. Nat Rev Nephrol. 2013;9(5):255–65.
Eleftheriadis T, Antoniadi G, Liakopoulos V, Kartsios C, Stefanidis I. Disturbances of acquired immunity in hemodialysis patients. Semin Dial. 2007;20(5):440–51.
Janus N, Vacher LV, Karie S, Ledneva E, Deray G. Vaccination and chronic kidney disease. Nephrol Dial Transplant. 2008;23(3):800–7.
Fabrizi F, Martin P. Hepatitis B vaccine and dialysis: current issues. Int J Artif Organs. 2001;24(10):683–94.
Remschmidt C, Wichmann O, Harder T. Influenza vaccination in patients with end-stage renal disease: systematic review and assessment of quality of evidence related to vaccine efficacy, effectiveness, and safety. BMC Med. 2014;12:244.
Principi N, Esposito S, Group EVS. Influenza vaccination in patients with end-stage renal disease. Expert Opin Drug Saf. 2015;14(8):1249–58.
Sarnak MJ, Jaber BL. Mortality caused by sepsis in patients with end-stage renal disease compared with the general population. Kidney Int. 2000;58(4):1758–64.
Betjes MG, Litjens NH. Chronic kidney disease and premature ageing of the adaptive immune response. Curr Urol Rep. 2015;16(1):471.
Betjes MG, Langerak AW, van der Spek A, de Wit EA, Litjens NH. Premature aging of circulating T cells in patients with end-stage renal disease. Kidney Int. 2011;80(2):208–17.
Meijers RW, Litjens NH, de Wit EA, Langerak AW, van der Spek A, Baan CC, et al. Uremia causes premature ageing of the T cell compartment in end-stage renal disease patients. Immun Ageing. 2012;9(1):19.
Cantrell DA. T-cell antigen receptor signal transduction. Immunology. 2002;105(4):369–74.
Smith-Garvin JE, Koretzky GA, Jordan MS. T cell activation. Annu Rev Immunol. 2009;27:591–619.
Johnson GL, Lapadat R. Mitogen-activated protein kinase pathways mediated by ERK, JNK, and p38 protein kinases. Science. 2002;298(5600):1911–2.
Mebratu Y, Tesfaigzi Y. How ERK1/2 activation controls cell proliferation and cell death: is subcellular localization the answer? Cell Cycle. 2009;8(8):1168–75.
Li G, Yu M, Lee WW, Tsang M, Krishnan E, Weyand CM, et al. Decline in miR-181a expression with age impairs T cell receptor sensitivity by increasing DUSP6 activity. Nat Med. 2012;18(10):1518–24.
Altan-Bonnet G, Germain RN. Modeling T cell antigen discrimination based on feedback control of digital ERK responses. PLoS Biol. 2005;3(11):e356.
Liu B, Carle KW, Whisler RL. Reductions in the activation of ERK and JNK are associated with decreased IL-2 production in T cells from elderly humans stimulated by the TCR/CD3 complex and costimulatory signals. Cell Immunol. 1997;182(2):79–88.
Kogkopoulou O, Tzakos E, Mavrothalassitis G, Baldari CT, Paliogianni F, Young HA, et al. Conditional up-regulation of IL-2 production by p38 MAPK inactivation is mediated by increased Erk1/2 activity. J Leukoc Biol. 2006;79(5):1052–60.
Ekerot M, Stavridis MP, Delavaine L, Mitchell MP, Staples C, Owens DM, et al. Negative-feedback regulation of FGF signalling by DUSP6/MKP-3 is driven by ERK1/2 and mediated by Ets factor binding to a conserved site within the DUSP6/MKP-3 gene promoter. Biochem J. 2008;412(2):287–98.
Bignon A, Regent A, Klipfel L, Desnoyer A, de la Grange P, Martinez V, et al. DUSP4-mediated accelerated T-cell senescence in idiopathic CD4 lymphopenia. Blood. 2015;125(16):2507–18.
Moro-Garcia MA, Alonso-Arias R, Lopez-Larrea C. Molecular mechanisms involved in the aging of the T-cell immune response. Curr Genomics. 2012;13(8):589–602.
Shiryaev A, Moens U. Mitogen-activated protein kinase p38 and MK2, MK3 and MK5: menage a trois or menage a quatre? Cell Signal. 2010;22(8):1185–92.
Ashwell JD. The many paths to p38 mitogen-activated protein kinase activation in the immune system. Nat Rev Immunol. 2006;6(7):532–40.
Yan M, Dai T, Deak JC, Kyriakis JM, Zon LI, Woodgett JR, et al. Activation of stress-activated protein kinase by MEKK1 phosphorylation of its activator SEK1. Nature. 1994;372(6508):798–800.
Salvador JM, Mittelstadt PR, Guszczynski T, Copeland TD, Yamaguchi H, Appella E, et al. Alternative p38 activation pathway mediated by T cell receptor-proximal tyrosine kinases. Nat Immunol. 2005;6(4):390–5.
Weng NP, Akbar AN, Goronzy J. CD28(−) T cells: their role in the age-associated decline of immune function. Trends Immunol. 2009;30(7):306–12.
Betjes MG, Huisman M, Weimar W, Litjens NH. Expansion of cytolytic CD4+CD28- T cells in end-stage renal disease. Kidney Int. 2008;74(6):760–7.
Fletcher JM, Vukmanovic-Stejic M, Dunne PJ, Birch KE, Cook JE, Jackson SE, et al. Cytomegalovirus-specific CD4+ T cells in healthy carriers are continuously driven to replicative exhaustion. J Immunol. 2005;175(12):8218–25.
Pawlik A, Ostanek L, Brzosko I, Brzosko M, Masiuk M, Machalinski B, et al. The expansion of CD4+CD28- T cells in patients with rheumatoid arthritis. Arthritis Res Ther. 2003;5(4):R210–3.
Lanna A, Henson SM, Escors D, Akbar AN. The kinase p38 activated by the metabolic regulator AMPK and scaffold TAB1 drives the senescence of human T cells. Nat Immunol. 2014;15(10):965–72.
Huang L, Langerak AW, Wolvers-Tettero IL, Meijers RW, Baan CC, Litjens NH, et al. End stage renal disease patients have a skewed T cell receptor Vbeta repertoire. Immun Ageing. 2015;12:28.
Huang L, Langerak AW, Baan CC, Litjens NH, Betjes MG. Latency for cytomegalovirus impacts T cell ageing significantly in elderly end-stage renal disease patients. Clin Exp Immunol. 2016;186(2):239–48.
Litjens NH, Huisman M, Baan CC, van Druningen CJ, Betjes MG. Hepatitis B vaccine-specific CD4(+) T cells can be detected and characterised at the single cell level: limited usefulness of dendritic cells as signal enhancers. J Immunol Methods. 2008;330(1–2):1–11.
Moro-Garcia MA, Alonso-Arias R, Lopez-Larrea C. When aging reaches CD4+ T-cells: phenotypic and functional changes. Front Immunol. 2013;4:107.
Betjes MG, Meijers RW, Litjens NH. Loss of renal function causes premature aging of the immune system. Blood Purif. 2013;36(3–4):173–8.
Shaw AS. How T cells ‘find’ the right dendritic cell. Nat Immunol. 2008;9(3):229–30.
Sharrocks AD. Cell cycle: sustained ERK signalling represses the inhibitors. Curr Biol. 2006;16(14):R540–2.
Koike T, Yamagishi H, Hatanaka Y, Fukushima A, Chang JW, Xia Y, et al. A novel ERK-dependent signaling process that regulates interleukin-2 expression in a late phase of T cell activation. J Biol Chem. 2003;278(18):15685–92.
Tsukamoto H, Irie A, Nishimura Y. B-Raf contributes to sustained extracellular signal-regulated kinase activation associated with interleukin-2 production stimulated through the T cell receptor. J Biol Chem. 2004;279(46):48457–65.
Holmstrom TH, Schmitz I, Soderstrom TS, Poukkula M, Johnson VL, Chow SC, et al. MAPK/ERK signaling in activated T cells inhibits CD95/Fas-mediated apoptosis downstream of DISC assembly. EMBO J. 2000;19(20):5418–28.
Goronzy JJ, Weyand CM. Thymic function and peripheral T-cell homeostasis in rheumatoid arthritis. Trends Immunol. 2001;22(5):251–5.
Singh K, Deshpande P, Pryshchep S, Colmegna I, Liarski V, Weyand CM, et al. ERK-dependent T cell receptor threshold calibration in rheumatoid arthritis. J Immunol. 2009;183(12):8258–67.
Cope AP. T cells in rheumatoid arthritis. Arthritis Res Ther. 2008;10 Suppl 1:S1.
Mandl M, Slack DN, Keyse SM. Specific inactivation and nuclear anchoring of extracellular signal-regulated kinase 2 by the inducible dual-specificity protein phosphatase DUSP5. Mol Cell Biol. 2005;25(5):1830–45.
Caunt CJ, Armstrong SP, Rivers CA, Norman MR, McArdle CA. Spatiotemporal regulation of ERK2 by dual specificity phosphatases. J Biol Chem. 2008;283(39):26612–23.
Cagnol S, Rivard N. Oncogenic KRAS and BRAF activation of the MEK/ERK signaling pathway promotes expression of dual-specificity phosphatase 4 (DUSP4/MKP2) resulting in nuclear ERK1/2 inhibition. Oncogene. 2013;32(5):564–76.
Caunt CJ, Keyse SM. Dual-specificity MAP kinase phosphatases (MKPs): shaping the outcome of MAP kinase signalling. FEBS J. 2013;280(2):489–504.
Ferguson BS, Nam H, Stephens JM, Morrison RF. Mitogen-dependent regulation of DUSP1 governs ERK and p38 signaling during early 3T3-L1 Adipocyte differentiation. J Cell Physiol. 2016;231(7):1562–74.
Feliers D, Kasinath BS. Erk in kidney diseases. J Signal Transduct. 2011;2011:768512.
Li GY, Zhou Y, Ying RS, Shi L, Cheng YQ, Ren JP, et al. Hepatitis C virus-induced reduction in miR-181a impairs CD4(+) T-cell responses through overexpression of DUSP6. Hepatology. 2015;61(4):1163–73.
Labalette M, Salez F, Pruvot FR, Noel C, Dessaint JP. CD8 lymphocytosis in primary cytomegalovirus (CMV) infection of allograft recipients: expansion of an uncommon CD8+ CD57- subset and its progressive replacement by CD8+ CD57+ T cells. Clin Exp Immunol. 1994;95(3):465–71.
Lachmann R, Bajwa M, Vita S, Smith H, Cheek E, Akbar A, et al. Polyfunctional T cells accumulate in large human cytomegalovirus-specific T cell responses. J Virol. 2012;86(2):1001–9.
Dodeller F, Schulze-Koops H. The p38 mitogen-activated protein kinase signaling cascade in CD4 T cells. Arthritis Res Ther. 2006;8(2):205.
Di Mitri D, Azevedo RI, Henson SM, Libri V, Riddell NE, Macaulay R, et al. Reversible senescence in human CD4+CD45RA+CD27- memory T cells. J Immunol. 2011;187(5):2093–100.
The research was supported by the China Scholarship Council for funding PhD fellowship to Ling Huang (File No. 201307720043).
Availability of data and materials
The datasets generated and/or analyzed during the current study are not publicly available as it concerns patient data, but are available from the corresponding author on reasonable request.
LH participated in design the study, performed the experiments, analyzed the data and wrote the manuscript. NK participated in establishing the experiment protocol and revised the manuscript. MK conducted some experiments and interpreted part of the data. CB participated in design of the study and revised the manuscript. NL and MB designed the study, interpreted the data and revised the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
All individuals included gave informed consent and the Erasmus medical center medical ethical committee approved the study (METC number: 2012–022). It was conducted according to the principles of Declaration of Helsinki and in compliance with International Conference on Harmonization/Good Clinical Practice regulations.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Auto-phosphorylation (baseline) of p38 according to T cell differentiation status in healthy individuals (HI) and end stage renal disease (ESRD) patients. Figure S2. CMV-effects on phosphorylation of ERK in T cells subsets of healthy individuals (HI) and end stage renal disease (ESRD) patients. Figure S3. CMV-effects on phosphorylation of p38 in T cells subsets of healthy individuals (HI) and end stage renal disease (ESRD) patients. Figure S4. Effects of renal replacement therapy (RRT) on phosphorylation of ERK in T cells subsets of end stage renal disease (ESRD) patients with and without dialysis. Figure S5. Effects of renal replacement therapy (RRT) on phosphorylation of p38 in T cells subsets of end stage renal disease (ESRD) patients with and without dialysis. Figure S6. Typical example of the gating strategy for analysis of percentages of CD69+ CD4+ T cell subsets. Figure S7. Phosphorylation of ERK in CD8+ T cell subsets without and with BCI treatment from healthy individuals (HI) and end stage renal disease (ESRD) patients. Figure S8. Typical example of the gating strategy for analysis of DUSP6 and DUSP1 expression in CD4+ T cell subsets. (PDF 643 kb)