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CD4+CD25bright regulatory T cells (Treg) play an important role in cancer-mediated immunosuppression. We and others have previously shown that prostaglandin E2 (PGE2) and transforming growth factor beta (TGF-β) induce CD4+CD25brightFOXP3+Treg. Based on these studies, we investigated the requirement for PGE2 in Treg induction by TGF-β. TGF-β stimulation of human CD4+ T cells induced COX-2-dependent production of PGE2. PGE2-neutralizing antibody treatment significantly reduced the suppressive function of TGF-β-induced Treg (TGF-β-Treg) in vitro. TGF-β concentration measured in the plasma of non-small cell lung cancer (NSCLC) patients directly correlated with the frequency of circulating CD4+CD25brightFOXP3+T cells. Flow cytometry analysis showed increased FOXP3 expression in circulating CD4+CD25+HLA-DR- cells of lung cancer patients compared to control subjects. Immunohistochemical analysis revealed co-expression of TGF-β, COX-2, and FOXP3 in serial sections from resected lung tumor tissues. All together these observations suggest interplay between TGF-β and COX-2 in the induction of Treg activities. Interrupting TGF-β and PGE2 signaling may be important in therapeutic interventions that aim to limit Tregfunction in lung cancer.
Lung cancer is the leading cause of cancer-related mortality in the United States . There is limited understanding of how lung cancers evade host immunity . Increased trafficking of suppressor cells to the tumor site and tumor-induced differentiation of CD4+ T cells into CD4+CD25bright Treg have been well documented, and both may contribute to cancer-mediated immunosuppression [2-4].
Treg are required for resolution of immune responses and maintenance of self-tolerance . Treg can be induced by exposing CD4+ T cells to antigens or polyclonal activators in the presence of immunosuppressive cytokines, notably TGF-β or IL-10 [5-7]. Woo et al. reported an increased frequency of CD4+CD25bright T cells with a regulatory phenotype in peripheral blood lymphocytes (PBL) of lung cancer patients [8, 9]. Similar findings have been reported in other malignancies [10,11]. Additional studies have demonstrated an enrichment of Treg among tumor infiltrating lymphocytes (TILs) within the primary tumor and draining lymph nodes of patients with lung cancer and other neoplasms [12-14]. Accumulation of Treg in tumor-associated tissues has been associated with recurrence in early stage NSCLC . These findings suggest that Treg are operative in the inhibition of local anti-tumor immunity and promotion of cancer progression [13-15]. Thus, therapies aimed at targeting Treg function may improve anti-tumor immune responses [16,17].
Immunosuppressive cytokines, such as TGF-β, induce regulatory properties in conventional CD4+ T cells [18,19], contribute to maintenance of lymphocyte homeostasis [20-22], and play a role in tumorigenesis . TGF-β is highly expressed in the lungs of some individuals at risk for lung cancer . Moreover, abnormally high levels of TGF-β and loss of negative regulatory signaling in response to TGF-β have been described in lung cancer and were associated with enhanced tumorigenicity and reduced survival [25-27].
There is growing evidence to suggest an integral relationship between aberrant inflammation (COX-2/PGE2 pathway) and cancer-mediated immunosuppression (TGF-β induction of Treg) . We have previously described a novel pathway in which PGE2 stimulates the development of Treg in vitro and in vivo, suggesting tumor-derived COX-2 promotion of the Treg phenotype [29,30]. Here, we investigated the contribution of COX-2/PGE2 network in TGF-β induced Treg in patients with NSCLC.
Human CD4+ T cells were purified from enriched buffy-coat from healthy volunteers using the CD4+ T cell isolation kit (Miltenyi Biotech, Auburn, CA) and the AutoMACS cell sorter (Miltenyi Biotech), following the manufacturer's instructions. Briefly, PBL, obtained by Ficoll gradient separation, were depleted of monocytes by 2 h adherence to tissue culture flasks and incubated with CD4-conjugated microbeads (20μl/106 cells) for 15 minutes at 4° C prior to CD4+ T cell selection using the AutoMACS cell sorter. Alternatively, monocyte-depleted PBL were utilized as a source of CD4+ T cells. To generate human Treg in vitro, purified CD4+ T cells were pre-incubated for 6 days in X-Vivo 15 medium (BioWhittaker, Walkersville, MD) + 10% FBS + 1% human AB serum (Gemini, Woodland, CA) with TGF-β1 (1-5ng/ml, Peprotech, Rocky Hill, NY) in the presence of soluble anti-CD3 (1μg/ml, eBioscience, San Diego, CA) and anti-CD28 (2μg/ml, eBioscience), as previously described . Alternatively, phorbol myristate acetate (PMA) (20ng/ml, Sigma, St. Louis, MO) and ionomycin (1μg/ml, Sigma) were utilized for co-stimulation. In dose-response experiments, purified CD4+ T cells or monocyte-depleted PBL were stimulated with escalating concentration of TGF-β (1-10ng/ml) in the presence of co-stimulation, as described above. In some experiments, CD4+ T cells were pre-incubated with celecoxib (1μM, Pfizer, New York, NY) for 2 h prior to stimulation with TGF-β (1-3ng/ml) for 24-48 h.
PGE2 production was measured in culture-conditioned media from CD4+ T cells stimulated as described above, using a specific enzyme immunoassay (PGE2 EIA kit, Cayman Chemical, Ann Arbor, MI) according to manufacturer's instructions. The sensitivity of this assay was 15.6pg/ml. COX-2 expression in the cell lysates was analyzed using the TiterZyme® human COX -2 enzyme immunometric assay (EIA) kit (Assay Designs, Ann Arbor, MI) according to manufacturer's instructions. Briefly, non-stimulated or stimulated [soluble CD3 (1ug/ml, eBioscience) and CD28 (2ug/ml, eBioscience) antibodies] magnetic bead-purified CD4+ T cells (2.5×106) were incubated with or without TGF-β (3ng/ml) for 48 h. Cells were harvested and cell lysate was prepared, as previously described . The sensitivity of the COX-2 EIA was 0.249ng/ml.
We measured T cell proliferation by 5′bromo-2′-deoxyuridine (BrdU) ELISA (Roche Applied Science, Indianapolis, IN), as previously described , with some modifications. Briefly, magnetic bead-purified CD4+ T cells were cultured with (1-3ng/ml) or without TGF-β (diluent medium) for 6 days to generate functional Treg . TGF-β was washed off and cells were utilized in a standard proliferation assay. Untreated and TGF-β-treated CD4+ autologous T cells were cultured at a 1:1 ratio in 96-well plates coated with anti-CD3 (lμg/ml, eBioscience) antibody. In some experiments, IL-2 (100 U/ml, Proleukin, biological activity 18×106 International Units (IU)/1.1mg, Chiron Corporation, Emeryville, CA) was added to the proliferation assay. To neutralize PGE2 in the culture-conditioned media, anti-PGE2 antibody (1μg/ml, provided by J. Portanova, Searle, Saint Louis, MO) was added, with a mouse IgG isotype antibody (1μg/ml, Sigma) serving as the control. After five days incubation at 37° C and 5% CO2, the cells were pulsed with BrdU (100μM) and were assessed for BrdU incorporation 4 h later. Results are expressed as optical density (OD) at 405 nm.
PBL were obtained from 26 lung cancer patients from the Jonsson Comprehensive Cancer Center (JCCC), University of California, Los Angeles (UCLA) and from 26 healthy volunteers from the UCLA Blood Bank. Each individual signed an informed consent form approved by the UCLA Institutional Review Board (IRB). Table 1 shows the clinical-pathologic characteristics of each patient. Mononuclear cells (MNC) were isolated by density gradient sedimentation on Ficoll-Hipaque (Amersham Biosciences, Uppsala, Sweden), as previously described . The mononuclear cell fraction was collected from the interface, washed twice in RPMI 1640 (Cellgro, Me-diatech, Herndon, VA) and cryopreserved in 10% DMSO (Sigma) and 90% AB serum (Gemini) at -80°C until use. Blood samples were collected in Vacutainer CPT MDSU 8 ml tubes (BD Biosci-ence) containing 0.1ml of 1M sodium citrate anticoagulant (Fisher Scientific, Pittsburgh, PA) and plasma was separated by centrifugation at 1500xg at room temperature (RT) for 20 min, followed by immediate cryopreservation at -80° C.
We utilized 5-color flow cytometry to analyze CD4+ T cells. Briefly, cryopreserved PBL specimens from patients and controls were thawed and allowed to recover for 2 h in adult bovine serum (Omega Scientific, Tarzana, CA) at 37°C. For surface staining, cells (106) were labeled with fluorescein isothiocyanate (FITC)-conjugated CD25 (IgG2a, Miltenyi Biotech), HLA-DR PE-Texas red (ECD) (IgG1, Immunotech, Marseille, France), CD4+ peridinin-chlorophyll-protein complex (PerCP) (IgG1, BD Bioscience) and CD45RO allophycocyanin (APC) (IgG2a, BD Bioscience) for 20 min at RT in FACS buffer (PBS+2% fetal calf serum) (Cellgro and Gemini, respectively). Cells were fixed and permeabilized with 1× Fix/Perm buffer (1ml, eBioscience) for 1 h at 4°C. For intracellular staining, cells were incubated with phycoerithrin (PE)-conjugated anti-human FOXP3 antibody (20μl/106, clone PCH101, eBioscience) in the presence of 2% rat serum (Gemini) in permeabilization buffer for 30 min at 4°C. CD4-PerCP antibody and specific manufacturer-recommended isotype controls for the fluorochromes FITC, PE, APC and ECD were also utilized to establish the parameters of specific staining. Cell acquisition was performed using a BD FACSAria™ cell sorter (BD Biosciences Immunocytometry System, San Jose, CA). All events were acquired within a pre-set lymphocyte gate based upon the forward and side scatter properties of the target cell population. We acquired a minimum of 500,000 events within this pre-set T cell region to reach statistical significance. FACS DiVa version 2.1 (BD Biosciences) was utilized to analyze the percentage of CD25+ FOXP3+ HLA-DR+ T cells within both CD4+CD45RO+ and CD4+CD45RO− populations.
For quantitative real time analysis of FoxP3 mRNA expression, PBL were isolated by Ficoll gradient centrifugation, as described above. RNA was extracted and cDNAwas prepared with a kit from Invitrogen (Carlsbad, CA) according to the manufacturer's instructions. Human FoxP3 mRNA was quantified using the SYBR Green quantitative PCR kit (Finnzymes, Espoo, Finland) in the iCycler thermocycler (Bio Rad, Hercules, CA). Amplification was carried out in a 20 μl reaction volume for 40 cycles of 15 seconds at 95°C, 20 seconds at 60°C and 30 seconds at 72°C. Samples were run in triplicate, and their relative expression was determined by normalizing values for each target to human β-actin and then comparing this normalized value to the normalized expression in a reference sample to calculate a fold change. The primers for FoxP3 were: forward 5′-CAA GTT CCA CAA CAT GCG AC3′; reverse 5′-ATT GAG TGT CCG CTG CTT CT -3′. FoxP3 primers were synthesized by Integrated DNA Technologies (Coralville, IA). For β-actin, the primers were: forward 5′-GATGAGATTGGC ATGGCTTT-3′; reverse 5′-CACCTTCACCGTTCCAGTTT-3′.
Because TGF-β1 is the main isoform secreted by most immune cells, we utilized the human TGF-β1 ELISA kit (RayBio, Norcross, GA) to measure TGF-β1 in citrated plasma of lung cancer patients and healthy controls, following the manufacturer's protocol. To activate latent TGF-β1 to the immune reactive form, plasma samples were first acidified with 2.5M acetic acid and 10M urea (1:1) for 10 min at RT and then neutralized with equal volume of 1.2M NaOH and 0.5M HEPES (pH 7.76). The detection limit of the TGF-β1 ELISA is > 80pg/ml. TGF-β1 is referred as TGF-β throughout the manuscript.
Immunohistochemical analysis was performed on formalin-fixed, paraffin-embedded tissue sections of resected lung tumors obtained from the UCLA Lung Cancer SPORE tissue bank. Only stage I and stage II patients were included (n=12). Expression of TGF-β, COX-2 and FOXP3 was examined by single staining of serial sections. Briefly, tissue sections (4μm-thick) were de-paraffinized in xylene and rehydrated through graded alcohol and deionized water. For antigen retrieval, the sections were heated in 50mM Tris buffer containing 2mM EDTA (pH 9.0) for 20 min in a steamer and washed with PBS (Cellgro). Endogenous peroxidases were inactivated by incubation with methanol containing 3% hydrogen peroxide (Sigma) for 10 min, followed by a wash in PBS. To block nonspecific binding, the sections were treated with normal horse serum (Vector Laboratories, Bur-lingame, CA) for 30 min at RT. For FOXP3 staining, the tissue sections were incubated with mouse anti-human FOXP3 monoclonal antibody (Dr. Alison H. Banham, University of Oxford, UK) diluted 1:50 in PBS for 40 min at RT. These specimens were rinsed and incubated with horse anti-mouse IgG-biotin (7.5μg/ml, Vector Laboratories) for 40 min at RT. Samples were then incubated with avidin-HRP (Vector Laboratories) diluted 1:1000 in PBS for 30 min at RT, washed, and treated with 3,3′ diaminobenzidine (DAB substrate kit, Vector Laboratories) for brown color development. For COX-2, a tissue section from the same patient was incubated with goat anti-human COX-2 polyclonal IgG (1.0μg/ml, Santa Cruz Biotechnology, Santa Cruz, CA) for 1 h at 37°C, followed by incubation with horse anti-goat IgG-biotin (7.5μg/ml, Vector Laboratories) and by incubation with Vectastain ABC-alkaline phosphates kit (Vector Laboratories) for red color development. For TGF-β, a tissue section from the same patient was incubated with mouse anti-human TGF-β1 monoclonal antibody (Abcam, Cambridge, MA) diluted 1:2000 in PBS for 1 h at RT, incubated with horse anti-mouse IgG-biotin (7.5μg/ml) for 40 min at RT, followed by incubation with avidin-HRP diluted to 1:1000 in PBS for 40 min. Samples were washed and treated with DAB substrate kit for brown color development.
Mixed-effects analysis of variance (ANOVA) was used to compare outcome (e.g. PGE2 and COX-2) levels between experimental groups. These models contained terms for the experimental parameters (dose and time) as well as the interaction effect between these parameters. To account for the technical and experimental replicates of the assays, we included random effects terms for both in the ANOVA models. In cases where the experimental parameters were significant, we performed post-hoc comparisons between individual experimental conditions using two-tailed unpaired t-tests. Due to unequal replicate counts, we used the coefficients estimated in the ANOVA models to derive estimates for the group means and standard errors for each experimental condition across all replicates (Figure 1). The t-test was used to compare two-group experiments (Figures 3A, ,3C,3C, ,3D3D and Table 2). Simple linear regression was used to assess the relationship between TGF-β and CD4 percentage (Figure 3E). Statistical analyses were performed in SAS version 9 (SAS Institute, NC) and Graph Pad Prism 4 (version 4.0c) (San Diego, CA) software.
To determine the contribution of COX-2/PGE2 to TGF-β Treg activity, we first analyzed the time-and concentration-dependent production of PGE2 by human CD4+ T cells from healthy donors following stimulation with TGF-β. PGE2 production by PBL was most effectively enhanced by TGF-β stimulation at 0.5 and 1ng/ml (Figure 1A). Maximal PGE2 production was observed 48 h following stimulation with TGF-β (Figure 1B). In addition, TGF-β (1-3ng/ml) induced COX-2 expression in both non-activated and CD3/CD28-stimulated CD4+ T cells (Figure 1C). Celecoxib (luM) significantly inhibited the capacity of TGF-β to induce PGE2 production by CD4+ T cells (Figure 1D).
The functional implications of these findings were assessed by generating TGF-β-Treg from purified CD4+ T cells from healthy donors . The suppressive activity of TGF-β-Treg on autologous T cell proliferation was assessed in the presence or absence of neutralizing anti-PGE2 antibody. TGF-β-Treg significantly inhibited the proliferation of autologous T cells (Figure 2A). Importantly, the addition of anti-PGE2 antibody significantly diminished this TGF-β-Treg inhibitory function (Figure 2A). These findings suggest that PGE2 may contribute to TGF-β-Treg suppression of T cell proliferation. Because of the fundamental role of IL-2 and the IL-2 receptor, CD25, in Treg biology and function [31,32], we evaluated the impact of IL-2 on TGF-β-Treg suppressive activity in vitro. Exogenous IL-2 (100 IU) added to the proliferation assay did not revert the suppressive activity of TGF-β-Treg; indeed IL-2 inhibited the proliferative capacity of autologous T cells (Figure 2B).
The COX-2/PGE2 pathway has been implicated in promoting the Treg phenotype [29,30,33]. We analyzed circulating Treg in both NSCLC patients and healthy subjects by flow cytometry. The patient characteristics, tumor stage, and tumor histology are reported in Table 1. The frequency of circulating CD4+CD25bright T cells expressing FOXP3 was significantly elevated in NSCLC patients compared to healthy subjects (Figure 3A), in agreement with previous findings [8,9]. The mean fluorescence intensity (MFI) for FOXP3 expression was similar in CD4+CD25bright T cells from both control and cancer groups (2222 ± 7 and 2021 ± 7, respectively). Because specific subsets of memory Treg may be selectively activated in cancer [3,34], we analyzed the expression of Major Histocompatibility Complex (MHC) class II in naïve and memory CD4+CD25brightand CD4+CD25dim T cells from the PBL of healthy individuals and NSCLC patients. On a percentage basis, none of the indicated T cell subsets were differentially expressed in the control subjects versus lung cancer patients. Both CD45RO+ and CD45RO− T cells from lung cancer and healthy donors expressed similar levels of HLA-DR (17-20% and 9-11%, respectively). Interestingly, the MFI of FOXP3 was increased only in the HLA-DR− subsets of CD45RO+CD25brightand CD45RO−CD25dimT cells of lung cancer patients compared to the control subjects (6851 ± 357 versus 5579 ± 261 and 3030 ± 325 versus 1854 ± 271, respectively) (Table 2). Figure 3B shows a representative density plot from a healthy donor (B1) and a cancer patient (B2).
Mouse and human genetic studies have demonstrated a fundamental role for FoxP3 in the regulation of Treg development and function [35,36]. Mutations in the FoxP3 gene were linked to autoimmune manifestations observed in the Scurfy mouse and in humans affected by immune dysregulation, polyendocrinopathy, enteropathy, X-linked syndrome (IPEX) disease, and other conditions characterized by lack of functional Treg . However, FoxP3 is not always expressed in every type of Treg [5-7], and discrepancies between protein and gene expression profiles have been reported . Thus, we analyzed FoxP3 mRNA from individual PBL samples by RT-PCR analysis. FoxP3 mRNA levels were 2-fold higher in PBL from lung cancer patients compared to control subjects (Figure 3C), consistent with the increased frequency of CD4+CD25brightFOXP3+ T cells detected in the peripheral blood of the NSCLC patients (Figure 3A).
Several malignancies, including lung cancer, produce high levels of TGF-β [25,26,39], and, similar to PGE2, exogenous TGF-β promotes the development of Treg [18,19]. Thus, we measured TGF-β in the plasma of NSCLC patients and healthy donors and evaluated whether plasma TGF-β and frequency of circulating Treg were correlated (n=18). As shown in Figure 3D, plasma TGF-β concentrations were increased in NSCLC patients compared to healthy individuals and were significantly correlated with the frequency of circulating CD4+CD25brightT cells of NSCLC patients (r2=0.43, p≤ 0.003, Figure 3E).
As we previously reported, PGE2 induces CD4+CD25brightFOXP3+ Treg with characteristics of both naturally and acquired Treg function [29,30]. Similarly, TGF-β drives conventional CD4+ T cells toward the development of acquired Treg phenotypes [18,19]. In addition, TGF-β has been shown to increase COX-2 expression and PGE2 production in several cell types [21-23]. Based on these findings, we investigated the interplay between TGF-β and COX-2/PGE2 in Treg induction at the tumor site. Herein, we evaluated TGF-β, COX-2, and FOXP3 expression by immunohistochemical analysis of NSCLC tumor biopsies (n=16). Figure 4 shows representative tissue sections of lung adenocarcinoma from the same patient. In Figure 4A, a hematoxylin and eosin (H&E) stained section of lungadenocarcinoma shows blue-stained areas that represent a prominent lymphoid infiltrate (100×). In Figure 4B, the red-stained areas represent positive cytoplasmic staining for COX-2 expression (200×). In Figure 4C, FOXP3 is detected as brown nuclear staining within lymphocyte-enriched areas of the neoplasm (200×). In Figure 4D, brown-stained areas represent positive staining for TGF-β within the connective tissue (200×). These observations along with our previous findings support the interplay between TGF-β and COX-2 in the induction of Treg activities within the lung tumor microenvironment.
While Treg serve an essential maintenance role in self-tolerance, increased number of circulating Treg has been reported in several malignancies and correlated with poor outcome [3,13-15]. As such, Treg represent a potential therapeutic target in cancer therapy . However depletion strategies may not be sufficient, since Treg populations can be replenished by conversion of conventional CD4+CD25× T cells into CD4+CD25+ Treg by exposure to TGF-β or PGE2 whose interplay in Treg induction is the object of the present investigation [4,18,19,29,30].
Several malignancies secrete the immunosup-pressive cytokine TGF-β [25,39,42], and tumor-derived TGF-β can convert naturally occurring CD4+ T cells into CD4+CD25brightFOXP3+ Treg in a mouse model of pancreatic cancer . TGF-β has also been shown to induce COX-2/PGE2 expression in numerous epithelial cell types [21-23], and we have reported that tumor-derived COX-2/PGE2 favor the development of a Treg phenotype in human and mouse CD4+ T cells [29,30].
COX-2, the rate-limiting enzyme for the production of pro- and anti-inflammatory prostaglandins, plays an important role in cancer-related inflammation and progression [33,44]. Aberrant or increased expression of COX-2 and its major metabolite, PGE2, are found in several malignancies including NSCLC in which they promote metastatic development [33,44]. While COX-2/PGE2 and TGF-β are implicated in tumorigenesis via different mechanisms [33,39,42,44], both are capable of generating peripherally induced Treg [18,19,29,30].
In the present study, we found that TGF-β can induce competent Treg from human PBL through a mechanism dependent upon COX-2/PGE2 signaling. Specifically, TGF-β stimulated PGE2 production and COX-2 expression in both PBL and purified CD4+ T cells, and pharmacologic inhibition of COX-2 suppressed the TGF-β-induced PGE2 production. PBL or CD4+ T cells stimulated with TGF-β exhibited a Treg phenotype in vitro evidenced by their capacity to inhibit the proliferation of autologous CD4+ T cells. Inhibition of PGE2 significantly reduced the TGF-β-Treg immu-nosuppressive activity, suggesting the involvement of COX-2/PGE2 in the inhibitory function of TGF-β-Treg. Interestingly, high concentrations of IL-2 did not prevent the in vitro suppression of T cell proliferation mediated by TGF-β-Treg, but it did hamper the overall proliferation of autologous T cells. It is possible that IL-2 may have recruited Treg precursors present in the T cell population and encouraged their suppressive function [31,32]. Alternatively, IL-2 may operate by sensitizing activated T cells to undergo apoptosis .
Clearly, our results indicate that TGF-β can drive purified CD4+ T cells towards a regulatory phenotype through the COX-2-induced production of PGE2. This observation may have important implications. First, it offers us an explanation why NSCLC, and maybe other tumors, rely greatly on TGF-β, COX-2 and PGE2. While the signaling between these players may go in both directions, positively feeding forwards and backwards the neoplastic process, it ultimately results in tumor progression and down-regulation of the immune response [33,42,44]. Our findings also emphasize that any given T cell phenotype may not be as static as previously thought, but rather environmental factors can shape the T cell repertoire/balance in the periphery . Baecher-Allan et al.  identified a functionally distinct population of mature Treg based on expression of HLA-DR: 1) HLA-DR+ Treg acting via an early contact-dependent mechanism associated with FoxP3 induction, and 2) HLA-DR− Treg characterized by increased production of IL-10 and IL-4 and induction of late suppression of T cell proliferation. In the present study, FOXP3 was expressed at significantly elevated levels in the HLA-DR− population of both naive and memory CD4+CD25dim and CD4+ CD25brightT cell subsets in NSCLC patients compared to healthy donors. We hypothesize that HLA-DR- CD25bright FOXP3+ T cells may initially function via IL-10-mediated-suppression, then, following conversion into HLA-DR+ CD25bright FOXP3+T cells, via a cell-contact dependent mechanism. Functional studies are under way to elucidate the significance and the immunologic implications of these HLA-DR negative Foxp3+ T cell subsets.
The interplay between TGF-β, COX-2 and PGE2 is further illustrated by our clinical findings which showed increased frequency of peripheral CD4+CD25bright T cells in NSCLC patients which was correlated to high plasma levels of TGF-β and co-localization of COX-2, TGF-β and FOXP3 in resected NSCLC tissues.
Our findings support the evidence implicating a pathogenic interaction between dysregulated inflammation (COX-2/PGE2 pathway) and cancer-mediated immunosuppression (TGF-β induction of Treg). We hypothesize that elevated levels of TGF-β in the plasma or peri-tumoral stroma of NSCLC patients may promote the generation of Treg in part through COX-2/PGE2 signaling. Additional studies are warranted to clarify the interaction between TGF-β and COX-2/PGE2 in the induction of adaptive Treg. Defining the factors that contribute to Treg induction and understanding Treg suppression mechanisms may facilitate the development of new therapeutic strategies in lung cancer.
Flow cytometry was performed at the UCLA Jonsson Comprehensive Cancer for AIDS Research Flow Cytometry Core Facility that is supported by the National Institutes of Health awards CA-16042 and AI-28697, Jonsson Comprehensive Cancer Center, UCLA AIDS Institute, and David Geffen School of Medicine at UCLA.
This study was supported by the National Institutes of Health Grants R01 CA111851, UCLA Lung Cancer SPORE P50 CA90388, 5K12CA076095, and 1K23CA131577; UC Tobacco Related Research Program; Merit Review Research Funds from the Department of Veteran Affairs; Ronald Binder Memorial Fund for Lung Cancer Research; STOP Cancer; and Jonsson Cancer Foundation.