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Journal of Immunology Research logoLink to Journal of Immunology Research
. 2016 Feb 16;2016:5290604. doi: 10.1155/2016/5290604

Group B Streptococcus Induces a Robust IFN-γ Response by CD4+ T Cells in an In Vitro and In Vivo Model

Damian Clarke 1, Corinne Letendre 1, Marie-Pier Lecours 1, Paul Lemire 1, Tristan Galbas 2, Jacques Thibodeau 2, Mariela Segura 1,*
PMCID: PMC4771917  PMID: 26989699

Abstract

Group B Streptococcus (GBS) serotype III causes life-threatening infections. Cytokines have emerged as important players for the control of disease, particularly IFN-γ. Although potential sources of this cytokine have been proposed, no specific cell line has ever been described as a leading contributor. In this study, CD4+ T cell activation profiles in response to GBS were evaluated through in vivo, ex vivo, and in vitro approaches. Total splenocytes readily produce a type 1 proinflammatory response by releasing IFN-γ, TNF-α, and IL-6 and actively recruit T cells via chemokines like CXCL9, CXCL10, and CCL3. Responding CD4+ T cells differentiate into Th1 cells producing large amounts of IFN-γ, TNF-α, and IL-2. In vitro studies using dendritic cell and CD4+ T cell cocultures infected with wild-type GBS or a nonencapsulated mutant suggested that GBS capsular polysaccharide, one of the major bacterial virulence factors, differentially modulates surface expression of CD69 and IFN-γ production. Overall, CD4+ T cells are important producers of IFN-γ and might thus influence the course of GBS infection through the expression balance of this cytokine.

1. Introduction

Group B Streptococcus (GBS) or Streptococcus agalactiae is the main cause of life-threatening infections in newborns worldwide [1, 2]. GBS also affects pregnant women, elders, and immunocompromised patients [3]. Type III GBS is frequently involved in neonatal infections and is the most common type in GBS meningitis [1, 2].

Cytokines are important for controlling GBS disease, although exaggerated responses might be dangerous [4, 5]. While IL-10, IL-12, and IL-18 are beneficial [6–9], TNF-α contributes to GBS-induced sepsis [7, 10]. IFN-γ appears promising for control of GBS disease; IL-12 and IL-18 exert therapeutic effects by stimulating immune cells to produce IFN-γ [6, 8, 9], IFN-γ production is impaired in neonates and this might partly explain their susceptibility to GBS infection [8, 11, 12], and IFN-γ inhibits GBS survival in human endothelial cells [13]. Although NK and NKT cells have been proposed to secrete IFN-γ in response to GBS [14, 15], no specific cell line has been clearly identified yet as a major source.

Activated CD4+ T cells can differentiate into T helper (Th) cell types depending on the signals they receive. Th1 cells readily produce IFN-γ upon activation. GBS-infected dendritic cells (DCs) produce large amounts of proinflammatory cytokines like TNF-α, IL-6, and IL-12 [16] that could activate T cells. Furthermore, GBS-activated DCs release chemokines recruiting T cells, like CXCL9 and CXCL10 [16]. Although these evidences support IFN-γ production by T cells [17, 18], the participation of CD4+ T cells during GBS-induced disease is unknown.

GBS possesses a thick sialylated polysaccharide capsule (CPS) [19]. It is known as the most important factor for GBS survival within the host and interferes with innate defense mechanisms [4, 20, 21]. Encapsulated GBS is highly internalized by DCs but survives better intracellularly than its nonencapsulated counterpart. Bacterial internalization and the presence of CPS are also related to modulation of several cytokines and chemokines released by GBS-infected DCs [16, 22, 23].

It is hypothesized here that GBS drives CD4+ T cells differentiation into IFN-γ-producing Th1 cells and that the CPS can modify this response. The role of CD4+ T cells in the immune response against GBS type III was investigated using in vivo, ex vivo, and in vitro approaches in a mouse model. A nonencapsulated GBS mutant was included to dissect the role of this virulence factor in T cell activation.

2. Materials and Methods

2.1. Bacterial Strains

COH-1, a highly encapsulated type III GBS isolate extensively described in [16, 22, 24], and its isogenic nonencapsulated (ΔcpsE) mutant [16, 22] were used. GBS strains were cultivated as described previously [22].

2.2. Antibodies

Anti-mouse antibodies (BioLegend unless otherwise noted) used for FACS analysis were as follows: FITC-conjugated anti-CD3 (17A2) and anti-CD4 (GK1.5; BD Pharmingen); PE-conjugated anti-CD4 (GK1.5), anti-CD19 (6D5), anti-CD69 (H1.2F3; BD Pharmingen), anti-IFN-γ (XMG1.2; eBioscience), anti-TNF-α (MP6-XT22; eBioscience), and anti-IL-2 (JES6-5H4; eBioscience); PE-Cy7-conjugated anti-NK-1.1 (PK136) and anti-CD44 (IM7; BD Pharmingen); APC-conjugated anti-IFN-γ (XMG1.2), anti-TNF-α (MP6-XT22) and anti-IL-7Rα (A7R34), and BV421-conjugated anti-CD62L (MEL-14).

2.3. Mice and Experimental Infections

Five-week-old female C57BL/6 mice (Charles River Laboratories) were used for all experiments. The University of Montreal Animal Welfare Committee guidelines and policies were followed. On the day of the experiment, 0.5 mL of the bacterial suspension (106, 107, or 108 CFU) or sterile vehicle solution was administrated intraperitoneally (i.p.). Mortality and clinical signs were monitored [25]. Blood samples (5 μL) were collected at different times after infection. Bacteremia (number of CFU/mL) was determined by plating samples onto blood agar using an Automated Spiral Plater (Spiral Biotech).

2.4. Generation of Bone Marrow-Derived DCs and Isolation of Splenic CD4+ T Cells

DCs were generated as described previously from naïve mice [16]. Cell purity was 86–90% CD11chigh and F4/80−/dim cells by FACS analysis as reported previously [16]. For purification of untouched CD4+ T cells, spleens (from either naïve or infected mice) were harvested, perfused with RPMI complete medium (Gibco), and pressed gently through a sterile fine wire mesh. After red blood cells lysis (eBioscience), total splenocytes were suspended in 2 mM EDTA-PBS solution and separated using Lympholyte-M density gradient (Cedarlane Lab.). Low-density cells at the interphase were purified by magnetic-activated cell sorting (MACS) negative selection (Miltenyi Biotec). The enriched CD4+ T cells had >96% purity by FACS analysis using CD3 and CD4 antibodies (data not shown). For all experiments, cells were incubated at 37°C, 5% CO2.

2.5. In Vivo Infection Model

For survival curves and selection of the infectious dose, mice (n = 16) were injected i.p. with 106, 107, or 108 CFU (strain COH-1) and clinical signs were monitored. Based on the obtained data (Figure 1(a)), mice were injected i.p. with 106 CFU. Surviving animals who displayed clinical signs were boosted with 106 CFU 2 weeks after initial infection. Bacteremia was monitored during 72 h after primary infection or at 24 h after boost. Spleens of animals with clinical signs and positive bacteremia were harvested 96 h after primary infection or 48 h after boost (n = 2 per group × 5 individual experiments). Five hours before spleen collection, mice were injected i.p. with 200 μg of Brefeldin A (eBioscience), a protein transport inhibitor. Control (mock-infected) animals were similarly treated. Brefeldin A was kept throughout the purification steps. The selected time points are based on pretrials analysis (data not shown). Purified CD4+ T cells were analyzed for cytokine production by intracellular flow cytometry (IC-FACS). Total splenocytes were analyzed for memory surface markers by multiparametric FACS. Cells were gated on CD3+ CD4+ double-positive cells, followed by gating CD44high CD62L− (effector [memory] T cells) and CD44high CD62L+ (central memory T cells). Analysis with a fifth surface marker, IL-7Rα +, was used to further identify memory cells (CD44high IL-7Rα +) within these two subsets [26, 27].

Figure 1.

Figure 1

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Survival curves and bacteremia levels of GBS-infected C57BL/6 mice. (a) Mice (n = 16) were injected intraperitoneally with different doses of wild-type GBS serotype III strain COH-1 and survival levels recorded. Mock-infected animals (injected with the vehicle solution) were used as controls. (b) Systemic bacteremia levels of infected mice were monitored at 18 h after infection (for mice infected with 106, 107, and 108 CFU) and at 72 h after infection (for mice infected with 106 CFU). Blood was drawn by tail puncture and serially diluted in PBS prior to plating on blood agar dishes. Individual colonies were counted and data expressed as CFU/mL of blood. ∗ P < 0.05, compared to higher infectious doses.

2.6. Ex Vivo Analysis of Total Splenocytes

Mice were injected i.p with 107 CFU (strain COH-1) (n = 3 per group × 3 individual experiments). Spleens were harvested 6 h after infection. Total splenocytes (5 × 106 cells/mL) were plated in complete medium without antibiotics and incubated for 48 and 72 h. After an initial 4 h incubation, the bacteriostatic agent chloramphenicol (12 μg/mL, Sigma-Aldrich) was added to control the bacterial load as reported previously [16]. Total splenocytes from control (mock-infected) animals were similarly treated. Concanavalin A (ConA, 0.1 μg/mL, Sigma-Aldrich) served as positive control. Supernatants were harvested at different time points for cytokine analysis. In selected experiments, Brefeldin A (3 μg/mL) was added for the last 5 h of incubation, and total splenocytes or CD4+ T cells (MACS-isolated from the culture wells) were analyzed by IC-FACS after a total 48 h incubation. The culture conditions were selected based on pretrials (data not shown).

2.7. In Vitro DC-T Cell Coculture Model

DCs were plated in 48-well flat-bottom plates (105 cells/well; 1 h) prior to a 1 h infection with COH-1 or ΔcpsE strains (MOI:1). After a 1 h treatment with 100 μg/mL gentamycin and 5 μg/mL penicillin G (Sigma-Aldrich) to kill extracellular bacteria as described previously [16], DCs were washed. Freshly isolated CD4+ T cells from naïve mice were added (5 : 1 T cell/DC ratio; 8 and 24 h). Cocultures incubated with medium alone or ConA (0.1 μg/mL) served as negative and positive controls, respectively. Cells were harvested for FACS analysis of surface marker expression. For T cell cytokine expression, after a 48 h incubation, plates were centrifuged and replenished with fresh medium containing 10 ng/mL of mouse rIL-2 (Miltenyi Biotec). After a 3-day resting period, T cells were harvested, washed, and seeded into 96-well flat-bottom culture plates coated with 5 μg/mL of anti-mouse-CD3 mAb (BD Pharmingen) (105 cells/well; 48 h). Supernatants were harvested for ELISA testing. Single cell cultures (DCs or T cells alone) served as controls.

2.8. Cytokine and Chemokine Quantification by ELISA

Levels of IL-6, IL-10, IFN-γ, TNF-α, CCL3, CXCL9, and CXCL10 in cell culture supernatants were measured by sandwich ELISA using pair-matched antibodies (R&D Systems or eBioscience). Sample dilutions giving OD readings in the linear portion of a standard curve were used to quantify the levels of each cytokine. The results include at least three independent ELISA measurements.

2.9. FACS Analysis

For multiparametric IC-FACS, total splenocytes were treated with FcR-blocking reagent (FcγIII/II Rc Ab; BD Pharmingen) for 15 min on ice. Cells were stained for CD19, NK-1.1, CD3, and/or CD69 (30 min on ice), fixed, and permeabilized (eBioscience). After intracellular staining for IFN-γ or TNF-α (45 min, room temperature), FACS was performed using a FACSCanto II instrument (BD Biosciences). Fluorescence Minus One (FMO) control staining was performed for proper analysis and gating of target cells. For IC-FACS of MACS-purified CD4+ T cells from in vivo or ex vivo experiments, cells were stained intracellularly for IFN-γ, TNF-α, and IL-2 as described above and analyzed with a FACSCalibur instrument (BD Biosciences). For analysis of the memory response by multiparametric FACS, total splenocytes were blocked and surface-stained for CD3, CD4, CD44, CD62L, and IL-7Rα (45 min on ice). FACS was performed using a FACSCanto II instrument. Cells from in vitro cocultures were surface-stained for CD4 and CD69 (30 min on ice). FACS was performed using a Cell Lab Quanta™ SC MPL MultiPlate Loader instrument (Beckman Coulter).

2.10. Statistical Analysis

Survival curves of infected mice were generated using Kaplan-Meier plots and log-rank (Mantel-Cox) tests allowed comparison between groups. Bacteremia levels were compared using the Mann-Whitney test. Cytokine data (expressed as means ± SEM) and FACS data were analyzed for significance using Student's unpaired t-test. All analyses were performed using the Sigma Plot System (Systat Software). A P < 0.05 was considered as statistically significant.

3. Results

3.1. Survival of GBS-Infected Mice Is Dose-Dependent

After 18 h, infection with 107 or 108 CFU of COH-1 strain resulted in 75% and 69% mortality (P > 0.05), respectively (Figure 1(a)). Mortality continued to increase until 24 h after infection to 82% and 94% (P > 0.05), respectively, and was maintained until 60 h after infection when the experiment was terminated. Mice infected with 106 CFU were significantly less prone to mortality than mice from the other groups. At 18 h after infection, only a 6% mortality rate was observed, which was significantly lower than in the other groups (P < 0.05). Mortality continued to increase at 24 and 36 h after infection yet remained significantly lower than in mice infected with higher doses (P < 0.05). Indeed, mice infected with 107 or 108 CFU manifested intense clinical signs as early as 8 h after infection, while 106 CFU usually induced less severe signs starting 12 h after infection.

Bacteremia induced by COH-1 infection was consistent with survival curves (Figure 1(b)). Mice infected with 107 or 108 CFU showed high bacteremia at 18 h after infection and reached an average of 2.6 × 108 and 1.3 × 109 CFU/mL, respectively. In contrast, mice infected with 106 CFU showed significantly lower bacteremia and reached an average of 5.7 × 105 CFU/mL. High mortality rates impeded follow-up of bacteremia in mice infected with high doses. However, in mice infected with 106 CFU, bacteremia slowly decreased, reaching an average of 7.2 × 104 CFU/mL at 72 h after infection.

3.2. Splenocytes Produce Type-1 Proinflammatory Cytokines in Response to Encapsulated GBS Infection

Before investigating T cell activation, the splenic immunological environment was characterized. Total splenocytes from mice infected with COH-1 strain were incubated ex vivo for 48 and 72 h (Figure 2). High amounts of IFN-γ, TNF-α, and IL-6 were detected (P < 0.05), suggesting a type-1 proinflammatory response. IL-10 was also upregulated in infected spleens, suggesting a homeostatic role. Important chemokines for T cell recruitment were also detected: CXCL9, CXCL10, and CCL3 (P < 0.05). It is worth noting that CXCL9 and CXCL10 are mainly released in response to IFN-γ activation [28], thus in agreement with the observed high levels of IFN-γ produced by GBS-infected splenocytes. No significant differences were observed between 48 and 72 h cultures, except for CXCL9 where maximal production was delayed to 72 h of incubation.

Figure 2.

Figure 2

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Ex vivo cytokine and chemokine production profile by total splenocytes. C57BL/6 mice were injected intraperitoneally with a dose of 107 CFU of wild-type GBS serotype III strain COH-1 (n = 3 per group × 3 individual experimental infections). Spleens were harvested 6 h after infection and total splenocytes plated at 5 × 106 cells/well. After 4 h of incubation, the bacteriostatic agent chloramphenicol (12 μg/mL) was added to the culture to prevent cell toxicity. Cells were then incubated for 48 h and 72 h and supernatants were collected for cytokine analysis by ELISA. Nonstimulated cells from mock-infected animals served as negative (−) control for basal expression. Cells stimulated with Concanavalin A (0.1 μg/mL) were used as positive (+) control. Data are expressed as means ± SEM (in pg/mL) from 3 different experimental infections. ∗ P < 0.05 indicates statistically significant difference compared to (−) control cells.

3.3. Activated CD4+ T Cells Contribute to IFN-γ Production during Encapsulated GBS Infection

With current understanding of the splenic environment, the contribution of activated T cells to cytokine production was investigated. A multiparametric IC-FACS analysis of IFN-γ production from ex vivo total splenocytes cultures was performed. CD3+ T cells markedly contributed to the IFN-γ response in the spleen of infected mice (Figure 3(a); P < 0.05). NKT cells (NK1.1+ CD3+) produced very low levels of IFN-γ (data not shown). NK cells (NK1.1+) were major contributors to IFN-γ production within the CD3− population (data not shown). As expected, B cells (CD19+) did not produce significant levels of this cytokine (data not shown). Activated CD3+ T cells also contributed to approximately half the production of TNF-α by splenic cells (Figure 3(c); P < 0.05). Compared to control mice, splenocytes from infected animals showed a significant increase in surface expression of the early activation marker CD69. High expression of CD69 was also observed within the CD3+ population (Figure 3(b); P < 0.05).

Figure 3.

Figure 3

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Ex vivo analyses of cellular sources of IFN-γ during GBS infection. C57BL/6 mice were injected intraperitoneally with a dose of 107 CFU of wild-type GBS serotype III strain COH-1 (n = 3 per group × 3 individual experimental infections). Spleens were harvested 6 h after infection and total splenocytes plated at 5 × 106 cells/well. After 4 h of incubation, the bacteriostatic agent chloramphenicol (12 μg/mL) was added to the culture to prevent cell toxicity. Nonstimulated cells from mock-infected animals served as negative (−) control for basal expression. Total splenocytes were incubated for 48 h with Brefeldin A (3 μg/mL) added during the last 5 h of incubation. Cells were harvested and intracellularly stained for IFN-γ (a) or surface-stained for CD69 (b) in combination with several surface markers for multiparametric FACS analysis. Representative data from 3 different experimental infections based on CD3+ population or total splenic population (Void). (c) Number of TNF-α + cells within the CD3+ population or total splenic population (All). Data are expressed as means ± SEM from 3 different experimental infections; ∗ P < 0.05 indicates statistically significant difference compared to (−) control cells. Fifty thousand gated events were acquired per sample and data analysis was performed using FACSDiva™ software.

CD4+ T cells were isolated from ex vivo total splenocyte cultures and analyzed by IC-FACS to specifically evaluate their role (Figure 4). Activated CD4+ T cells contributed to the production of IFN-γ and TNF-α. Low levels of intracellular IL-2 were also observed (Figure 4). In vivo experiments confirmed these results; CD4+ T cells directly isolated from the spleen of infected mice 96 h after primary infection showed that they contribute to the production of IFN-γ and TNF-α. Intracellular levels of IL-2 were hardly detected during a primary infection (Figure 5, black histograms). CD4+ T cells isolated 48 h after boost displayed an enhanced contribution to IFN-γ, TNF-α, and IL-2 production (Figure 5, dark grey histograms). This is consistent with the generation of memory CD4+ T cells (CD44high IL-7Rα +) observed at that time with the increase in IL-7Rα + cells in the central memory subset (CD44high CD62L+) (Figures 6(a) and 6(b), red population and histograms). The decrease in IL-7Rα + cells in the effector (memory) subset (CD44high CD62L−) likely reflects cellular migration from the spleen to peripheral tissues (Figures 6(a) and 6(b), blue population and histograms).

Figure 4.

Figure 4

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Ex vivo analyses of CD4+ T cell contribution to cytokine production. C57BL/6 mice were injected intraperitoneally with a dose of 107 CFU of wild-type GBS serotype III strain COH-1 (n = 3 per group × 3 individual experimental infections). Spleens were harvested 6 h after infection and total splenocytes plated at 5 × 106 cells/well. After 4 h of incubation, the bacteriostatic agent chloramphenicol (12 μg/mL) was added to the culture to prevent cell toxicity. Nonstimulated cells from mock-infected animals served as negative (−) control for basal expression. Cells stimulated with Concanavalin A (0.1 μg/mL) were used as positive (+) control. Total splenocytes were incubated for 48 h. Brefeldin A (3 μg/mL) was added during the last 5 h of incubation and CD4+ T cells were MACS-isolated from the culture, stained intracellularly for different cytokines, and analyzed by FACS. Data are expressed as means ± SEM (in % of positive cells) from 3 individual experimental infections. ∗ P < 0.05 indicates statistically significant difference compared to (−) control cells. Twenty thousand gated events were acquired per sample and data analysis was performed using CellQuest software. Histograms were drawn based on PE-control stain and were plotted on logarithmic scales.

Figure 5.

Figure 5

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In vivo CD4+ T cell contribution to cytokine production during primary and secondary GBS infections. C57BL/6 mice were injected intraperitoneally with a dose of 106 CFU of wild-type GBS serotype III strain COH-1. Surviving animals who had previously displayed clinical signs were boosted with a second dose of 106 CFU of GBS strain COH-1 two weeks after initial infection. Spleens of animals with clinical signs and positive bacteremia were harvested 96 h after primary infection or 48 h after boost infection (n = 2 per group × 5 individual experimental infections). Five hours prior to spleen collection, mice were injected with Brefeldin A (200 μg). (−) Control animals were similarly treated. Splenic CD4+ T cells were MACS-purified, stained intracellularly for different cytokines, and analyzed by FACS. Representative data from 5 different experimental infections. Cytokine basal expression levels in (−) control animals were similar at 96 h after primary mock-infection and 48 h after secondary mock-infection. Representative histograms from the latter time point were selected for the figure. Twenty thousand gated events were acquired per sample and data analysis was performed using CellQuest software. Histograms were drawn based on PE-control stain and were plotted on logarithmic scales. It should be noted that isotype controls are the same in both groups, but only displayed on left panels to simplify the figure.

Figure 6.

Figure 6

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In vivo generation of memory CD4+ T cells during GBS infection. C57BL/6 mice were injected intraperitoneally with a dose of 106 CFU of wild-type GBS serotype III strain COH-1. Surviving animals who had previously displayed clinical signs were boosted with a second dose of 106 CFU of GBS strain COH-1 two weeks after initial infection. Spleens of animals with clinical signs and positive bacteremia were harvested 48 h after boost infection. Total splenocytes were stained and analyzed by multiparametric FACS. (a) Cells were gated on CD3+ CD4+ double-positive cells, followed by gating CD44high CD62L− (effector [memory] T cells) and CD44high CD62L+ (central memory T cells). A histogram from a representative control (mock-infected) mouse was selected for the figure. (b) A fifth surface marker, IL-7Rα +, was used to further identify memory cells (CD44high IL-7Rα +) within the CD44high CD62L− (effector [memory] T cells) and CD44high CD62L+ (central memory T cells). IL-7Rα + cells reflect memory cells within these respective populations. Histograms from representative control (mock-infected) and infected mice were selected for the figure. Thirty thousand events gated on CD3+ CD4+ cells were acquired per sample and data analysis was performed using Kaluza® Flow Analysis software.

3.4. The CPS of GBS Modulates Cytokine Release by CD4+ T Cells

As GBS is a well-encapsulated bacterium, the impact of CPS on CD4+ T cell activation was evaluated by comparing COH-1 with its nonencapsulated mutant, ΔcpsE, in an in vitro DC-T cell coculture system. Since nonencapsulated GBS mutants are rapidly cleared from circulation [20], in vivo comparison was impossible. Coculture supernatants were tested by ELISA for CD4+ T cell-derived cytokines. No significant cytokine production was observed in single cell cultures (DCs or T cells alone) that served as controls (data not shown). COH-1-activated cocultures showed extremely high levels of IFN-γ (~45000 pg/mL) and significant levels of TNF-α (~1500 pg/mL). ΔcpsE-activated cocultures showed a significant reduction in IFN-γ production (Figure 7; P = 0.012), along with reduced TNF-α production, although this difference was not statistically significant (P = 0.053). Overall, these results suggest that nonencapsulated GBS-pulsed DCs induce reduced cytokine production by CD4+ T cells compared to encapsulated GBS-pulsed DCs.

Figure 7.

Figure 7

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Role of bacterial capsular polysaccharide in the modulation of cytokine production by CD4+ T cells. Dendritic cells (DCs) were infected with either wild-type GBS strain COH-1 or its nonencapsulated isogenic mutant ΔcpsE (MOI:1) for 1 h. Extracellular bacteria were killed by antibiotic treatment and cultures washed prior to addition of freshly isolated splenic CD4+ T cells from naïve mice (T cell : DC ratio of 5 : 1). Cocultures were incubated for 48 h, resuspended in fresh medium containing 10 ng/mL of IL-2 for 72 h (resting period), and then transferred to anti-CD3 coated plates for 48 h. Supernatants were then collected and cytokines quantified by ELISA. Nonstimulated cocultures served as negative (−) controls for basal expression. Data are expressed as means ± SEM (in pg/mL) from 5 different experiments. ∗ P < 0.05 indicates statistically significant differences compared to (−) control. # P < 0.05 indicates statistically significant differences between cocultures infected with wild-type strain COH-1 and those infected with the nonencapsulated mutant ΔcpsE.

3.5. The CPS of GBS Affects Surface Expression of CD69 on Activated CD4+ T Cells

In addition to cytokine production, expression of surface molecules is essential for proper T cell activation. The effect of CPS on CD69 expression on activated CD4+ T cells was investigated. In COH-1-activated cocultures, CD69 expression on CD4+ T cells was significantly lower than in ΔcpsE-activated cocultures after an 8 h incubation (Figure 8; P < 0.01). CD69 expression remained lower in COH-1-activated cocultures at 24 h (P < 0.05), although the difference and levels of expression were less pronounced. After 48 h, no significant differences in CD69 expression were observed between strains (data not shown).

Figure 8.

Figure 8

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Role of bacterial capsular polysaccharide in the modulation of CD4+ T cell surface expression of CD69. Dendritic cells (DCs) were infected with either wild-type GBS strain COH-1 or its nonencapsulated isogenic mutant ΔcpsE (MOI:1) for 1 h. Extracellular bacteria were killed by antibiotic treatment and cultures washed prior to addition of freshly isolated splenic CD4+ T cells from naïve mice (T cell : DC ratio of 5 : 1). Cocultures were incubated for 8 h and 24 h, cells were harvested, and CD69 expression was analyzed by FACS. Cocultures incubated with medium alone or Concanavalin (0.1 μg/mL) served as negative (−) and positive controls (+), respectively. (a) Representative data from 3 different experiments. Twenty thousand gated events were acquired per sample and data analysis was performed using Cell Lab Quanta Collection/Analysis software. Quadrants were drawn based on FITC- and PE-control stains and were plotted on logarithmic scales. Numbers in the upper quadrants indicate the % of CD4+ CD69+ cells. (b) Data are expressed as means ± SEM from 3 different experimental infections; ∗ P < 0.05 indicates statistically significant differences between cocultures infected with wild-type strain COH-1 and those infected with the nonencapsulated mutant ΔcpsE.

4. Discussion

Although interactions between GBS and innate immune cells are increasingly documented, activation profiles of adaptive immune cells have never been investigated. This is the first study evaluating CD4+ T cells contribution to GBS immune response using in vivo, ex vivo, and in vitro analysis.

While cytokines contribute to host defense development, they can also exacerbate GBS-induced pathologies. Initial ex vivo analysis of cytokine production by total splenocytes from encapsulated GBS-infected mice revealed the presence of IFN-γ, TNF-α, IL-6, and IL-10. Production of IFN-γ, TNF-α, and IL-6 suggests a type-1 proinflammatory response being developed shortly after infection, while IL-10 production can be related to immune regulation. Interestingly, TNF-α and IL-6 have routinely been reported as mediators of GBS sepsis [7, 10]. This result might also highlight the homeostatic role of IL-10. Indeed, IL-10 was shown to reduce TNF-α and thus protect neonatal mice from developing GBS sepsis [7].

DCs, monocytes, and macrophages are known to secrete TNF-α, IL-6, and/or IL-10 when responding to GBS [16, 17, 29–31]. However, sources of IFN-γ remain poorly identified. Early works reporting IFN-γ production used GBS-infected total splenocytes or mixed mononuclear cells, without identifying the cellular source [8–10, 17]. The present study defined the role of T cells in IFN-γ production. Ex vivo and in vivo analysis showed that CD4+ T cells are important producers of IFN-γ and TNF-α during GBS infection. Activated CD4+ T cells also produce low, but still significant levels of IL-2, suggesting the development of a Th1 response. CD4+ T cells produce the same pattern of cytokines more efficiently after a boost infection, likely thanks to the memory response [32]. An important contribution of NK cells to the IFN-γ response was also evidenced in vivo, in accordance with previous in vitro studies with splenocytes from severe combined immunodeficiency mice [15]. IFN-γ production by NKT cells was very limited during GBS infection, even at earlier time points (unpublished observations), although purified GBS glycolipids have been shown to activate NKT cells [14].

Early chemokine release by innate immune cells attracts T cells to the site of infection. Ex vivo analysis of chemokine production by total splenocytes suggested that T cells are actively recruited via CCL3, CXCL9, and CXCL10. Interestingly, CXCL9 and CXCL10 are two CXCR3 ligands, both induced by IFN-γ. CXCR3 is rapidly upregulated on naive T cells following activation and remains preferentially highly expressed on Th1 cells [28]. Different splenic cell types, like DCs, might produce these chemokines in response to GBS [16]. Although upregulation of Cxcl10 gene expression was observed in mouse peritoneal macrophages [31], GBS was unable to induce either CXCL10 or CXCL9 secretion by these cells [33]. Nevertheless, both macrophages and DCs seem to contribute to CCL3 production [31, 33, 34].

As GBS possesses a thick CPS, its most important virulence factor, the potential of CPS to modulate CD4+ T cell activation was investigated. Similarly to ex vivo and in vivo results, DCs pulsed in vitro with encapsulated GBS induced the release of high levels of IFN-γ and TNF-α by CD4+ T cells. The production of IFN-γ was significantly decreased with nonencapsulated GBS. Production of TNF-α was also reduced. It is surprising that the loss of capsule does not trigger an exaggerated response or increased IFN-γ production by T cells, as reported for other encapsulated pathogens [35–37]. However, studies on GBS-activated DCs have shown similar trends; encapsulated GBS induced similar or stronger cytokine production by infected DCs than nonencapsulated GBS-infected counterparts [16, 34]. The only exception was IL-10, where production was significantly higher in DCs infected with the nonencapsulated mutant [16]. Two interrelated hypotheses were suggested to explain these observations: (a) increased IL-10 production by DCs reduces the production of other cytokines; or (b) more efficient killing of the nonencapsulated mutant reduces cytokine production by DCs [16, 22]. Moreover, it was reported that the presence of CPS modulates the endocytic pathways used by DCs for GBS uptake [22]. Since the route of entry influences the repertoires of epitopes presented to CD4+ T cells, the ensuing immune response might be affected [38]. Thus, in our DC-T cell coculture system, DC modulation by the nonencapsulated strain may lead to lower levels of IFN-γ production by CD4+ T cells.

In contrast to cytokine production, the surface expression of CD69 was higher (early time points) or similar (late time points) in CD4+ T cells cocultured with nonencapsulated mutant-pulsed DCs compared to encapsulated GBS-infected cocultures. However, this could just be related to different kinetics of CD69 expression. In fact, attempting to explain modulation of CD69 expression on CD4+ T cells is quite difficult, due to limited information on this marker. Indeed, characterization of its ligand has just started [39]. CD69 is known to be one of the earliest markers induced upon activation of T cells and acts as a signal-transmitting receptor for immunoregulatory events [40]. Of the few studies available on CD69 expression by T cells upon streptococcal infection, Harimaya et al. demonstrated a dose-dependent upregulation of CD69 on CD3+ T cells from peripheral blood lymphocytes infected with Streptococcus pneumoniae. Yet, authors failed to correlate CD69 expression and IFN-γ production by these target cells [41]. More recently, in a S. pneumoniae mouse model of infection, CD4+ T cells exhibited significant upregulation of CD69 in the spleen. As this response was MHC-II unrestricted, authors suggested that this increased CD69 expression on T cells might be due to secondary factors like cytokine release by other cells [42]. Likely, a polyclonal (indirect) activation of T cells in our system cannot be ruled out, although GBS failed to directly activate T cells without antigen-presenting cells (data not shown), similarly to that reported for S. pneumoniae [37, 42]. Finally, it has been suggested that CD69 plays an immunoregulatory role by preventing infection-induced immunopathology [43]. Enhanced expression of CD69 may result in reduced IFN-γ production by CD4+ T cells [44].

5. Conclusion

Undoubtedly, IFN-γ production by CD4+ T cells during GBS infection is crucial for host defense [8] but might also result in disease pathology, as suggested in the mouse model of pneumococcal sepsis [42]. Although this study characterized for the first time IFN-γ production by CD4+ T cells, a definitive understanding of all mechanisms regulating IFN-γ production during GBS infection requires further research. For instance, as the CPS confers a survival advantage to GBS [16, 22], persistence of GBS within antigen-presenting cells may affect their activation and thus the ensuing T cell immune response, including altered IFN-γ and CD69 expression balance early during infection.

Acknowledgments

This work was supported by Natural Sciences and Engineering Research Council of Canada (NSERC no. 342150-2013 to Mariela Segura) and by Canadian Institutes of Health Research (CIHR) and Canada Foundation for Innovation (CFI) through grants to Jacques Thibodeau (CIHR no. 93592). Corinne Letendre is the recipient of a M.S. award granted by NSERC. Marie-Pier Lecours and Paul Lemire are the recipients of Ph.D. awards granted by NSERC and by the Fonds de recherche du Québec-Nature et technologies, respectively.

Conflict of Interests

The authors declare that they have no conflict of interests in the research.

Authors' Contribution

Damian Clarke and Corinne Letendre contributed equally to this work.

References

  • 1.Melin P. Neonatal group B streptococcal disease: from pathogenesis to preventive strategies. Clinical Microbiology and Infection. 2011;17(9):1294–1303. doi: 10.1111/j.1469-0691.2011.03576.x. [DOI] [PubMed] [Google Scholar]
  • 2.Verani J. R., Schrag S. J. Group B streptococcal disease in infants: progress in prevention and continued challenges. Clinics in Perinatology. 2010;37(2):375–392. doi: 10.1016/j.clp.2010.02.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 3.Edwards M. S., Baker C. J. Group B streptococcal infections in elderly adults. Clinical Infectious Diseases. 2005;41(6):839–847. doi: 10.1086/432804. [DOI] [PubMed] [Google Scholar]
  • 4.Maisey H. C., Doran K. S., Nizet V. Recent advances in understanding the molecular basis of group B Streptococcus virulence. Expert Reviews in Molecular Medicine. 2008;10, article e27 doi: 10.1017/S1462399408000811. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5.Wennekamp J., Henneke P. Induction and termination of inflammatory signaling in group B streptococcal sepsis. Immunological Reviews. 2008;225(1):114–127. doi: 10.1111/j.1600-065X.2008.00673.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 6.Cusumano V., Midiri A., Cusumano V. V., et al. Interleukin-18 is an essential element in host resistance to experimental group B streptococcal disease in neonates. Infection and Immunity. 2004;72(1):295–300. doi: 10.1128/iai.72.1.295-300.2004. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7.Cusumano V., Genovese F., Mancuso G., Carbone M., Fera M. T., Teti G. Interleukin-10 protects neonatal mice from lethal group B streptococcal infection. Infection and Immunity. 1996;64(7):2850–2852. doi: 10.1128/iai.64.7.2850-2852.1996. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 8.Cusumano V., Mancuso G., Genovese F., et al. Role of gamma interferon in a neonatal mouse model of group B streptococcal disease. Infection and Immunity. 1996;64(8):2941–2944. doi: 10.1128/iai.64.8.2941-2944.1996. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 9.Mancuso G., Cusumano V., Genovese F., Gambuzza M., Beninati C., Teti G. Role of interleukin 12 in experimental neonatal sepsis caused by group B streptococci. Infection and Immunity. 1997;65(9):3731–3735. doi: 10.1128/iai.65.9.3731-3735.1997. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 10.Teti G., Mancuso G., Tomasello F. Cytokine appearance and effects of anti-tumor necrosis factor alpha antibodies in a neonatal rat model of group B streptococcal infection. Infection and Immunity. 1993;61(1):227–235. doi: 10.1128/iai.61.1.227-235.1993. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 11.Lewis D. B., Larsen A., Wilson C. B. Reduced interferon-gamma mRNA levels in human neonates. Evidence for an intrinsic T cell deficiency independent of other genes involved in T cell activation. The Journal of Experimental Medicine. 1986;163(4):1018–1023. doi: 10.1084/jem.163.4.1018. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 12.Wilson C. B. Immunologic basis for increased susceptibility of the neonate to infection. The Journal of Pediatrics. 1986;108(1):1–12. doi: 10.1016/s0022-3476(86)80761-2. [DOI] [PubMed] [Google Scholar]
  • 13.Lione V. D. O. F., dos Santos M. H. B., de Oliveira J. S. S., Mattos-Guaraldi A. L., Nagao P. E. Interferon-γ inhibits group B Streptococcus survival within human endothelial cells. Memorias do Instituto Oswaldo Cruz. 2014;109(7):940–943. doi: 10.1590/0074-0276140201. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 14.Kinjo Y., Illarionov P., Vela J. L., et al. Invariant natural killer T cells recognize glycolipids from pathogenic Gram-positive bacteria. Nature Immunology. 2011;12(10):966–974. doi: 10.1038/ni.2096. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 15.Derrico C. A., Goodrum K. J. Interleukin-12 and tumor necrosis factor alpha mediate innate production of gamma interferon by group B Streptococcus-treated splenocytes of severe combined immunodeficiency mice. Infection and Immunity. 1996;64(4):1314–1320. doi: 10.1128/iai.64.4.1314-1320.1996. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 16.Lemire P., Houde M., Lecours M.-P., Fittipaldi N., Segura M. Role of capsular polysaccharide in Group B Streptococccus interactions with dendritic cells. Microbes and Infection. 2012;14(12):1064–1076. doi: 10.1016/j.micinf.2012.05.015. [DOI] [PubMed] [Google Scholar]
  • 17.Kwak D. J., Augustine N. H., Borges W. G., Joyner J. L., Green W. F., Hill H. R. Intracellular and extracellular cytokine production by human mixed mononuclear cells in response to group B streptococci. Infection and Immunity. 2000;68(1):320–327. doi: 10.1128/iai.68.1.320-327.2000. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 18.La Pine T. R., Joyner J. L., Augustine N. H., Kwak S. D., Hill H. R. Defective production of IL-18 and IL-12 by cord blood mononuclear cells influences the T helper-1 interferon gamma response to group B streptococci. Pediatric Research. 2003;54(2):276–281. doi: 10.1203/01.pdr.0000072515.10652.87. [DOI] [PubMed] [Google Scholar]
  • 19.Cieslewicz M. J., Chaffin D., Glusman G., et al. Structural and genetic diversity of group B Streptococcus capsular polysaccharides. Infection and Immunity. 2005;73(5):3096–3103. doi: 10.1128/iai.73.5.3096-3103.2005. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.Doran K. S., Nizet V. Molecular pathogenesis of neonatal group B streptococcal infection: no longer in its infancy. Molecular Microbiology. 2004;54(1):23–31. doi: 10.1111/j.1365-2958.2004.04266.x. [DOI] [PubMed] [Google Scholar]
  • 21.Carlin A. F., Uchiyama S., Chang Y.-C., Lewis A. L., Nizet V., Varki A. Molecular mimicry of host sialylated glycans allows a bacterial pathogen to engage neutrophil Siglec-9 and dampen the innate immune response. Blood. 2009;113(14):3333–3336. doi: 10.1182/blood-2008-11-187302. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 22.Lemire P., Houde M., Segura M. Encapsulated group B Streptococcus modulates dendritic cell functions via lipid rafts and clathrin-mediated endocytosis. Cellular Microbiology. 2012;14(11):1707–1719. doi: 10.1111/j.1462-5822.2012.01830.x. [DOI] [PubMed] [Google Scholar]
  • 23.Costa A., Gupta R., Signorino G., et al. Activation of the NLRP3 inflammasome by group B Streptococci . The Journal of Immunology. 2012;188(4):1953–1960. doi: 10.4049/jimmunol.1102543. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Mancuso G., Gambuzza M., Midiri A., et al. Bacterial recognition by TLR7 in the lysosomes of conventional dendritic cells. Nature Immunology. 2009;10(6):587–594. doi: 10.1038/ni.1733. [DOI] [PubMed] [Google Scholar]
  • 25.Lemire P., Calzas C., Segura M. The NOD2 receptor does not play a major role in the pathogenesis of Group B Streptococcus in mice. Microbial Pathogenesis. 2013;65:41–47. doi: 10.1016/j.micpath.2013.09.006. [DOI] [PubMed] [Google Scholar]
  • 26.Stephens R., Langhorne J. Effector memory Th1 CD4 T cells are maintained in a mouse model of chronic malaria. PLoS Pathogens. 2010;6(11) doi: 10.1371/journal.ppat.1001208.e1001208 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 27.Khan M. N., Pichichero M. E. CD4 T cell memory and antibody responses directed against the pneumococcal histidine triad proteins PhtD and PhtE following nasopharyngeal colonization and immunization and their role in protection against pneumococcal colonization in mice. Infection and Immunity. 2013;81(10):3781–3792. doi: 10.1128/IAI.00313-13. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 28.Groom J. R., Luster A. D. CXCR3 in T cell function. Experimental Cell Research. 2011;317(5):620–631. doi: 10.1016/j.yexcr.2010.12.017. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Bebien M., Hensler M. E., Davanture S., et al. The pore-forming toxin β hemolysin/cytolysin triggers p38 MAPK-dependent IL-10 production in macrophages and inhibits innate immunity. PLoS Pathogens. 2012;8(7) doi: 10.1371/journal.ppat.1002812.e1002812 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 30.De Francesco M. A., Gargiulo F., Negrini R., Gelmi M., Manca N. Different sequence strains of Streptococcus agalactiae elicit various levels of cytokine production. Immunological Investigations. 2008;37(8):741–751. doi: 10.1080/08820130802403283. [DOI] [PubMed] [Google Scholar]
  • 31.Draper D. W., Bethea H. N., He Y.-W. Toll-like receptor 2-dependent and -independent activation of macrophages by group B streptococci. Immunology Letters. 2006;102(2):202–214. doi: 10.1016/j.imlet.2005.09.005. [DOI] [PubMed] [Google Scholar]
  • 32.Zhang Q., Bagrade L., Clarke E., Paton J. C., Nunez D. A., Finn A. Bacterial lipoproteins differentially regulate human primary and memory CD4+ T and B cell responses to pneumococcal protein antigens through toll-like receptor 2. Journal of Infectious Diseases. 2010;201(11):1753–1763. doi: 10.1086/652495. [DOI] [PubMed] [Google Scholar]
  • 33.Fan H., Williams D. L., Zingarelli B., et al. Differential regulation of lipopolysaccharide and Gram-positive bacteria induced cytokine and chemokine production in macrophages by Gαi proteins. Immunology. 2007;122(1):116–123. doi: 10.1111/j.1365-2567.2007.02619.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 34.Lemire P., Roy D., Fittipaldi N., et al. Implication of TLR- but not of NOD2-signaling pathways in dendritic cell activation by group B Streptococcus serotypes III and V. PLoS ONE. 2014;9(12) doi: 10.1371/journal.pone.0113940.e113940 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 35.Lecours M.-P., Gottschalk M., Houde M., Lemire P., Fittipaldi N., Segura M. Critical role for Streptococcus suis cell wall modifications and suilysin in resistance to complement-dependent killing by dendritic cells. Journal of Infectious Diseases. 2011;204(6):919–929. doi: 10.1093/infdis/jir415. [DOI] [PubMed] [Google Scholar]
  • 36.Kolb-Mäurer A., Unkmeir A., Kämmerer U., et al. Interaction of Neisseria meningitidis with human dendritic cells. Infection and Immunity. 2001;69(11):6912–6922. doi: 10.1128/iai.69.11.6912-6922.2001. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 37.Olliver M., Hiew J., Mellroth P., Henriques-Normark B., Bergman P. Human monocytes promote Th1 and Th17 responses to Streptococcus pneumoniae . Infection and Immunity. 2011;79(10):4210–4217. doi: 10.1128/iai.05286-11. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 38.von Delwig A., Bailey E., Gibbs D. M., Robinson J. H. The route of bacterial uptake by macrophages influences the repertoire of epitopes presented to CD4 T cells. European Journal of Immunology. 2002;32(12):3714–3719. doi: 10.1002/1521-4141(200212)32:12<3714::AID-IMMU3714>3.0.CO;2-Y. [DOI] [PubMed] [Google Scholar]
  • 39.Lin C. R., Wei T. W., Tsai H. Y., Wu Y. T., Wu P. Y., Chen S. T. Glycosylation-dependent interaction between CD69 and S100A8/S100A9 complex is required for regulatory T-cell differentiation. The FASEB Journal. 2015;29(12):5006–5017. doi: 10.1096/fj.15-273987. [DOI] [PubMed] [Google Scholar]
  • 40.Ziegler S. F., Ramsdell F., Alderson M. R. The activation antigen CD69. STEM CELLS. 1994;12(5):456–465. doi: 10.1002/stem.5530120502. [DOI] [PubMed] [Google Scholar]
  • 41.Harimaya A., Himi T., Fujii N., et al. Induction of CD69 expression and Th1 cytokines release from human peripheral blood lymphocytes after in vitro stimulation with Alloiococcus otitidis and three middle ear pathogens. FEMS Immunology and Medical Microbiology. 2005;43(3):385–392. doi: 10.1016/j.femsim.2004.10.014. [DOI] [PubMed] [Google Scholar]
  • 42.LeMessurier K., Häcker H., Tuomanen E., Redecke V. Inhibition of T cells provides protection against early invasive pneumococcal disease. Infection and Immunity. 2010;78(12):5287–5294. doi: 10.1128/IAI.00431-10. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 43.Vega-Ramos J., Alari-Pahissa E., Valle J. D., et al. CD69 limits early inflammatory diseases associated with immune response to Listeria monocytogenes infection. Immunology and Cell Biology. 2010;88(7):707–715. doi: 10.1038/icb.2010.62. [DOI] [PubMed] [Google Scholar]
  • 44.Radulovic K., Manta C., Rossini V., et al. CD69 regulates type I IFN-induced tolerogenic signals to mucosal CD4 T cells that attenuate their colitogenic potential. The Journal of Immunology. 2012;188(4):2001–2013. doi: 10.4049/jimmunol.1100765. [DOI] [PubMed] [Google Scholar]

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