Background
Undifferentiated nasopharyngeal carcinoma (NPC) is associated with Epstein-Barr virus (EBV) infection, which has a high incidence in Southern China and Southeast Asia. Conventional therapy is often ineffective for NPC patients with late-stage disease [
1,
2]. Recently, immunotherapy has become a promising therapeutic option for various types of cancer with high immunogenicity, including NPC [
3‐
5]. The success of EBV-specific cytotoxic T lymphocyte (CTL) treatment has been reported in NPC. However, it has been difficult to obtain consistent results or stable clinical efficacy [
6‐
8]. One possibility is that immune-suppressive environments may be created in patients with NPC [
9‐
11]. Thus, a better understanding of the immune status of NPC patients, including the distribution of specific lymphocyte subsets and their functions, is crucial in developing more effective immunotherapy strategies.
CD8
+ T cells that express high levels of the transcription factors Eomes and T-bet are usually destined to develop into cytotoxic effector cells that produce interferon (IFN) γ, granzyme B and perforin, however, CD8
+ cells may also give rise to a regulatory lineage (Tcreg). The CD4
+Foxp3
+ regulatory T cells (Tregs), which have been recognized as a suppressor of antitumor immunity because of its natural suppressive effect on the proliferation and IL-2 secretion of naïve and effector T cells [
12,
13], but the distribution, generation, characteristics, and function of Tcregs in cancer remain poorly understood, as does their pathogenic antigen specificity. Furthermore, interleukin (IL)-17-producing CD8
+ T cells (Tc17 cells) have been identified in mice and humans, and their enrichment inside solid tumors has been reported [
14]. However, the generation and function of Tc17 cells in cancer remain largely uncharacterized.
In this study, we aimed to investigate the distribution, characterization, and generation of CD8+ Tcregs and Tc17 cells in NPC patients. We observed an increase of Tcregs and decrease of Tc17 cells from peripheral blood mononuclear cells (PBMCs) and an accumulation of Tcregs and Tc17 cells in tumor tissues from 21 NPC patients. The Tcreg subset expressed CC chemokine receptor 6 (CCR6), cytotoxic T lymphocyte antigen 4 (CTLA4), and glucocorticoid-induced tumor necrosis factor (TNF)-related (GITR) proteins at high levels, resulting in a Treg-like phenotype. The Tc17 cells expressed high levels of CCR6 and low levels of CTLA4 and GITR protein, and they contained a high proportion of cells secreting TNFα, which is a Th1 cytokine. Moreover, the Tcregs from the tumor-infiltrating lymphocytes (TILs) secreted high levels of IL-10 and IFNγ but low levels of IL-2, IL-4, TNFα, and IL-17, resulting in a Tr1-like cytokine profile; Tcregs from PBMCs, in contrast, secreted high levels of IL-10 and low levels of transforming growth factor β (TGFβ), IL-2, IFNγ, TNFα, and IL-17. In addition, there was a significantly higher percentage of IFNγ-secreting cells among the Tc17 cells from the TILs than among those from the PBMCs, and this was true of cells from both NPC patients and healthy donors. Furthermore, the Tcregs from NPC patients possessed a suppressive function to the proliferation of CD4+ naive T cells, which was mainly mediated by a cell-to-cell contact-dependent mechanism. IFNγ failed to impair the suppressive function of Tcregs in vitro. Collectively, these data suggest that, in addition to CD8+ cytolytic effector cells, Tcregs and Tc17 cells with diverse functions are present in NPC patients. Additionally, this is the first demonstration of the existence of EBV antigen-induced Tcregs in patients with NPC.
Materials and methods
Samples
Tumor biopsy tissues and blood samples were collected from 21 newly diagnosed patients with NPC in Sun Yat-Sen University Cancer Center between 2009 and 2010. The tissue samples were cut into pieces. In addition to pathological diagnosis, one portion was used to generate and expand TILs, and another portion was used for fluorescence-activated sorting (FACS) analysis. Prior to FACS analysis, cells were briefly cultured in low dose IL-2 (20 IU/ml) RPMI 1640 complete medium to obtain a sufficient number of lymphocytes. PBMCs were isolated from the blood samples of 21 patients with NPC and 21 age-matched healthy donors; the samples had been frozen for FACS analysis. This study was conducted in accordance with the Helsinki Declaration, with written informed consent provided by the patients and with approval from the Research Ethics Committee of the Sun Yat-Sen University Cancer Center. Written consent was also obtained from all healthy donors before their participation.
Generation of TILs and FACS analysis
Bulk TILs were isolated from the NPC biopsy specimens by mincing the tissue into small pieces and digesting with collagenase type IV. Cells were then cultured in RPMI 1640 medium that contained 10% human AB serum supplemented with L-glutamine, 2-mercaptoethanol, and recombinant human IL-2 (300 IU/ml) so as to generate T cells, as described previously [
15].
The expression of markers on T cells was investigated by FACS analysis after surface or intracellular staining with specific antibodies that were conjugated to different fluorescent dyes (eBioscience, San Diego, CA, USA). Intracellular staining for IL-17 and other cytokines was performed on T cells stimulated by phorbol12-myristate13-acetate (PMA) and ionomycin for 4 h in the presence of brefeldin A (10 μg/ml, Sigma-Aldrich). Intracellular cytokines and Foxp3 were detected using a fixation and permeabilization protocol and buffers that were purchased from eBioscience.
The proportion of T cells that were specific for HLA-A2-restricted epitopes in LMP1 and LMP2 were analyzed by staining with HLA-A2 tetramers. The tetramers were assembled with synthetic peptides that originated from LMP1 (YLQ QNWWTL) and LMP2 (LLW TLVVLL and GLG TLGAAI) (Guangzhou Taimo Corporation, Guangzhou, China). Aliquots of 0.5-1 × 106 cells were incubated at 4°C for 30 min in PBS that contained 1% fetal calf serum and 1 μg/ml phycoerythrin (PE)-labeled tetrameric complex. The samples were stained with anti-CD8-FITC and anti-Foxp3-APC antibodies and were then fixed in 0.5% paraformaldehyde for 20 min. For each sample, 105 cells were analyzed using an FC500 flow cytometer and CXP analysis software (Beckman Coulter, Inc., Fullerton, CA, USA).
Sorting and expansion of CD8+CD25+ Tcregs and suppression assay
CD8
+CD25
+ Treg cells from PBMCs or TILs were stained with anti-CD8 and anti-CD25 antibodies and were sorted by FACS (MoFlo XDP Cell Sorter; Beckman Coulter, Inc.). Proliferation assays were performed as described previously [
16]. In brief, 10
5 CD4
+ naïve T cells or CD8
+ effector T cells were labeled with 5- or 6-(N-Succinimidyloxycarbonyl)-3', 6'-O, O'-diacetylfluorescein (CSFE, Invitrogen) and co-cultured with CD8
+ Tregs at the indicated ratios. Cells were co-cultured for 5 days in 96-well round-bottom plates coated with human anti-CD3 (1 μg/ml), with or without the presence of anti-IL-10 or anti-IFNγ antibodies. The proliferation of CSFE-labeled CD4
+ naïve T cells was detected by FACS analysis. Transwell experiments were performed in 24-well plates using inserts with a pore size of 0.4 μm (Corning Gilbert Inc, Arizona, USA).
Statistical analysis
Numerical data were expressed as means ± standard error. Statistical differences between the means for the different groups were evaluated with SSPS 13.0 software using a one-way analysis of variance with the level of significance at P < 0.05.
Discussion
The development and progression of cancer are associated strongly with the unique immunosuppressive characteristics of the tumor microenvironment, regardless of the chronic inflammatory response and infiltrating inflammatory cells that are often produced around tumor tissue [
19‐
22]. The increase and accumulation of CD4
+ Tregs in circulating PBMCs and tumor tissues have been observed in many kinds of malignancy, including NPC [
23‐
26]. In a recent study, we showed by double immunohistochemical staining that there was a CD8
+Foxp3
+ TIL subset in NPC tissues
in vivo[
17].
In the present study, we showed that the percentage of CD8
+ Tcregs increased in both circulating PBMCs and TILs of NPC patients when compared with PBMCs from healthy individuals (Figure
1, Figure
2A and
2B). This indicates that the accumulation of Tcregs in tumor tissue not only results from their recruitment from the peripheral blood to tumor tissue but also from the induction of CD8
+ Tcreg precursor cells at the tumor site. As a consequence, this Tcreg subset should contain natural Tregs (nTregs) and induced Tregs (iTregs) together at tumor site. This hypothesis was supported by the following findings. First, the Tcregs in TILs expressed CD45RO and CD45RA, which implied that Tcregs contained both memory and naïve Tcreg cells. Second, the Tcregs in PBMCs showed high levels of expression of CCR6, a ligand of chemokine CCL20, which is usually overexpressed in the NPC tumor microenvironment and upregulated by the EBV-encoded LMP1 protein [
27,
28]. Thus, these cells had migrated to the tumor tissue. Third, the Tcregs from the TILs expressed an IFNγ
highIL-10
highTGFβ
lowIL-2
lowTNFα
lowIL-17
low cytokine secretion phenotype (Tr1-like cytokine profile) (Figure
3). Moreover, we found that the Tcreg subset also contained some IL-17-producing cells (approximately 10%) and that the Tcregs from TILs expressed a significantly higher level of IFNγ than those from PBMCs of patients and controls. These results indicate that Tcregs in TILs of patients with NPC were not stable and did secrete some proinflammatory cytokines, such as IL-17 and IFNγ.
Our data demonstrate that Tcregs from TILs of NPC patients can suppress the proliferation of CD4
+ naïve T cells and CD8
+ effector T cells
in vitro. This suppression was mainly mediated by cell-to-cell contact, and IFNγ did not affect the suppressive function of Tcregs in NPC (Figure
4). The results are supported by others' reports on the mechanism of suppression by Tcregs [
29‐
32], and they reveal unique functions for Tcregs in NPC tumor tissue. On one hand, Tcregs facilitate tumor growth by suppressing activated T cells; on the other hand, they secrete a large amount of the Th1 cytokine IFNγ, which inhibits tumor cell growth and promotes the differentiation of Th1 cells.
In recent years, attention has focused on the role of CD4
+ Th17 cells in solid tumors, but their function remains largely unclear. Some researchers have suggested that Th17 cells promote tumor growth through an IL-6/STAT3 pathway, up-regulation of IL-8, and induction of tumor angiogenesis [
33‐
35]. Others believe that Th17 cells have an antitumor function and that the number of Th17 cells is associated with a better outcome for cancer patients. Additionally, Th17 cells amplified adoptive CTL immunotherapy in one mouse model [
34,
35], and we have identified one CD4
+ Th17 clone from an NPC patient that could inhibit melanoma growth in a NOD/SCID mouse model (unpublished data). However, the role of Th17 cells in NPC remains poorly understood.
In sum, the present study is the first to investigate the distribution, generation, and function of Tc17 cells in NPC. We found that the proportion of Tc17 cells was reduced significantly in PBMCs when compared to TILs from NPC patients or to PBMCs from healthy donors (Figure
2C and
2D). The Tc17 cells in TILs expressed only CD45RO and not CD45RA (Figure
3A), indicating that this cell population was derived from memory cells and migrated from the peripheral blood. In addition, the high levels of expression of CCR6 in the Tc17 cells from PBMCs also indicate that these cells were able to migrate to tumor tissue. Therefore, the proportion of Tc17 cells from PBMCs was reduced compared to TILs from paired NPC patients or PBMCs from healthy individuals.
Tc17 cells expressed high levels of IL-17 and TNFα, intermediate levels of IL-10, and low levels of IL-2. Similar to Tcregs, Tc17 cells in the TILs but not in the PBMCs of patients with NPC expressed high levels of IFNγ (Figure
3C). This was consistent with a recent report of a similar cytokine profile for Tc17 cells in human liver cancer [
36]. Furthermore, other research groups have shown that Tc17 cells, after polarization
in vitro, can inhibit the growth of B16 tumors in mouse models by secreting IFNγ
in vivo[
14,
37]. Most Tc17 cells are derived from CD8
+ T cells that lacked the expression of T-bet and Eomes; however, the expression of T-bet and Eomes is important for IFNγ production and for the antitumor function of CD8
+ T cells, especially in TILs [
38]. We also found that in NPC patients, only Tc17 cells from TILs expressed high levels of IFNγ, which implied that Tc17 from TILs have a Th1 cell function and might have an antitumor function.
To address whether EBV antigens could induce Tcregs in NPC, we analyzed Tcregs specific for the EBV HLA-A2-restricted LMP1 and LMP2 epitopes by tetramer and Foxp3 staining. We identified CD8
+ T cells and Tcregs that were specific for the LMP1 epitopes LLW and YLQ and the LMP2 epitope GLG both in the PBMCs and TILs from NPC patients (Figure
5). The percentage of LLW-, YLQ-, and GLG-specific CD8
+ T cells and Tcregs was increased slightly in TILs as compared to PBMCs, but this increase was only significant for the LLW epitope antigen-specific CD8
+ T cells and the YLQ and GLG epitope antigen-specific Tcregs. These findings demonstrate that EBV epitope-specific CD8
+ T cells and Tcregs could home to or be induced in NPC tumor tissues, and some EBV epitope antigens, specifically YLQ and GLG, induced more antigen-specific Tcregs in tumor tissues than others. CD4
+ Tregs that are specific for the LAGE1 and ARTC1 tumor antigens have been identified in melanoma, and EBNA1 P
561-573 and P
607-619 peptide-specific CD4
+ Tregs have been identified in PBMCs from healthy donors [
39,
40]. These reports indicate that some antigens activate Tregs preferentially. In sum, the present study is the first to identify EBV epitopes that can induce antigen-specific CD8
+ Tcregs in PBMCs and TILs of NPC patients. Our results suggest that when EBV antigen- or peptide-specific CTL immunotherapy is established for NPC patients, antigen selection may affect clinical efficacy.
Competing interests
The authors declare that they have no competing interests.
Authors' contributions
Conceived and designed the experiments: JL, YXZ. Performed the experiments: JL, ZFH, GX, JH. Analyzed the data: JL, HZF, LMZ, CNQ. Contributed reagents/materials/analysis tools: HYM, FQ, HQM, QYC. Wrote the manuscript: JL, CNQ. All authors read and approved the final manuscript.