- Research article
- Open Access
Direct and indirect effects of retinoic acid on human Th2 cytokine and chemokine expression by human T lymphocytes
BMC Immunologyvolume 7, Article number: 27 (2006)
Vitamin A (VA) deficiency induces a type 1 cytokine response and exogenously provided retinoids can induce a type 2 cytokine response both in vitro and in vivo. The precise mechanism(s) involved in this phenotypic switch are inconsistent and have been poorly characterized in humans. In an effort to determine if retinoids are capable of inducing Th2 cytokine responses in human T cell cultures, we stimulated human PBMCs with immobilized anti-CD3 mAb in the presence or absence of all-trans retinoic acid (ATRA) or 9-cis-RA.
Stimulation of human PBMCs and purified T cells with ATRA and 9-cis-RA increased mRNA and protein levels of IL-4, IL-5, and IL-13 and decreased levels of IFN-γ, IL-2, IL-12p70 and TNF-α upon activation with anti-CD3 and/or anti-CD28 mAbs. These effects were dose-dependent and evident as early as 12 hr post stimulation. Real time RT-PCR analysis revealed a dampened expression of the Th1-associated gene, T-bet, and a time-dependent increase in the mRNA for the Th2-associated genes, GATA-3, c-MAF and STAT6, upon treatment with ATRA. Besides Th1 and Th2 cytokines, a number of additional proinflammatory and regulatory cytokines including several chemokines were also differentially regulated by ATRA treatment.
These data provide strong evidence for multiple inductive roles for retinoids in the development of human type-2 cytokine responses.
An uncommitted precursor T helper (pTh) cell can be induced to differentiate into at least two distinct subsets of effector cells, T helper type 1 (Th1) and T helper type 2 (Th2) cells [1, 2]. Th1 cells secrete IFN-γ, TNF-α, and TNF-β and are important for the development of delayed type hypersensitivity (DTH) reactions and protective responses to intracellular pathogens [1, 2]. These cells also contribute to the pathology of autoimmune disease and graft rejection. Th2 cells express and secrete IL-4, IL-5, and/or IL-13 and are essential for the development of humoral and allergic reactions [1, 2]. During T cell activation, the relative cytokine milieu within the local microenvironment is a major determinant of the direction of pTh cell differentiation. Cytokines such as IL-12 and to a lesser extent IFN-γ directly induce pTh cell differentiation into type 1 cells . In contrast, IL-4 stimulates pTh cell differentiation into type 2 cells even in the presence of moderate levels of IL-12 and IFN-γ . In addition to IFN-γ, IL-12 and IL-4, recent evidence also suggests an important role for cytokines such as IFN-(, IL-1α/β, IL-15, and IL-18 in stimulating type 1 responses  and IL-10 and IL-13 in stimulating type 2 responses [1, 3]. Additional factors including hormones, growth factors and co-stimulatory molecules have also been shown to influence T cell development of type 1 or type 2 responses .
Vitamin A (VA) or VA-like analogs known as retinoids, are potent hormonal modifiers of rodent type 1 or type 2 responses but a definitive description of their mechanism(s) of action is lacking [4–16]. Several early studies using models of pathogen-challenged rodents indicated that VA deficiency induced a dominant Th1 response that interfered with the development of a protective humoral response . These researchers proposed several potential mechanisms to account for these observations including the direct downregulation of T cell IFN-γ synthesis, direct promotion of Th2-cell differentiation, and/or alteration of accessory or antigen presenting cell function toward a Th2-inducing phenotype . Recent evidence from interventional studies show that VA supplementation of VA-deficient infants and children reduces morbidity and/or mortality from measles, malaria, and certain forms of diarrhea . These studies have stimulated renewed interest in elucidating VA's role in the immune response, particularly in modification of human Th1 or Th2 response development.
There are a number of contradictory findings in the literature examining the effects of retinoids on type 1 and 2 cytokine production in rodent models and cells. Several reports using murine and rat models of VA deficiency have demonstrated diminished type 1 reactions including DTH and anti-viral responses [7, 19–21]. Exogenous administration of VA or RA have also been shown to increase DTH reactions and augment immune responses to viruses suggesting that these compounds potentiate type 1 reactions [21, 22]. Several additional published studies using in vitro and in vivo systems of VA or retinoid deficiency and rodents and humans have also demonstrated either inhibitory, stimulatory or no effects on IFN-γ production [4–15, 23, 24]. As for Th2 cytokines, to date only one study has described a decrease in IL-4 production in VA deficiency , while several recent studies have demonstrated that retinoids induce IL-4 synthesis during in vitro murine T cell activation [9, 25, 26]. The majority of rodent studies have failed to demonstrate any effect of exogenous retinoids on IL-4 production but have observed a type 2-promoting effect of RA only when exogenous IL-4 was added to the cultures [12, 22, 27–29]. However, a recent study by Iwata et al.  demonstrated the direct effects of ATRA and 9-cis-RA on Th2 cytokine production by murine T cells derived from TCR transgenic mice. These authors also demonstrate the ability of RA to inhibit Th1 cytokine responses, while enhancing IL-4 production by Th2-polarized cells. In contrast, RA has also been shown to inhibit IL-4 production by a antigen-stimulated rat mast cell line  and inhibited IL-4-induced IgE synthesis from CD40-stimulated B cells [31, 32]. Moreover, additional studies have suggested that VA or retinoids possess limited direct type 2 differentiating effects on purified T cells but appear to act primarily at the level of the APC by reducing type 1 cytokine synthesis [28, 33]. Obviously, given all the variations in these findings, the selective differentiating effects of VA and retinoids on cytokine synthesis by T cells remains controversial. Despite all of this work, little to no detailed data exists utilizing purified human T cells and T cell subsets in such studies. In the current manuscript, we provide the first systematic analysis of the effects of the retinoids, ATRA and 9-cis-RA, on the development of a Th2 cytokine response as well as several cytokines and chemokines using an in vitro model of human T cell activation.
ATRA and 9-cis-RA inhibit Th1 and promote Th2 reactions by human T cells and peripheral blood mononuclear cells (PBMC)
Given the multiple reports describing the effects of retinoids on cytokine production by murine splenocytes and T cells, we initially examined the effects of various concentrations of ATRA and 9-cis-RA on the production of Th1- and Th2-associated cytokines by anti-CD3-stimulated human T cells and PBMC in vitro. Culture supernatants were examined 48 hrs after stimulation for cytokine levels. The results in Figure 1 demonstrate a representative dose response curve of ATRA and 9-cis-RA on the expression of IL-4, IL-5 and IFN-γ by human T cells and PBMC. These data reveal that the Th2 cytokines, IL-4 and IL-5, are induced in T cells and PBMC in a dose-dependent manner, while the production of the Th1 cytokine, IFN-γ, is inhibited in response to increasing concentrations of ATRA and 9-cis-RA. These findings were highly reproducible in greater than 95% of the PBMC and T cells donors examined (n > 20). Based on the above curves, ATRA and 9-cis-RA were utilized in subsequent experiments at the 10-7 M (100 nM) concentration, a dose range that we and others  have shown to be optimal for human T cell stimulation.
Besides these Th1 and Th2 cytokines, additional cytokines were also examined including IL-12p70, IL-13 and TNF-α. Protein levels of IL-12p70, TNF-α and IFN-γ in the culture supernatants were significantly decreased, while IL-4, IL-5 and IL-13 protein levels were significantly increased by ATRA treatment in all donors tested (Table 1). ATRA and 9-cis-RA were equipotent in their effect on the majority of these cytokines. However, 9-cis-RA was significantly more effective than ATRA in inhibiting TNF-α. ATRA and 9-cis-RA failed to significantly alter IL-10 and IL-15 cytokine production by stimulated human PBMCs. While not shown, IL-18 levels were not consistently affected by ATRA or 9-cis-RA.
As PBMCs are a heterogeneous population of cytokine producing cell populations, we also examined the influence of ATRA on Th1- and Th2-associated cytokine production from purified CD4+, CD8+ and non-fractionated T cells. Similar to the above results, our data revealed that IL-4 and IL-5 synthesis was increased and IFN-γ expression was inhibited in the supernatants of all stimulated T cell populations examined (data not shown). The ATRA-induced changes in the ratio of these two cytokines were greatest in PBMCs followed by CD4+ T cells, T cells and then by CD8+ T cells.
ATRA also modulated the expression of several other inflammatory cytokines and chemokines by human PBMCs (Table 2). Many of these factors have not been previously shown to be influenced by retinoids. Interestingly, the expression of IL-8 and MCP-1 were both augmented by ATRA treatment, while the expression of RANTES, MIP-1β, G-CSF, IL-1β and IL-6 were significantly inhibited by ATRA treatment of anti-CD3 mAb-stimulated human PBMCs. While MIP-1α was not significantly different between the control and ATRA-treated groups, there was a trend towards downregulation (p = 0.09). IL-17, GM-CSF and IFN-α failed to demonstrate any significant differences between control and experimental cultures. The relevance of exogenous or endogenous retinoids and their nuclear receptors in the expression and production of various cytokines and chemokines remains to be defined.
We next sought to determine whether the RA-induced decrease in IFN-γ and increase in IL-4 production may be due to a shift in the frequency of cytokine producing T cells and/or the quantity of cytokine being produced by individual cytokine-producing cell. Using intracellular flow cytometric analysis of several donors, we observed a decrease in the percentage of T cells staining for IFN-γ in cultures treated with either ATRA (5.2%) or 9-cis-RA (6.3%) when compared to control T cells (15.8%). Similar studies were performed for IL-4 and IL-5; however, consistently poor intracellular staining for these cytokines was observed using several human T cell donors in our hands. So to more accurately measure the effects of RA on the frequency of Th2 cytokine production, ELISPOT analysis was performed. The results in Table 3 demonstrate the representative results of anti-CD3 mAb-activated T cells derived from single donor of two examined where a range of an approximate 3-fold increase in the frequency of IL-4- and an approximate 2-fold increase in the frequency of IL-5-producing T cells in ATRA-treated T cell cultures compared to vehicle-treated cells. In addition, a 1.5-fold decrease in IFN-γ-producing T cells was also observed between cultures treated with ATRA compared to a vehicle control. These data suggest that treatment with RA results in an increase in the frequency of T cells producing Th2 cytokines, possibly through the direct induction of type 2 cytokine or transcription factor RNA.
ATRA inhibits type 1 and promotes type 2 reactions even under Th1- or Th2-polarizing culture conditions
We believe that inhibition of accessory cell cytokine production by ATRA or 9-cis-RA may account for the greater type 2 polarization observed in PBMCs versus non-fractionated T cells or the CD4+ and CD8+ T cell populations. We therefore examined whether ATRA-induced alterations in IL-4, IL-5 and IL-13 production persisted under strong Th1- or Th2-polarizing conditions. ATRA-induced changes in IL-5 and IL-13 were not further altered upon the addition of exogenous IL-12, IL-4, or neutralizing anti-IL-4 and anti-IL-12 antibody (Figure 2). The biological activity of such manipulation is evident from corresponding increase or decrease in IFN-γ production. Due to extreme variations in the degree of stimulation by IL-4 and IL-12 in the human donors examined, only a representative experiment with one donor is shown in Figure 2. Three individual donors were examined in this experimental series and each donor demonstrated similar effects. Moreover, we have found that the addition of other potential type 1-inducing cytokines including IFN-γ or IL-18 in the presence of neutralizing anti-IL-4 antibody also failed to alter the effect of ATRA on IL-5 or IL-13 production within the cultures (data not shown). Moreover, similar to primary human T cells and these polarization cultures, we have also found that ATRA increases the proliferation and IL-4 production by human and murine Th2 clones with little to no major effects or inhibition on Th1 clones (data not shown).
ATRA promotes Th2 responses in the presence or absence of CD28 co-stimulation
To assess whether this same requirement was necessary for RA using human cells, purified human T cells were stimulated with anti-CD3 mAb and ATRA in the presence or absence of CD28 costimulation. The results in Figure 4 demonstrate that even in the absence of CD28 costimulation, ATRA increases IL-5 production by primary human T cells. Upon stimulation with anti-CD28mAb, there is even a greater level of IL-5 production by T cells stimulated with ATRA. In addition, CD28-costimulation was previous found to be necessary to observe the IFN-γ-inhibitory effects of ATRA using a murine model . Similarly, we have found that ATRA inhibited IFN-γ production in the presence of anti-CD28 mAb (Figure 3). Thus, ATRA is capable of inducing Th2 cytokine expression in the absence of costimulatory signals such as CD28.
As type 2 differentiation is thought to involve two temporally separate signals, a differentiation and proliferation signal , we next examined the time course of ATRA-induced Th2 polarization of CD4+ T cells in response to anti-CD3 and -CD28 mAb. As shown in Figure 4, the effects of ATRA were evident as early as 12 hrs after the initiation of the cultures. However, these differences did not reach statistical significance for IL-5 levels until 24 and 48 hr of culture. Similar trends for IL-4 expression were observed as shown here for IL-5 (data not shown).
ATRA and 9-cis-RA induced Th2 cell polarization occurs at the mRNA level
We next examined the effects of ATRA and 9-cis-RA on the level of mRNA of each Th1- or Th2-associated cytokine. As shown in Figure 5, the relative copy number of IL-4 and IL-5 mRNA was significantly increased by ATRA and 9-cis-RA utilizing PBMC derived from 5 different donors. Although similar levels of IL-4 protein were induced by both retinoids, 9-cis-RA was found to be at least two-fold more effective at inducing IL-4 message compared to ATRA. In addition, the relative copy number of IFN-γ mRNA was modestly but significantly decreased by both 9-cis-RA and ATRA. The results in Figure 5 were performed in the presence of low dose IL-2 to assist in cell activation and the maintenance of the cells. Similar results were observed in the absence of IL-2 or in the presence of anti-CD28 mAb (data not shown). Moreover, ATRA treatment of human T cells over various time intervals enhanced the expression of the Th2 cytokine, IL-4 and the Th2 transcription factors, GATA-3, c-MAF and STAT6 at 6 and 24 hours post stimulation and decreased the expression of the Th1 transcription factor, T-bet, at these same time points (Figure 6). The specific effects on the expression of Th2 transcription factors and subsequently cytokine production strongly support the ability of RA to facilitate the polarization of human T cells to a Th2 phenotype.
In the current study, we have described induction of the expression of the type 2 cytokines, IL-4, IL-5, and IL-13, and the inhibition of IFN-γ production upon treatment of human T cells with either ATRA or 9-cis-RA. To our knowledge, this is the first report describing retinoid-induced stimulation of IL-4 and IL-13 synthesis in human T cells. Furthermore, our IL-5 production data supports other reports that describe a decrease in IL-5-secreting T cells in VA-deficient mice and an increase in murine and human IL-5 synthesis by ATRA treatment of activated T cells in vitro [13, 18]. This suggests a coordinated regulation of IL-4, IL-5, and IL-13 production from T cells ; however, there are important differences in the activation stimuli, kinetics, transcription factors, and cell types which govern their production. The production of IL-4, IL-5, and IL-13 is frequently, but not exclusively, co-expressed by individual CD4+ T cells [38–40]. In vivo murine models suggest that CD28 co-stimulation is required to induce IL-4-, but not IL-13-dependent responses . There are reported differences in the regulation of IL-4, IL-5, and IL-13 by transcription factors including c-MAF [42, 43]. Furthermore, human CD8+ cells reportedly produce low levels of IL-4 but substantial quantities of IL-5 and IL-13 . The potential independent regulation of the production of these cytokines was also reflected in our observation of a limited effect of IL-4 or IL-12 addition or neutralization on IL-5 and IL-13 production.
One question that may arise from these studies is the vitamin A status of the donors utilized in these experiments. Serum for tissue culture contains a variable amount of vitamin A and a low amount of retinoic acid  and the individuals that the PBMC and T cells were obtained from are most likely vitamin A sufficient. The use of charcoal-stripped media to reduce the vitamin A levels used in cell culture adds the potential for artifactual data generation because there is no selectivity in the removal process. Similarly, the use of serum free media adds to the potential for artifactual data generation because it frequently provides a minimal set of nutrients (HL-1) and/or artificial growth stimulators such as diacylglycerol (AIM-V). Human T cells , Epstein-Barr Virus (EBV)-transformed human B cell lines  and myelocytic leukemia cells (HL-60) cells are known to contain esterified vitamin A . This would allow the cells to survive for the 10–14 days in serum-free media it takes to deplete them of endogenous retinoids . However, the time spent ex vivo greatly adds to the potential for artifactual data generation. Perhaps for these reasons, most recent studies, including many human studies on the potential immunoregulatory mechanisms of retinoids in primary T cells or PBMCs generally use unadulterated FBS and cells from vitamin A sufficient animals or humans [13, 34, 45, 49, 50]. In addition, retinoic acid is present in human plasma at a concentration of around 10–20 nM mainly in two stereoisomeric forms, all-trans-RA (tRA, ~75%) and 13-cis-RA (~25%) . The concentration of RA in most rat and human tissues is higher than the plasma concentration [52, 53]. When rats, mice and humans are supplemented with pharmacological amounts of RA, plasma RA concentrations can approach 0.5–3.0 uM . A very large number of studies, including several studies similar to ours have used ATRA concentrations of 0.5 to 1.0 e-7M ATRA, doses that the authors had previously determined to be optimal in their systems [13, 34, 45, 50].
Our observation that ATRA and 9-cis-RA had no consistent effect on IL-10 production was unexpected. A previous report indicated that overexpression of IL-10 mRNA occurs during VA deficiency in rats . However, several studies have reported either a stimulatory or no effect of retinoids on IL-10 synthesis [12, 15, 18]. While our data strongly support a RA-induced type 2 response, the lack of a consistent effect of RA on IL-10 production provides compelling evidence that IL-10 may not be an ideal indicator of a type 2 phenotype . IL-10 has not only been shown to be expressed during anti-inflammatory and type 2 responses , but also has been reported to be expressed by CD4+ T cells and T cell clones producing both IFN-γ and IL-10 .
A role for retinoids in inhibiting IL-12 synthesis in humans is consistent with data from studies describing overexpression of IL-12p40 mRNA during VA deficiency in mice  and rats  as well as from several in vitro studies demonstrating diverse inhibitory effects of retinoids on IL-12 production by LPS- or KLH-stimulated mouse macrophages [33, 57]. However, our current studies suggest that ATRA-induced reduction in IL-12 expression is not a critical factor in RA-induced type 2 polarization of human T cells. Furthermore, in contrast to our current findings, the addition of exogenous IL-12 to cultures reduced ATRA and 9-cis-RA-induced murine T cell IL-4 synthesis to the level of control cultures  and the neutralization of IL-4 within the cultures decreased the type 2-promoting effect of 9-cis-RA . Our current data also contrast with the recent studies suggesting that the RA-induced type 2 polarization of T cells is exclusively regulated at the level of the APC [28, 33]. In these studies, RA-pretreated, LPS-stimulated macrophages induced antigen-specific T cells to polarize into Th2-like cells in the absence of exogenous RA, presumably through reduced IL-12 synthesis. However, our studies demonstrate an IL-12 independent role for ATRA in type 2 cytokine polarization in vitro.
Data presented herein showing the equipotency of ATRA and 9-cis-RA in promoting a type 2 response in human T cells contrasts with in vitro murine T cell development studies where 9-cis-RA, but not ATRA, stimulated Th2 development . Our data suggest the involvement of ligated nuclear retinoic acid receptors (RARs) but not retinoid X receptors (RXRs) in Th2 differentiation as ATRA binds to only to RARs and 9-cis-RA binds to both RARs and RXRs. We have found that RARα agonists recapitulate the effect of retinoic acid shown here and the use of a RARα antagonist inhibits the effect of retinoic acid on the Th2-related responses (data not shown). These data must be interpreted with caution because of the non-specific interconversion of ATRA and 9-cis-RA under normal cell culture conditions . In addition, we can not rule out the possibility that RXR receptors also play a role in Th2 development as have recently been shown in murine T cells . We are currently exploring which nuclear receptors (RAR and/or RXR) are involved in ATRA-induced Th2 differentiation by the use of stable receptor-selective retinoids.
Costimulation with CD28 reportedly favors development of human type 2 T cells in vitro . CD28-costimulation was also necessary to observe the IFN-γ-inhibitory effects of ATRA using a murine model . However, our observation that the preservation of the ATRA-induced type 2 responses by T cells in the absence of CD28-costimulation is unique. The differential CD28-dependency of these two responses is unknown but is supported by previous data which suggests that CD28 costimulation is required for inhibition of IFN-γ production but not induction of IL-5 production during Th2 polarization . Unlike murine T cells , we have also observed a relatively equal decrease (ranging from 10–30%) in the frequency (Table 3) and the percentage and intensity of T cells staining for IFN-γ (intracellular flow analysis, data not shown) in cultures treated with ATRA and 9-cis-RA in the presence or absence of CD28 mAb. These data are inconsistent with a murine study where ATRA failed to alter the frequency of the IFN-γ secreting T cells . Our preliminary observations demonstrating that this decrease appears to only occur within TNF-α/IFN-γ double producing T cells supports a general negative regulatory effect of retinoids on type 1 cytokine production. These cytokines have been reported to be frequently co-expressed by pathogen-generated human Th1 clones .
What are the potential mechanisms for direct induction of Th2 differentiation by ATRA or 9-cis-RA? It is possible that RA directly activates transcription through its nuclear receptors, RAR and or RXRs; however, our search of the 5' promoter region of the Th2 cytokine genes, IL-4, IL-5 and IL-13, did not reveal any RAR or RXR-response elements. The refractory nature of retinoid-induced Th2 differentiation to changes in IL-4 and IL-12 levels and CD28-mediated costimulation suggests that ATRA may act through a master Th2 differentiation factor such as Ets-1, cMAF, GATA-3 or STAT-6. This is consistent with recent data obtained from tumor cell lines where RA induced the synthesis of Ets-1  and STAT-6 , transcription factors that are involved in Th2 differentiation . Ectopic expression of GATA-3 in Th1 cells induces IL-4, IL-5, and IL-13 production and ectopic expression of Stat6 in Th1 cells induces the production of Th2-cytokine such as IL-4 and IL-5 . STAT-6 also induces the expression of Ets-1, MAF and GATA-3 and reduces the expression of IL-12R∃2 message independently of IL-4 production . Here, through the use of real time RT-PCR using several of the retinoid-treated T cells and PBMCs, we also observed increases in the gene expression of the Th2 factors, cMAF, GATA-3, and STAT-6, using ATRA and a concomitant decrease in the expression of the Th1 factor, T-bet, 4–12 hours post stimulation (Figure 6). These data strongly support a specific role for retinoids in the development of Th2 cells.
In conclusion, we have demonstrated that ATRA and 9-cis-RA increase the expression of IL-4, IL-5 and IL-13 but not IL-10 mRNA and protein from activated human T cells. ATRA acts early and directly polarizes T cells towards type 2 responses even in the presence of type 1-inducing signals or in the absence of CD28-costimulation. Although ATRA decreased IL-12 synthesis within PBMC cultures, this was not obligatory as RA directly induced type 2 cytokine production by highly purified human T cells in the absence of APCs. A better understanding of the type 2 cytokine promoting activity of ATRA and 9-cis-RA in human T cells would provide better clinical interventions to boost vaccine efficacy to certain antigens or to reduce various types of pro-inflammatory and autoimmune pathologies .
ATRA, 9-cis-RA were purchased from Sigma, St. Louis, MO. Retinoids were dissolved at various concentrations in 100% ETOH, overlayered with argon gas and stored at -80°C in the dark until used. Recombinant human IFN-γ, IL-4, IL-12 and IL-18 were obtained from R & D Systems (Minneapolis, MN). Recombinant IFN-γ was obtained from Biosource Int. (Camarillo, CA). Neutralizing monoclonal antibodies (mAbs) to human IFN-γ (clone 25718.111) IL-4 (clone 34019.111), and IL-12 (clone 24910.1) were also obtained from R & D Systems. Based upon manufacturer's testing lot-specific testing, 1 :g of anti-IFN-γ, anti-IL-4, and anti-IL-12 will neutralize 5 ng/ml, 300 pg/ml and 700 pg/ml of rhIFN-γ, rhIL-4, and rhIL-12, respectively.
Whole blood was acquired from healthy human volunteers between the ages of 21–55 years who provided informed consent. PBMC were isolated by Ficoll Paque (Amersham Pharmacia Biotech, Piscataway, NJ) density gradient centrifugation followed by treatment with ammonium chloride (ACK) lysis solution (Biofluids, Gaithersburg, MD) to eliminate the remaining erythrocytes. The isolated cells were subsequently washed 2 times in PBS and resuspended in RPMI 1640 (Biofluids) supplemented with 10% heat-inactivated FBS (Sigma), 2% heat-inactivated pooled human AB serum (Sigma), 50 μM mercaptoethanol (Gibco BRL Gaithersburg, MD), 1 mM sodium pyruvate (Biofluids), 2 mM glutamine, 1 × non-essential amino acid solution (Biofluids), 1 mg/ml gentamicin (Biowhittaker, Walkersville, MD), 100 U/ml penicillin (Biofluids), 100 :g/ml streptomycin (Biofluids), and 20 mM HEPES buffer (Biofluids). T cells, CD4+ T cells and CD8+ T cells were isolated by negative selection using enrichment columns according to manufacturer's instructions (R & D Systems). All of these cells were typically > 93% pure as assessed by flow cytometric analysis. The contaminating cell population was largely CD8+ cells. Most likely, these cells were NK cells based on their size and granularity.
Cell culture and harvest
PBMC (2.5 × 10 6 cells/ml) were activated with 200 ng/ml of immobilized anti-CD3ε OKT-3, Ortho, Raritan, NJ) ± 0.001 to 1 μM of various retinoids or ETOH vehicle control for 48 h. IL-2 (Teceleukin, Hoffman LaRoche, Nutley, NJ) at 10 U/ml was added where indicated. Where indicated, 1 μg/ml of neutralizing anti-cytokine mAb was added to the cultures. Alternatively, T cells (1.0 × 10 6 cells/ml) were activated with 200 ng/ml of immobilized anti-CD3 and 0.1 to 1 μg of soluble anti-CD28 (clone 28.2, Pharmingen) or IL-2 at 10 U/ml was added where indicated to provide co-activation or costimulatory signals. PBMCs or T cells were harvested at various times after incubation at 37° and 5% CO2. The 48 hr time interval was selected for many of the studies shown based on the optimal and reproducible cytokine expression in response to anti-CD3 mAb. Non-adherent cells were decanted from the flasks and centrifuged to obtain supernatants. The flasks were then treated with Enzyme-Free cell disassociation solution (Specialty Media, Phillipsburg, NJ) to remove the adherent cells (a typical result of cell activation and the anti-CD3 coated flasks) and were gently scraped to remove and harvest the cells. Viable cells from the decanted cells and cell removal mixture were isolated by Ficoll Paque density gradient centrifugation (as described above). Cell viability was not significantly affected by this enzyme treatment process (viability >95%).
It should be noted that we have also utilized the serum free medium AIMV in these various cultures and observed similar effects to serum containing medium (data not shown).
ELISA (Biosource) and Bio-Plex Human Cytokine 17-Plex (Biorad, Hercules, CA) were utilized to examine the following human-specific cytokines: IFN-α, IFN-γ, IL-1α, IL-1β, IL-4, IL-5, IL-6, IL-7, IL-8, IL-10, IL-12 p70, IL-13, IL-15, IL-17, G-CSF, GM-CSF, MIP-1∀, MIP-1∃, RANTES, MCP-1 and TNF-α. The IL-18 ELISA was obtained from R & D Systems (Minneapolis, MN). All of the ELISAs and multiplex assays were performed according to the manufacturer's instructions. The results are expressed as pg/ml or ng/ml and all assays were run in duplicate with at least three separate experiments being examined.
Real Time PCR
Cytoplasmic RNA was extracted and purified using a commercially available kit (RNAeasy, Qiagen, Valencia, CA). Purified RNA was electrophoresed on a 1% agarose gel to assess the integrity of the purified RNA. One :g of RNA was reverse transcribed into cDNA using a commercial available kit (Applied Biosystems, Foster City, CA). One hundred pg RNA equivalent of this cDNA was used for PCR amplification. PCR reactions were performed in special optical tubes in a 96 well microtiter plate format on an ABI PRISM 7700 Sequence Detector System (PE Applied Biosystems) using pre-developed FAM- and TAMRA-labeled internal oligonucleotide probes and primers for IFN-γ, IL-4, IL-5, IL-10, IL-12p30, IL-12p40, IL-15, and TNF-α (PE Applied Biosystems). Each reagent also contains VIC- and TAMRA-labeled internal oligonucleotide probes and primers specific for the 18S RNA ribosomal subunit. Amplification conditions were as follows 25°C for two min; 95°C for 10 min; 40 cycles of 95°C 15 s and 60°C for 1 min. Fluorescence signals measured during amplification were processed post-amplification and were regarded as positive if the fluorescence intensity was ten fold greater than the standard deviation of the baseline fluorescence. This level is defined as the threshold cycle (Ct). The Ct value for 18S ribosomal subunit was subtracted from the Ct value for each cytokine message to normalize for RNA content. This value is defined as ΔCT. To evaluate the effects of retinoids, ΔCTtreatment was subtracted from ΔCtcontrol. This value is defined as ΔΔCT. The relative folds increase or decrease was then calculated as 2 -ΔΔCT.
The PCR was also set up using SYBR green Master Mix (Applied Biosystems), 1 μl cDNA and gene-specific primers at a final concentration of 0.3 μM. Thermal cycling was carried out on the Applied Biosystems GeneAmp 7700 Sequence Detector and SYBR green dye intensity was analyzed using GeneAmp 7700 SDS software. Primers for human GATA3, STAT6, C-MAF, and T-bet genes and glyceraldehyde-3-phosphate dehydrogenase (GAPDH) as control were designed using ABI prism software (PE Applied Biosystems). Primers are available upon request. Similar amplification procedures and data computation were followed as described above. No PCR products were generated from genomic versus cDNA template.
Intracellular Flow Cytometry and ELISPOT analysis
Mouse anti-human CD3-Cy-Chrome®, anti-human IL-4-phycoerytrin (PE), anti-human IFN-(-fluorescein isothiocyanate (FITC) anti-human TNF-∀-FITC, and the appropriately labeled isotype control mAbs were obtained from Pharmingen. PBMCs were cultured for 36 hrs as described above after which the cells were treated with 2 :M monensin (Sigma) and subsequently harvested as described above. Cells (0.25 × 106) were suspended in 50 :L of staining buffer (1% FCS, 1% goat serum, 2.5 :g of mouse IgG/50 μL) in round-bottom 96-well plates at 4°C for 15 min. 5 :L of the appropriate dilution of each antibody was then added. Cells were then incubated for 30–40 min at 4°C. Cells were pelleted and medium was aspirated carefully. Cells were then washed with 100 :L of PBS/FBS buffer twice. Cells were fixed and permeabilized with Cytofix/Cytoperm® solution (Pharmingen). Various combinations of labeled anti-human cytokines were used to stain cells. Cytochrome-conjugated mouse IgG1 mAb and PE mouse-IgG were used as isotype controls at the same concentrations as the anti-cytokine antibody. Additional controls in which the labeled mAbs and 10 fold saturating recombinant cytokine proteins were pre-incubated for 30 min at room temperature before staining (IL-4). Alternatively, cells were pretreated with unlabeled mAb (IFN-γ). Three-color cytofluorometry was performed using a FacScan (Becton Dickinson, San Diego, CA). A minimum of 10,000 CD3+ cells were analyzed in these experiments. Data are expressed as the % of CD3+ cells expressing the marker of interest or the mean channel number (MCN) of the marker's fluorescent intensity.
The ELISPOT assays (BD Biosciences) used to quantify IFN-γ-, IL-4, and IL-5-producing T cells were performed according to the manufacturer's instructions. Briefly, T cells were prepared at different cell densities ranging from 1 × 105, 1 × 106, and 2.5 × 106 cells per ml and 100 :l of the suspensions were added to each well of mouse anti-human cytokine antibody-coated BD ELISPOT plates. The cells were stimulated using ATRA or 9-cis-RA and/or soluble anti-CD3 and CD28 antibodies described above under cell culture. The plates were then incubated at 37°C in a 5% CO2 humidified incubator for 24 hr after which the cell suspension were aspirated, the wells were washed with various combinations of deionized water and wash buffer, and subsequently developed using the proper antibody, conjugate and substrate pairs defined by the manufacturer. The plates were air-dried overnight at room temperature and the plates were stored in a sealed bag in the dark until analyzed. Spots were then enumerated using an ImmunoSpot® Series 2 Analyzer (Cellular Technology Limited, Cleveland, Ohio) and the supporting ImmunoSpot® Software. Spots were counted by an automated system using a defined set of parameters for size, intensity, and gradient. The background (the mean numbers of spots in wells without stimulation) was subtracted from each well on each cytokine plate. A response was considered positive if the average number of cytokine-producing cells (CPC) per triplicate wells exceeded background +/- 2SD. The data are shown as the average number of CPC per 106 cells.
Data were analyzed for equality of variance using Fischer's F test (Statview 5.0 for Macintosh, Abacus Concepts, Berkeley, CA). If the variance was heterogeneous, the appropriate transformation of the data was performed. A two-tailed paired T test was then used to determine statistical significance. A P < 0.05 was considered statistically significant for all analysis.
all-trans retinoic acid
9-cis- retinoic acid
delayed type hypersensitivity
precursor T helper
retinoic acid receptors
retinoid X receptors
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The content of this publication does not reflect the views or policies of the Department of Health and Human Services, nor does mention of trade names, commercial products or organizations imply endorsement by the U.S. Government. This research was supported in part by the Intramural Research Program of the National Institute on Aging, National Institutes of Health. We would like to thank the members of the GRC Flow Cytometry Laboratory and the Pheresis Unit for assistance with the flow cytometric analysis presented herein. We would like to thank Drs. Eric Schaffer, Paritosh Ghosh, and Dan L. Longo for their thoughtful review and comments on this manuscript. In addition, we would also like to thank Ms. Angie Feehley for her assistance in the preparation of this manuscript and Mr. Gregory Maher for his excellent technical assistance.
HD, GC, RP, MLK, AW, VDD, CN and DDT did the experiments. HD and DDT prepared the figures and co-wrote the paper. DDT supervised the work and edited the manuscript. All authors have read and approved the final version of the manuscript.
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