Research Article | Open Access
Linking Innate and Adaptive Immunity: Human V9V2 T Cells Enhance CD40 Expression and HMGB-1 Secretion
T cells play an important role in regulating the immune response to stress stimuli; however, the mean by which these innate lymphocytes fulfill this function remains poorly defined. The main subset of human peripheral blood T cells responds to nonpeptidic antigens, such as isopentylpyrophosphate (IPP), a metabolite in the mevalonate pathway for both eukaryote and prokaryote cells. IPP-primed T cells significantly augment the inflammatory response mediated by monocytes and T cells to TSST-1, the staphylococcal superantigen that is the major causative agent of toxic shock syndrome. Here we show that the small pool of activated peripheral T cells induces an early upregulation of CD40 on monocytes and the local release of High Mobility Group Box-1 (HMGB-1), the molecule designated as the late mediator of systemic inflammation. This finding provides a new basis for how T cells may serve as influential modulators of both endogenous and exogenous stress stimuli.
γδ T cells have a nonredundant role in regulating immune homeostasis. In comparison to αβ T cells, they lack receptor diversity yet demonstrate remarkable plasticity in response to both infectious and noninfectious stimuli. As an extension of their dichotomous nature, γδ T cells have been held liable for both instigating over-zealous immune responses [1–3] as well as reigning in inflammation by controlling activated macrophages and promoting wound healing [4–6]. In humans, the main subset of peripheral blood γδ T cells usually comprises between 1 and 5% of circulating T cells and bears the canonical Vγ9Vδ2 T cell receptor. These Vγ9Vδ2 T cells are unique to primates, and they respond to endogenous and exogenous stress-induced molecules that are nonpeptidic in nature and preclude the requirement for processing or presentation by classical MHC molecules [7–9]. Isopentylpyrophosphate (IPP) is the prototypical phosphoantigen recognized by Vγ9Vδ2 T cells that was first isolated from lysates of mycobacteria . It was later determined to be a metabolite in the mevalonate pathway in all eukaryotic and some prokaryotic cells, including Staphylococcus aureus [10, 11]. During the initial phase of infection with low bacterial inocula of S. aureus, Vγ9Vδ2 T cells are activated by endogenous mevalonate metabolites through the accumulation and dephosphorylation of the hydroxymethylglutaryl-coenzyme A reductase, the rate-limiting enzyme of the mevalonate pathway . Therefore, primates have evolved the ability to readily respond to bacterial infection as well as endogenous damage by sensing the dysregulation of the mevalonate pathway, which may be considered a stress-associated “alarmin” for these primordial lymphocytes.
We have shown that stimulating the small pool of human γδ T cells present in PBMC with IPP markedly augmented the early proinflammatory response to Toxic Shock Syndrome Toxin-1 (TSST-1) . TSST-1 is a staphylococcal superantigen that exerts a potent inflammatory response by bridging Vβ2 specific αβ T cell receptors with conserved regions of the MHC class II molecules of antigen presenting cells (APCs) outside the peptide-binding groove . Ferry et al.  demonstrated the presence of specific Vβ T cell signatures of various superantigenic toxins, including TSST-1, in the blood of patients with staphylococcal TSS. We previously demonstrated that IPP-activated γδ T cells augment the levels of proinflammatory cytokines within the first 6 hours post-TSST-1 treatment, thereby changing the kinetics and magnitude of the immune response to the superantigen . We have also shown that High Mobility Group Box Protein-1 (HMGB-1) is released following TSST-1 stimulation . HMGB-1 is a highly conserved nonhistone DNA-binding protein found in virtually all nucleated cells and is regarded as being the late mediator of sepsis . Activated monocytes secrete HMGB-1 after exposure to endotoxin , and it is detectable in the serum of septic patients within 24 hours. Importantly, neutralizing the effects of HMGB-1 at this late time point, either by anti-HMGB-1 antibodies or antagonists, rescued mice from sepsis-induced mortality . In contrast to endotoxin, which activates only macrophages to secrete HMGB-1, both T cells and macrophages participate in the nuclear translocation and subsequent release of HMGB-1 into the extracellular environment following TSST-1 stimulation .
The first aim of the present study was to evaluate the influence exerted by IPP-primed Vγ9Vδ2 T cells on the change in costimulatory molecule expression that could explain their ability to enhance the immune response to TSST-1. The second objective was to determine the consequence of γδ T cell mediated immune modulation on the expression and secretion of HMGB-1.
2. Materials and Methods
2.1. Toxin Purification
Recombinant TSST-1 was purified from culture supernatants of S. aureus strain RN4220 previously transformed to carry the tst gene, using both preparative isoelectric focusing and chromatofocusing . Toxin purity was assessed by silver staining after sodium dodecyl sulfate-polyacrylamide gel electrophoresis on 14% acrylamide gels, and LPS activity was undetectable by the Limulus amoebocyte lysate gelation (sensitivity limit, 10 pg/mL).
2.2. Preparation of Cells and Culture Conditions
Fresh human peripheral blood mononuclear cells (PBMC) from healthy donors were obtained by Ficoll-Paque PLUS (Amersham Biosciences Corp., Piscataway, NJ) density centrifugation, and cultured in 96-well U-bottom plates at cells/ml in complete culture medium consisting of RPMI 1640 (StemCell Technologies Inc., Vancouver, BC, Canada), 10% heat-inactivated fetal bovine serum (HyClone Laboratories Inc., Logan, UT), 2 mM L-glutamine (StemCell), 25 mM Hepes buffer (StemCell), and 2 ug/ml of polymyxin B sulphate (Sigma-Aldrich Corp., St. Louis, MO). Depletion of γδ T cells was accomplished by immunomagnetic positive cell selection with an anti-γδ TCR MAb (clone Immu510, BD BioSciences Pharmingen Inc., San Diego, CA) conjugated to an antidextran MAb tetramer (StemCell), which left the rest of the PBMC untouched, using the StemSep protocol (StemCell). Purity of the γδ T cell-depleted PBMC was analyzed by flow cytometry using phycoerythrin-(PE-) conjugated anti-Vδ2 antibody (BD BioSciences Pharmingen). Figure 1 shows the population of Vγ9Vδ2 T cells in PBMCs before (which made up 1.5% of live cells) and after depletion (0.1%).
2.3. Treatment of PBMC with IPP and TSST-1
PBMCs with or without γδ T cell depletion were treated with either 45 M IPP (Sigma-Aldrich) or left untreated in complete growth medium for 16–18 hours (overnight) at C, 5% C prior to treatment with 1 nM TSST-1. For secreted HMGB-1 detection, culture supernatants were microcentrifuged at for 5 minutes and frozen at C until analysis.
2.4. Flow Cytometric Analysis of Surface-Expressed HMGB-1 on Differentiated Cells and Expression of Costimulatory Molecules
Surface expressed HMGB-1 was analyzed by flow cytometry (FACSCalibur Flow Cytometry System, BD BioSciences Pharmingen) using the anti-HMGB-1 antibody and secondary Alexa488-conjugated antibody (as described below). Costimulatory molecule cell surface expression was performed by incubating cells at C (protected from light) for 30 minutes with the following fluorescently-conjugated antibodies: APC antihuman HLA-DR (LN3), PE-Cy5 anti-human CD86 (B7-2) (eBioscience, Inc), FITC anti-CD40 (5C3), PE-Cy5 anti-CD80 (B7-1), PE-Cy5 anti-CD28 (CD28.2), and APC anti-CD25 (M-A251) (BD Biosciences, PharMingen). Cells were subsequently washed, resuspended in buffer containing 2 mM EDTA (to facilitate detachment of adherent cells), and transferred to FACS to analyze by flow cytometry (a minimum of 10 000 events were collected).
2.5. Fluorescent Microscopy Analysis
Surface expression of HMGB-1 on PBMC by fluorescent microscopy has been previously described in detail . In brief, PBMCs were cultured (C, 5% C) directly on sterile cover slips to allow attachment of adherent cells overnight before stimulation with 1 nM of TSST-1. For HMGB-1 expression, cells were incubated with rabbit anti-human HMGB-1 IgG as previously described , diluted in blocking buffer (PBS, 3% FBS), followed by a secondary Alexa488-conjugated goat antirabbit IgG antibody. Cells were subsequently fixed using Cytofix buffer (Pharmingen). Fluorescently labelled PBMCs were then stained with Hoechst 3342 nuclear dye (Molecular Probes) according to manufacturer's directions, and mounted on slides using Prolong Anti-Fade reagent (Molecular Probes). Cells were visualized with an AxioPlan II fluorescence microscope equipped with a CCD camera using Northern Eclipse software (Epix) for acquisition of images. Images were taken with the 63 x oil immersion objective lens, and Adobe Photoshop 6.0 software was used for image layout.
2.6. Western Blot Analysis of Secreted HMGB-1
PBMC culture supernatants were concentrated (~10-fold) from the original volume of 1.5 ml using Amicon Ultra centrifugal filters with a molecular weight cutoff of 10 kDa (Millipore). The supernatants then had been further prepared using the SDS-PAGE Clean-up kit (Amersham) according to the manufacturer’s directions prior to running on a 12% polyacrylamide gel. Western blotting was performed by semidry transfer of proteins (Trans-Blot SD Semi-Dry Electrophoretic Transfer Cell, BioRad) onto an Immobilon-P PVDF membrane (Millipore) which was blocked for 1 hour at room temperature with 1% BSA, 0.5% Tween in TBS prior to overnight incubation (at C) with rabbit polyclonal anti-HMGB-1 antibody. The membrane was subsequently incubated with anti-rabbit IgG horse-radish-peroxidase-(HRP-) conjugated secondary antibody for 1 hour at room temperature on a shaker. HMGB-1 detection was performed using Super Signal substrate (Pierce) and developed as well as analyzed using the Alpha Innotech 3400 Gel Documentation system (Alpha Innotech).
2.7. Statistical Analysis
Statistical analysis was performed using Prism 4.0 software package (GraphPad Software, Inc., San Diego, CA). Student -tests (one-tail) were used to assess the significance of differences in HMGB-1 and co-stimulatory molecule expression between IPP treated and untreated PBMC at different times post-TSST-1 stimulation. The effects of IPP over time on co-stimulatory molecule expression by APC (CD40, CD80, CD86, HLA-DR) and αβ T cells (CD25, CD28) were further examined by 2-way ANOVA. Differences were considered significant if the probability of the null hypothesis was less than five percent (). Each experiment represents 3 to 4 healthy subjects unless otherwise noted.
3.1. IPP-Primed γδ T Cells Induce an Early Upregulation of CD40 following TSST-1 Stimulation
Following overnight treatment with IPP, CD40 expression was upregulated in comparison to those that were untreated (IPP + TSST-1 versus TSST-1 alone; , Student’s -test) (Figure 2(a)). The elevated CD40 expression was observed up to 6 hours postsuperantigen stimulation, after which time CD40 was downregulated or internalized. We previously demonstrated that CD40L (CD154) is expressed on T cells within 3 hours following exposure to TSST-1 , therefore, the down-regulation of CD40 beyond 6 hours is likely a consequence of CD40 binding to CD40L on TSST-1-activated T cells. We verified that up-regulation of CD40 expression in populations exposed to IPP was solely attributed to the presence of activated γδ T cells, since removal of γδ T cells completely abrogated the effect of IPP (Figure 2(b)). The effect of IPP-activated γδ T cells over time on CD40 expression following TSST-1 stimulation was further verified using 2-way ANOVA (IPP x time interaction, ). In contrast to CD40, the expression of CD86 was down-regulated early in IPP treated PBMC at 3 hours following TSST-1 stimulation (IPP + TSST-1 versus TSST-1 alone; , Student’s -test) (Figure 2(a)). Again, this effect was abrogated following depletion of γδ T cells (Figure 2(b)). Two-way ANOVA confirmed an interaction effect (IPP x time interaction, ). There was a similar trend for decreased expression of HLA-DR (the MHC class II molecule to which TSST-1 binds on APC) and CD80 by IPP treatment, but the differences were not statistically significant.
3.2. TSST-1, but Not IPP-Primed γδ T Cells, Activate αβ T Cells
In contrast to the direct affect of IPP on monocyte function, there was little notable direct influence on the activation state of αβ T cells as evaluated by the expression of CD25 or CD28, which remained largely unchanged in response to IPP pretreatment (Figure 3). The upregulation of CD25 on αβ T cells at 24 hours was solely dependent on TSST-1 stimulation regardless of IPP, as shown by the comparison of IPP + TSST-1 versus IPP alone (, Student’s -test, Figure 3). Two-way ANOVA confirmed this effect (TSST-1 effect, ; TSST-1 x time interaction, ).
3.3. IPP-Primed γδ T Cell Potentiates the Release of Cell Surface Expression of HMGB-1 (Amphoterin) into the Extracellular Milieu following TSST-1 Stimulation
Rouhiainen et al. established that monocytes that had become adherent export HMGB-1 to the cell surface where it serves a function for process extension, migration, and cell-cell interaction . Extracellular cell-surface expressed HMGB-1 has been called amphoterin to differentiate it from intracellular HMGB-1 found in the nucleus . Given the direct influence of γδ T cells on the activation, maturation, and regulation of cells of monocytic lineage [20, 21], we wanted to determine how IPP stimulation would influence the surface manifestation of HMGB-1 on cultured monocytes present in PBMC. Figure 4(a) shows that resting adherent cells have HMGB-1 (stained in green) localized at focal points around the perimeter in vesicle-like pockets (top left corner; RPMI). T cells, which are nonadherent cells in suspension (stained in red), do not express HMGB-1 on the surface in this manner. Adherent monocytes bearing surface expressed HMGB-1 subsequently released it following TSST-1 stimulation (Figure 4(a); top right panel). Overnight treatment with IPP alone also led to a change in extracellular HMGB-1 expression in PBMC cultures (Figure 4(a); bottom left panel). There was an observable modification on both the morphological appearance of macrophages as well as the distribution of HMGB-1 around the perimeter, which became less concentrated in vesicle-like foci and more dispersed. Overnight incubation of PBMCs with IPP followed by TSST-1 stimulation resulted in significantly more HMGB-1 being released into the extracellular environment compared to TSST-1 alone (Figure 4(a), upper and lower right panel). This change in surface expressed HMGB-1 was assessed by flow cytometry, which enabled us to both confirm and quantify the release of HMGB-1 from differentiated monocytes following TSST-1 stimulation. Figure 4(b) displays the difference between the various treatment conditions on the loss of cell-surface expressed HMGB-1 assessed by flow cytometry. IPP-pretreated PBMCs that were subsequently stimulated with TSST-1 released more HMGB-1 from the cell surface (i.e., less HMGB-1 expression on the cell surface) than those cells that were left untreated with IPP prior to superantigen stimulation (IPP + TSST-1 versus TSST-1 alone, , paired Student’s -test). The actual secretion of HMGB-1 into the extracellular milieu from TSST-1 stimulated PBMC was further verified by Western blot of cell culture supernatants (Figure 4(c)), which again substantiated that IPP pretreatment followed by TSST-1 stimulation led to its greater release than PBMC stimulated with TSST-1 without IPP-activation of γδ T cells (IPP + TSST-1 versus TSST-1 alone, , paired Student’s -test).
Overnight treatment with IPP resulted in a notable up-regulation of CD40 on monocytes in the presence of γδ T cells. We previously demonstrated that impeding the CD40-CD40L interaction with CD40 monoclonal antibodies (but not the CD86 or CD80 interaction) completely blocks TSST-1-induced inflammation . The early up-regulation of CD40 on monocytes by IPP-primed γδ T cells in the current study provides a basis for the prior observation that TNFα and IFNγ levels increased 3-to 4-fold during the early phase of the immune response to TSST-1 in PBMC containing activated γδ T cells . This early augmentation was also abrogated after depletion of γδ T cells . This study also demonstrates that the exaggerated response to TSST-1 by activated γδ T cells is through the direct modulation of the responsiveness of monocytes and not αβ T cells since we found that the upregulation of CD25 on αβ T cells was affected only by stimulation with TSST-1 and not IPP. The regulation of CD40 expression by activated γδ T cells appears to parallel the mechanism of linking innate to adaptive immunity by glycolipid responsive Vα14 + NK T cells stimulated with α-galactosylceramide. It was found that the rapid release of TNFα and IFNγ to ovalalbumin, acquisition of CD4+ and CD8+ T cell immunity, and maturation of dendritic cells were all dependent on the CD40-CD40L interaction induced by the priming of Vα14+ NK T cells by α-galactosylceramide . In contrast to CD40, CD86 expression was found to be reduced in PBMC treated with IPP overnight. This monocytic phenotype may be reflective of a state described as “immature dendritic cells” in which cycling of the HLA-DR molecule is rapid and levels of CD86 are relatively low . Taken together, these studies suggest that innate T lymphocytes responsive to specific “alarmins” influence the ability of APC to effectively stimulate cells of adaptive immunity, and the CD40-CD40L interaction likely plays a pivotal role in this process. This scenario is in agreement with recent demonstrations that γδ T cells induce early dendritic cell maturation and share an intimate relationship with APC [21, 24, 25]. Eberl et al.  further provided evidence that human γδ T cells are activated by microbial mevalonate metabolites and interact with monocytes and local macrophages to drive the acute inflammation in bacterial infections. Thus, γδ T cells provide a direct link between innate and adaptive immunity. It should be noted, however, that these studies primarily used either expanded γδ T cell lines or a large number of purified γδ T cells in coculture conditions. The conditions used in this study may be more reflective of the physiological state in which a small number of γδ T cells present in peripheral blood would be able to immediately respond to their stress-associated antigens, such as IPP. This early event would preclude the possibility of any expansion of γδ T cells, but it would lead to the efficient priming of APC.
This study also provides the first demonstration that IPP-primed human peripheral blood γδ T cells influence the secretion of HMGB-1 by macrophages. This finding is similar to the work by Semino et al.  who demonstrated that NK cells reciprocally activate autologous dendritic cells, and this interaction was also mediated through the secretion of HMGB-1. It is feasible that the enhanced HMGB-1 secretion observed in cells containing activated γδ T cells could be in response to an increase in apoptosis  due to the fact that IPP-stimulated γδ T cells are particularly susceptible to activation-induced cell death [29, 30] as a self-limiting precaution. During apoptosis, HMGB-1 is normally tightly bound to nucleosomes  as opposed to necrosis where HMGB-1 is released from cells . However, work by Urbonaviciute et al.  showed that biologically active HMGB-1 may also be released from apoptotic cells. One of the main ligands for extracellular HMGB-1 is the receptor for advanced glycation end (RAGE) products, a member of the Ig superfamily. The expression of RAGE increases following activation on both dendritic cells and antigen stimulated T cells . The release of HMGB-1 and its subsequent binding to RAGE is required for the clonal expansion, survival, and functional polarization of naive T cells .
Both dendritic cell maturation and Th1 polarization are events that have been attributed to the activity of γδ T cells and HMGB-1, respectively [21, 34–36]. Our findings connect these two previously unrelated concepts and brings forth the suggestion that γδ T cells mediate this effect and link innate and adaptive immunity by influencing the early upregulation of CD40 expression and release of HMGB-1 from APC, thereby priming the immune response to subsequent stimuli.
This study was supported in part by a Grant from the Canadian Institutes of Health Research to A.W.Chow (MT-7630), and by the Michael Smith Foundation for Health Research to S.Kalyan (MSFHR Doctoral Studentship).
- L. Wang, H. Das, A. Kamath, L. Li, and J. F. Bukowski, “Human V2V2 T cells augment migration-inhibitory factor secretion and counteract the inhibitory effect of glucocorticoids on IL-1 and TNF- production,” The Journal of Immunology, vol. 168, no. 10, pp. 4889–4896, 2002.
- M. Lahn, A. Kanehiro, K. Takeda et al., “ T cells as regulators of airway hyperresponsiveness,” International Archives of Allergy and Immunology, vol. 125, no. 3, pp. 203–210, 2001.
- S. Kalyan and A. W. Chow, “Human peripheral T cells potentiate the early proinflammatory cytokine response to staphylococcal toxic shock syndrome toxin-1,” Journal of Infectious Diseases, vol. 189, no. 10, pp. 1892–1896, 2004.
- S. R. Carding and P. J. Egan, “The importance of T cells in the resolution of pathogen-induced inflammatory immune responses,” Immunological Reviews, vol. 173, pp. 98–108, 2000.
- P. J. Egan and S. R. Carding, “Downmodulation of the inflammatory response to bacterial infection by T cells cytotoxic for activated macrophages,” Journal of Experimental Medicine, vol. 191, no. 12, pp. 2145–2158, 2000.
- J. Jameson, K. Ugarte, N. Chen et al., “A role for skin T cells in wound repair,” Science, vol. 296, no. 5568, pp. 747–749, 2002.
- P. Constant, F. Davodeau, M.-A. Peyrat et al., “Stimulation of human T cells by nonpeptidic mycobacterial ligands,” Science, vol. 264, no. 5156, pp. 267–270, 1994.
- J. F. Bukowski, C. T. Morita, Y. Tanaka, B. R. Bloom, M. B. Brenner, and H. Band, “V2V2 TCR-dependent recognition of non-peptide antigens and Daudi cells analyzed by TCR gene transfer,” The Journal of Immunology, vol. 154, no. 3, pp. 998–1006, 1995.
- C. T. Morita, E. M. Beckman, J. F. Bukowski et al., “Direct presentation of nonpeptide prenyl pyrophosphate antigens to human T cells,” Immunity, vol. 3, no. 4, pp. 495–507, 1995.
- C. T. Morita, H. K. Lee, D. S. Leslie, Y. Tanaka, J. F. Bukowski, and E. Märker-Hermann, “Recognition of nonpeptide prenyl pyrophosphate antigens by human T cells,” Microbes and Infection, vol. 1, no. 3, pp. 175–186, 1999.
- M. Kistowska, E. Rossy, S. Sansano et al., “Dysregulation of the host mevalonate pathway during early bacterial infection activates human TCR cells,” European Journal of Immunology, vol. 38, no. 8, pp. 2200–2209, 2008.
- T. Krakauer, “Immune response to staphylococcal superantigens,” Immunologic Research, vol. 20, no. 2, pp. 163–173, 1999.
- T. Ferry, D. Thomas, T. Perpoint et al., “Analysis of superantigenic toxin V T-cell signatures produced during cases of staphylococcal toxic shock syndrome and septic shock,” Clinical Microbiology and Infection, vol. 14, no. 6, pp. 546–554, 2008.
- S. Kalyan and A. W. Chow, “Staphylococcal toxic shock syndrome toxin-1 induces the translocation and secretion of high mobility group-1 protein from both activated T cells and monocytes,” Mediators of Inflammation, vol. 2008, Article ID 512196, 7 pages, 2008.
- H. Wang, O. Bloom, M. Zhang et al., “HMG-1 as a late mediator of endotoxin lethality in mice,” Science, vol. 285, no. 5425, pp. 248–251, 1999.
- U. Andersson, H. Wang, K. Palmblad et al., “High mobility group 1 protein (HMG-1) stimulates proinflammatory cytokine synthesis in human monocytes,” Journal of Experimental Medicine, vol. 192, no. 4, pp. 565–570, 2000.
- W. W. S. Kum, K. B. Laupland, R. H. See, and A.W. Chow, “Improved purification and biologic activities of staphylococcal toxic shock syndrome toxin 1,” Journal of Clinical Microbiology, vol. 31, no. 10, pp. 2654–2660, 1993.
- W. W. S. Kum, R. W. Y. Hung, S. B. Cameron, and A. W. Chow, “Temporal sequence and functional implications of V-specific T cell receptor down-regulation and costimulatory molecule expression following in vitro stimulation with the staphylococcal superantigen toxic shock syndrome toxin-1,” Journal of Infectious Diseases, vol. 185, no. 4, pp. 555–560, 2002.
- A. Rouhiainen, J. Kuja-Panula, E. Wilkman et al., “Regulation of monocyte migration by amphoterin (HMGB1),” Blood, vol. 104, no. 4, pp. 1174–1182, 2004.
- J. E. Dalton, J. Pearson, P. Scott, and S. R. Carding, “The interaction of T cells with activated macrophages is a property of the V1 subset,” The Journal of Immunology, vol. 171, no. 12, pp. 6488–6494, 2003.
- J. Ismaili, V. Olislagers, R. Poupot, J.-J. Fournié, and M. Goldman, “Human T cells induce dendritic cell maturation,” Clinical Immunology, vol. 103, no. 3, pp. 296–302, 2002.
- S.-I. Fujii, K. Liu, C. Smith, A. J. Bonito, and R. M. Steinman, “The linkage of innate to adaptive immunity via maturing dendritic cells in vivo requires CD40 ligation in addition to antigen presentation and CD80/86 costimulation,” Journal of Experimental Medicine, vol. 199, no. 12, pp. 1607–1618, 2004.
- J. K. H. Tan and H. C. O'Neill, “Maturation requirements for dendritic cells in T cell stimulation leading to tolerance versus immunity,” Journal of Leukocyte Biology, vol. 78, no. 2, pp. 319–324, 2005.
- F. Dieli, N. Caccamo, S. Meraviglia et al., “Reciprocal stimulation of T cells and dendritic cells during the anti-mycobacterial immune response,” European Journal of Immunology, vol. 34, no. 11, pp. 3227–3235, 2004.
- L. Conti, R. Casetti, M. Cardone et al., “Reciprocal activating interaction between dendritic cells and pamidronate-stimulated T cells: role of CD86 and inflammatory cytokines,” The Journal of Immunology, vol. 174, no. 1, pp. 252–260, 2005.
- M. Eberl, G. W. Roberts, S. Meuter, J. D. Williams, N. Topley, and B. Moser, “A rapid crosstalk of human T cells and monocytes drives the acute inflammation in bacterial infections,” PLoS Pathogens, vol. 5, no. 2, Article ID e1000308, 2009.
- C. Semino, J. Ceccarelli, L. V. Lotti, M. R. Torrisi, G. Angelini, and A. Rubartelli, “The maturation potential of NK cell clones toward autologous dendritic cells correlates with HMGB1 secretion,” Journal of Leukocyte Biology, vol. 81, no. 1, pp. 92–99, 2007.
- V. Urbonaviciute, B. G. Furnrohr, S. Meister et al., “Induction of inflammatory and immune responses by HMGB1-nucleosome complexes: implications for the pathogenesis of SLE,” Journal of Experimental Medicine, vol. 205, no. 13, pp. 3007–3018, 2008.
- P. Rovere, E. Clementi, M. Ferrarini et al., “CD95 engagement releases calcium from intracellular stores of long term activated, apoptosis-prone T cells,” The Journal of Immunology, vol. 156, no. 12, pp. 4631–4637, 1996.
- M. Ferrarini, S. Heltai, E. Toninelli, M. G. Sabbadini, C. Pellicciari, and A. A. Manfredi, “Daudi lymphoma killing triggers the programmed death of cytotoxic V9/V2 T lymphocytes,” The Journal of Immunology, vol. 154, no. 8, pp. 3704–3712, 1995.
- P. Rovere-Querini, A. Capobianco, P. Scaffidi et al., “HMGB1 is an endogenous immune adjuvant released by necrotic cells,” EMBO Reports, vol. 5, no. 8, pp. 825–830, 2004.
- B. Moser, D. D. Desai, M. P. Downie et al., “Receptor for advanced glycation end products expression on T cells contributes to antigen-specific cellular expansion in vivo,” The Journal of Immunology, vol. 179, no. 12, pp. 8051–8058, 2007.
- I. E. Dumitriu, P. Baruah, B. Valentinis et al., “Release of high mobility group box 1 by dendritic cells controls T cell activation via the receptor for advanced glycation end products,” The Journal of Immunology, vol. 174, no. 12, pp. 7506–7515, 2005.
- D. Messmer, H. Yang, G. Telusma et al., “High mobility group box protein 1: an endogenous signal for dendritic cell maturation and Th1 polarization,” The Journal of Immunology, vol. 173, no. 1, pp. 307–313, 2004.
- M.-C. Devilder, S. Maillet, I. Bouyge-Moreau, E. Bonnadieu, M. Bonneville, and E. Scotet, “Potentiation of antigen-stimulated V9V2 T cell cytokine production by immature dendritic cells (DC) and reciprocal effect on DC maturation,” The Journal of Immunology, vol. 176, no. 3, pp. 1386–1393, 2006.
- D. S. Leslie, M. S. Vincent, F. M. Spada et al., “CD1-mediated / T cell maturation of dendritic cells,” Journal of Experimental Medicine, vol. 196, no. 12, pp. 1575–1584, 2002.
Copyright © 2009 Shirin Kalyan and Anthony W. Chow. 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.