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Clinical and Developmental Immunology
Volume 2013 (2013), Article ID 506807, 9 pages
O-Glycosylation of NnTreg Lymphocytes Recognized by the Amaranthus leucocarpus Lectin
1Unidad de Investigación, Instituto de Oftalmología Fundación Conde de Valenciana, 06800 México, DF, Mexico
2Laboratorio de Inmunología, Departamento de Bioquímica, Facultad de Medicina, (UNAM), P.O. Box 70159, 04510 México, DF, Mexico
3Departamento de Inmunología, Escuela Nacional de Ciencias Biológicas, IPN, 11340 México, DF, Mexico
4Departamento de Bioquímica, Instituto Nacional de Enfermedades Respiratorias, 4502 México, DF, Mexico
Received 18 June 2013; Accepted 4 August 2013
Academic Editor: Lenin Pavon
Copyright © 2013 María C. Jiménez-Martínez et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
O-glycosidically-linked glycans have been involved in development, maturation, homing, and immune regulation in T cells. Previous reports indicate that Amaranthus leucocarpus lectin (ALL), specific for glycans containing galactose-N-acetylgalactosamine and N-acetylgalactosamine, recognizes human naïve CD27+CD25+CD4+ T cells. Our aim was to evaluate the phenotype of CD4+ T cells recognized by ALL in peripheral blood mononuclear cells obtained from healthy volunteers. CD4+ T cells were isolated by negative selection using magnetic beads-labeled monoclonal antibodies; the expression of T regulatory cell phenotypic markers was assessed on ALL-recognized cells. In addition, IL-4, IL-10, IFN-, and TGF- intracellular production in cells was also evaluated. The analyses of phenotypic markers and intracellular cytokines were performed through flow cytometry. ALL-recognized CD4+ T cells were mainly CD45RA+, CCR7+ cells. Although % CD25+Foxp3+ cells were positive to ALL, only % of cells corresponded to CD25+Foxp3− cells. Intracellular cytokines in freshly obtained CD4+ T cells exhibited 8% of IL-4, 15% of IL-10, 2% of IFN-, and 15% of TGF-, whereas CD4+ T cells depicted 1% of IL-4, 2% of IL-10, 1% of IFN-, and 6% of TGF-. Our results show that galactose-N-acetylgalactosamine and N-galactosamine-bearing CD4+ T cells expressed phenotypic markers of NnTreg cells.
Lectins specific for O-glycosidically-linked glycans, containing galactose-N-acetylgalactosamine or N-acetylgalactosamine, have been used to study T-cell activity, as reviewed by [1, 2]. In these studies, the lectin from Artocarpus heterophyllus is considered to be mitogenic for human CD4+ T cells , whereas Artocarpus lakoocha has antiproliferative effect on human leukemic cells , and Dolichos biflorus agglutinin is used to isolate leukemic T cells .
Amaranthus leucocarpus lectin (ALL) is a nonmitogenic lectin with specificity for galactose-N-acetylgalactosamine (Galβ1,3 GalNAcα1,O-Ser/Thr) or N-acetylgalactosamine (GalNAcα1,O-Ser/Thr) . In contrast to other GalNAc-specific lectins such as S. sclarea  or PNA , the recognition of ALL is limited when GalNAc residues are arranged in clusters, as demonstrated by using glycopeptides with different GalNAc distribution [9, 10]. This lectin binds murine medullary thymocytes  and a human peripheral blood CD4+ T cell subset with phenotypic markers CD25, CD27, and CD45RA . Interestingly, ALL is capable of inducing suppression of the immune response in mice , and it recognizes dexamethasone-resistant thymocytes with increased GalNAc transferase-activity . It has been shown that dexamethasone administration to mice allows the survival of functional CD4+CD25+ T regulatory cells in the thymus . Likewise, the dexamethasone treatment in asthma patients promotes differentiation toward T regulatory cells by a Foxp3-dependent mechanism , and when patients, receiving allogeneic lymphocyte transplantation, are treated with glucocorticoid, graft versus host disease is suppressed by expansion of CD4+CD25+Foxp3+ T cells .
The existence of T-cell subsets with regulatory capacity of the immune response, expressing CD4, CD25, and Foxp3 has been evidenced . Naturally occurring CD4+CD25+ regulatory T cells (nTregs) represent a major lymphocyte population engaged in the maintenance of immune tolerance as reviewed in . CD4+CD25+ nTregs are differentiated in the normal thymus as a functionally distinct subpopulation of T cells [19, 20]. In humans, the CD4+CD25+ nTregs are CD27+CCR7+Foxp3+, and most of these cells express CD45RO . On the other hand, the existence of CD45RA+ Tregs that resemble a naïve cell subset (NnTreg) have been described [22, 23]. Glycosylation changes have also been reported in nTregs, suggesting that sialylation could be a regulatory ligand in CD4+CD25+ Foxp3+ cells . In this context, O-glycosylation has been proposed to play a direct and powerful role in regulating T-cell function [14, 25, 26]. Recently, ALL has also shown a costimulatory effect on human CD4+ T cell activated via CD3  turning ALL into a new tool to study O-glycans-bearing glycoproteins in T-cell populations. Thus, the aim of this work was to know whether the O-glycosidically linked structures recognized by ALL are expressed by a Treg subset.
2. Material and Methods
2.1. Antibodies and Reagents
Phycoerythrin (PE)-labeled mouse IgG monoclonal antibodies (mAbs) against human IL-4, IL-10, and CTLA-4 and fluorescein isothiocyanate (FITC)-labeled antibodies against human IFN-γ, CD62L, Foxp3, and CyChrome-streptavidin were purchased from BD PharMingen (San Jose, CA, USA). FITC- and PE-labeled mouse anti-human CD45RA and CD45RO mAbs and anti-IgG-FITC were obtained from Southern Biotech, Inc. (Birmingham, AL, USA). FITC- and PE-labeled mAbs antihuman CCR7 and anti-hLAP (TGF-β1) were from RD Systems (Minneapolis, MN, USA). CD4 T-cell isolation Kit II (MiniMACS system) was obtained from Miltenyi Biotec (Auburn, CA, USA). Lymphoprep (Ficoll 1.077 density) was from Nycomed Pharma (Nyegaard, Oslo, Norway). RPMI-1640 culture medium, concanavalin A, FITC- and PE-labeled streptavidin, N-Acetyl-D-galactosamine (GalNAc), and salts were from Sigma Chemical Co. (St. Louis, MO, USA). Biotin was obtained from Pierce Chem, Co (Rockford, IL, USA). Sodium pyruvate, L-glutamine, and 2-mercaptoethanol were purchased from Gibco BRL. (Rockville, MD, USA). Fetal calf serum was from HyClone Labs. (Logan, UT, USA), and BD Cytofix/Cytoperm Kit and FASTImmune Kit (IFN-γ/IL-4) were from e-Biosciences (San Diego, CA, USA).
Amaranthus leucocarpus seeds were obtained from Tulyehualco, Mexico, and the lectin (ALL) was purified by affinity chromatography  and subsequently labeled with biotin at a biotin/protein ratio of 2 : 1 .
2.3. Isolation of Peripheral Blood Mononuclear Cells (PBMC)
Heparinized peripheral blood was diluted 1 : 2 (vol/vol) in phosphate buffered saline (PBS), pH 7.2. PBMC were separated on a Ficoll density gradient by centrifugation at 1700 rpm for 30 min at room temperature (°C). After centrifugation, the interface cells were collected, washed twice, and counted using a hemocytometer to assess viability by trypan blue dye exclusion.
2.4. Isolation of CD4+ T Cells
CD4+ T cells were purified from PBMC by negative magnetic separation in a MiniMACS system. For all cell isolations, the manufacturer’s instructions were followed. The purity of the separated CD4+ T cells was determined to be >95% in analyses through a flow cytometry (Becton & Dickinson FACScan; Mountain View, CA, USA), using an antihuman CD4 mAb coupled to FITC. Cell viability (>90%) of the purified cell subset was determined by the trypan blue dye exclusion method.
2.5. Inhibition Assays
Purified CD4+ cells were incubated with optimal concentration of biotin-labeled ALL in PBS supplemented with 0.2% bovine serum albumin and 0.2% sodium azide (PBA). After incubation, the cells were washed in PBA and incubated for a second step with PE-labeled streptavidin in PBA. To evaluate specificity of ALL, cells were again washed and incubated for the third time with 200 mM GalNAc in PBA. All incubations were carried out during 30 min at 4°C. Cells incubated only with PE-streptavidin were used as staining control.
2.6. Cell Cultures
CD4+ T cells were cultured in 24-well flat bottomed cell culture plates (Costar, Cambridge, MA, USA) at 1 × 106 cells/well in RPMI-1640 medium supplemented with 1 mM sodium pyruvate, 2 mM L-glutamine, 50 μg/mL gentamicin, and 10% heat-inactivated fetal calf serum and incubated at 37°C in a 5% CO2 humidified chamber. Concanavalin A (2 μg/mL) was added and, after 48 h, the cells were harvested and processed to measure Foxp3, TGF-β, and CTLA-4 expression through flow cytometry.
2.7. Immunofluorescence Staining of Cell Surface Markers
Triple-color staining was performed on purified CD4+ T cells by direct immunofluorescence, using FITC- or PE-labeled mAbs against CD45RA, CD45RO, CCR7, or CD25, and indirect fluorescence, using an optimal concentration of biotin-ALL plus CyChrome-labeled streptavidin. Briefly, 2 × 105 cells were suspended in 20 μL PBA and incubated with the fluorochrome-labeled mAb and biotin-ALL for 30 min at 4°C. After incubation, the cells were washed twice with PBA and incubated with CyChrome-streptavidin for 30 min. Then, cells were washed twice with PBA, fixed with 1% p-formaldehyde, and analyzed by flow cytometry.
2.8. Flow Cytometric Analysis of Intracellular Proteins
Purified CD4+ cells were incubated with biotin-ALL and CyChrome-streptavidin, as described above. Then, cells were fixed and permeabilized with the BD Cytofix/Cytoperm kit. Individually, cells were incubated with mAbs anti-IFN-γ FITC/IL-4 PE, anti-IL-10 PE, anti-Foxp3-FITC, or anti-CTLA-4-PE or anti-hLAP (TGF-β). After 30 min, cells were washed with PBS, incubated with anti-IgG-FITC for 30 min, and finally analyzed by flow cytometry.
2.9. Flow Cytometric Analysis
All cells were analyzed for marker’s expression by collecting 5000 events using a FACScan flow cytometer (Becton Dickinson, Mountain, View, CA, USA) and Cell Quest Pro software. To evaluate cell surface marker staining, a gate was drawn around the lymphocyte populations based on their physical properties (forward and side scatter), and a second gate was drawn based on positive or negative fluorescent ALL-binding to CD4+ T cells. To analyze intracellular protein staining, positive fluorescence staining of IFN-γ, IL-4, IL-10, TGF-β, Foxp3, and CTLA-4 (forward scatter and fluorescence) was set manually based on the distribution of cells stained with the isotype controls. Data are presented as two-dimensional dot plots or histograms. Control stains were performed using isotype-matched mAbs of unrelated specificity that were labeled with FITC or PE. Background staining was <1% and was subtracted from experimental values.
2.10. Statistical Analysis
Experiments were done independently and repeated at least three times. Data were analyzed by Mann-Whitney test to detect significant differences. Analyses were performed with Sigma-Stat 3.1 software. Differences were considered statistically significant when .
3.1. Flow Cytometric Phenotypic Analysis
The ALL+ T cell subset corresponded to 29% of the purified CD4+ T cell population (Figure 1(a)). The specific interaction of ALL with a subset of CD4+ T cells was confirmed by inhibition assays with their characteristic ligand, as expected GalNAc inhibited most of ALL-binding sites for CD4+ cells (Figure 1(b)). Phenotypic characterization of both ALL+ and ALL−CD4+ T cells showed that the frequency of CD62L+ cells was 1.1 times higher in ALL+CD4+ T cells (78% ± 1.4) than in ALL−CD4+ T cells (69.2% ± 2.4) (). In ALL+CD4+ T cells, the percentage of CD45RA+ cells was higher (71%) than the percentage of CD45RO+ cells (9%) () (Figure 2(a)). We observed also that the frequency of CCR7+ cells was increased 1.5 times more in ALL+CD4+ T cells (72%) than in ALL−CD4+ T cells (41%) (Figure 2(b)).
3.2. Frequency of CD25 and Foxp3 on CD4+ T Cells
Despite that the frequency of CD25+Foxp3+ cells was similar in both ALL+ and ALL− T cells (Table 1), we observed that CD25+Foxp3− cells were 1.9 times more frequent in ALL− T helper populations (62%) than in ALL+ T helper cells (38%) (). Similarly, CD25+Foxp3+ cells were 1.3 times less frequent in ALL−CD4+ T cells (47%) () than in ALL+CD4+ T cells (53%) (Figure 3).
3.3. Intracellular Cytokines in ALL+CD4+ T Cells
To know the cytokine profile of ALL+ and ALL− T helper cells at basal conditions, we performed intracellular staining to the cytokines IL-4, IL-10, IFN-γ, and TGF-β in nonstimulated CD4+ cells. Our results showed that ALL+CD4+ cells were IL-10+ (15%), IL-4+ (8%), IFN-γ+ (2%), and TGF-β+ (15%); in contrast, the percentages of cells positive to intracellular cytokines in the ALL−CD4+ T cells subset were as follows: IL-10+ cells (2%), IL-4+ cells (1%), IFN-γ+ cells (<1%), and TGF-β+ cells (6%) (Figure 4).
3.4. Frequency of CD25, Foxp3, CTLA-4, and TGF-β Cells after Polyclonal Stimulation
To determine whether the polyclonal stimulation influenced the frequency of CD25, Foxp3, and TGF-β in ALL+ and ALL− cells, we performed an in vitro Con A stimulation assay during 48 hours. We observed that the frequency of ALL−CD25+Foxp3+CD4+ T cells was increased 66.7 times in Con A-stimulated cells when they were compared to nonstimulated cells (), whereas the frequency of ALL+CD25+Foxp3+CD4+ T cells was increased 2-times in ConA-stimulated cells as compared to nonstimulated cells () (Figure 5(a)). Despite the increment in the number of CD25+Foxp3+CD4+ T cells in the ALL− cell subset, the percentage of CD25+Foxp3+CD4+ predominated in the ALL+ cell subset () at the end of the culture (Figure 5(b)). Although, we did not find statistical differences in intracellular/surface frequency of CTLA-4+ cells among ALL+ () and ALL− () T helper cells () (data not shown); the percentage of TGF-β+ cells was statistically higher in ALL+CD4+ T cells (98%) than in ALL−CD4+ T cells (51%) () (Figure 5(c)). After polyclonal stimulation, the percentage of TGF-β+ T cells increased 2.6 times in the ALL+CD4+ T cell subset as compared to ALL−CD4+ T cells; no significant differences were observed when we compared Con A-stimulated ALL−CD4+ T cells with nonstimulated cells (Table 2).
Surface O-glycosylation pattern of lymphocytes has been involved in development, maturation, homing, and immune regulation [24, 25, 29]. It has been shown that glycosylation changes occur in activated lymphocytes , and differences in sialylation as well as in expression of O-glycans are related to control of T-cell activation . In this study, we found that a subpopulation of CD25+Foxp3+CD4+ T cells expressing galactose-N-acetylgalactosamine or N-acetylgalactosamine is recognized by the Amaranthus leucocarpus lectin. A significant percentage of freshly obtained ALL-recognized T cells exhibited intracellular cytokines with regulatory activity such as IL-10 and TGF-β. It has been shown that CD25+CD4+ Treg cells are able to produce IL-4 and IL-10, without production of IFN-γ . Likewise, other authors have shown that sorted CD25+CD4+ Treg cells produce high concentrations of IL-10 and low IFN-γ . In agreement with these data, our results suggest that ALL+ T cells correspond to a Treg cell subset.
Previous reports concerning ALL binding to T cells suggest that this lectin recognizes specific O-glycans on recently activated naïve T cells . Our results showed that ~29% of the purified CD4+ T cells were positive to ALL. Phenotypic characterization of ALL+CD4+ T cells included a subset of CD45RA+, CCR7+, CD25+, and Foxp3+ cells, which resemble natural naïve NnTregs . The NnTregs represent a major lymphocyte population engaged in the control of self-reactive T responses and in maintenance of immune tolerance [18, 20]. Along with our findings, CD4+ T cells recognized by ALL were reported CD45RA+CD27+ cells . The CD27 molecule is a member of the TNF receptors that have been involved in early activation of naïve cells . It is interesting to note that CD27 expression on CD4+ T cell lines discriminates between regulatory and nonregulatory cells [33, 34]. Different authors have reported a distinct subset of CD25+Foxp3+CD4+ T cells characterized by CCR7, CD62L, and CTLA-4 expression contained in the CD45RA+/RO− naïve compartment [22, 23, 35]. CCR7 is a chemokine receptor that controls homing of lymphocytes to secondary lymphoid organs, and its expression in Tregs has been associated with maintenance of these cells for prolonged periods of time at those sites, inhibiting effector T-cell expansion . CD62L and CCR7 expression in T cells mediates lymphocyte homing to secondary lymphoid organs . CTLA-4 is a cell surface molecule that is expressed rapidly before cell activation, surface CTLA-4 is immediately internalized, which could explain the low levels of expression generally detected on the cell surface . Diverse authors have related CTLA-4 expression with nTreg cells [22, 23], and CTLA-4 expression is increased in Treg > NnTreg. Consistent with these data, we observed that the percentage of CTLA-4+ cells was increased in ALL+ than in ALL−CD4+ T cells, suggesting that CD4+ cells recognized by ALL could be either a subpopulation enriched in NnTreg cells or recently activated Treg cells . A proposal could be explained based on results obtained with in vivo antigenic-experienced circulating cells, as has been reported for other proteins related to Treg cells, such as Foxp3 , or for the intracellular CTLA-4 [22, 23].
Regulatory T cells are resistant to apoptosis ; similarly, ALL+ thymocytes are resistant to apoptosis after treatment with dexamethasone ; for this reason it would be interesting to examine apoptosis resistance in the ALL+CD4+ T cells from human peripheral blood to understand better the potential regulatory characteristics of this ALL+ NnTreg cell subset. Golks et al.  showed that an N-acetylglucosaminyltransferase is required for T cell activation, suggesting that modifications in glycosylation accompany T cell activation as reviewed . In this regard, the glycosylation status could generate differences among subsets of T cells, and possibly Tregs, as we observed in this study.
Taken together, our results suggest that ALL constitutes an important tool to study differences in O-glycans on CD4+ T cells with a regulatory-like phenotype, these CD4+ T cells are enriched NnTregs or recently activated Tregs expressing galactose-N-acetylgalactosamine and N-acetylgalactosamine.
The authors are grateful to Marisela Linares for her technical assistance. This work was supported by DGAPA (PAPIIT-IN2230105-3) UNAM CONACyT CB-1 0129932 and Fundación Conde de Valenciana.
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