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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Biol Blood Marrow Transplant. Author manuscript; available in PMC 2009 June 22.
Published in final edited form as:
PMCID: PMC2699940

Host derived interleukin-18 differentially impacts regulatory and conventional T cell expansion during acute graft-versus-host disease


Interleukin (IL)-18 stimulates T helper 1 (Th1) and Th2-mediated immune responses and has been shown to modulate acute graft-versus-host disease (aGvHD). It is still unknown whether increased IL-18 levels during aGvHD are of host or donor origin and how the absence of IL-18 impacts migration and expansion of conventional CD4+CD25 (Tconv) and CD4+CD25+ regulatory (Treg) T cells in vivo. By utilizing IL-18 gene deficient donor versus recipient animals we found that the major cytokine production during the early phase of aGVHD induction was recipient derived, while donor hematopoietic cells contributed significantly less. By generating IL-18−/− luciferase transgenic mice we were able to investigate the impact of IL-18 on Tconv and Treg expansion and trafficking with in vivo bioluminescence imaging. While migration to secondary lymphoid organs was not significantly impacted by the absence of host IL-18, Tconv but not Treg expansion increased significantly. Absence of host IL-18 production translated into lower IFN-γ levels in the early phase after transplantation. We conclude that host derived IL-18 is a major factor for IFN-γ production that may have a protective effect on CD4+ mediated aGvHD, but is non-essential for Treg expansion in an allogeneic environment.

Keywords: Acute graft-versus-host disease, regulatory T cells, Interleukin-18


The production of proinflammatory cytokines, such as IL-1, IL-2, IL-12, IL-18, TNF and IFN-γ, is a key feature of acute graft-versus-host disease (aGvHD) and the balance between T helper 1 (Th1) and Th2 cytokine production determines end organ damage [1]. While TNF was demonstrated to affect regulatory T cell (Treg) function [2], the impact of IL-18, which is increased in human and murine aGvHD [3, 4], on Treg is not yet defined. IL-18R engagement leads to MyD88 signaling followed by activation of TNF-receptor-associated factor and NFκB [5] which enhances the production of IFN-γ [6, 7]. Interestingly, IFN-γ and other Th1 cytokines have been shown to be involved in mechanisms that are protective against aGvHD [812].

Cell types that are relevant in GvHD with reported ability to produce IL-18 include macrophages, Kupffer cells, dendritic cells, T-cells, intestinal epithelial cells and keratinocytes [4, 1315]. Itoi and colleges have shown that IL-18 levels were only slightly elevated when Caspase-1-deficient recipients were engrafted with wildtype H-2 disparate splenocytes [4]. Although this indicates that IL-18 secretion during GvHD is dependant on host caspase-1, there is currently no information on the relative contribution of host versus donor to IL-18 cytokine levels and whether host or donor IL-18 is critical for GvHD induction and promotion. Increased levels of serum IL-18 and IL-18(R)α receptor expression on T lymphocytes were found in patients that developed GvHD after aHCT [3, 16]. In murine studies IL-18 was demonstrated to have a differential impact on CD4 as compared to CD8 mediated GvHD [17], to be critical for Fas mediated donor T-cell apoptosis [18] and to reduce GvHD severity when administered to the donor prior to transplantation [19]. Another study confirmed that IL-18 neutralization increased T cell expansion but did not influence GVHD severity, which may be explained by the use of a different model with non-irradiated recipients and the difference in IL-18 neutralization by a soluble IL-18 binding protein [20]. CD4+CD25+ regulatory T cells (Treg) have been demonstrated to play a major role in modulating GvHD [21, 22]. The relevance of IL-18 for this cell population has so far only been investigated in a model of oral tolerance induction, a study that indicated that IL-18 is essential for the induction of antigen-specific regulatory T cells, that were defined by CD25 expression and the production of TGF-β [23].

In the present study we investigate the kinetics of IL-18Rα expression on Treg and Tconv as well as the origin and the relevance of IL-18 in the early phase after transplantation for Treg and Tconv expansion by utilizing cytokine deficient donor or recipient animals.



C57B/6 (H-2kb), IL-18−/− (H-2kb), FVB/N (H-2kq), and Balb/c (H-2kd) mice were purchased from Jackson Laboratory (Bar Harbor, ME) or Charles River Laboratory (Wilmington, MA). Mice were used between 6 and 12 weeks of age. Only male to male or female to female combinations were used for transplant experiments. The luciferase-expressing (luc+) transgenic FVB/N line was generated as previously described [24]. luc+ offspring of the transgenic founder line FVB-L2G85 were backcrossed onto the C57B/6 background (F8) and then crossed with IL-18−/− animals, both on C57B/6 background. All animal protocols were approved by the University Committee on Use and Care of Laboratory Animals at Stanford University.

Generation of luciferase-(luc+) transgenic IL-18−/− mice

In order to track Treg and Tconv in the absence of IL-18 production by donor derived hematopoetic cells, we generated luciferase transgenic IL-18−/− animals. The luciferase-expressing (luc+) transgenic line [24] was backcrossed onto the C57B/6 background (F8) and then crossed with IL-18−/− animals (C57B/6). IL-18 gene deficiency was verified by RT-PCR (Fig. 4A) and luciferase expression was monitored by bioluminescence imaging (Fig. 4B). The employed luc+/IL-18−/− mice were bred for more than 10 generations on the C57B/6 background.

Figure 4
Generation of IL-18−/− luciferase transgenic C56Bl/6 mice

Flow cytometric cell purification and analysis

The following antibodies were used for flow cytometric analysis: unconjugated anti-CD16/32 (2.4G2), CD4 (RM4-5), CD8α (53-6.7), CD25 (PC61), CD11c (M1/70), CD45R/B220 (RA3-6B2), H-2Kq (KH114), H-2Kd (34-2-12) from BD Pharmingen (San Diego, CA) and eBiosciences (San Diego, CA). Foxp3 staining was performed using the intracellular Foxp3 staining kit (Ab: FJK-16s) as described in the manufacturers instructions (eBioscience, San Diego, CA). Goat anti-murine IL-18Rα(R&D Systems) staining was followed by SP-biotinylated mouse anti–goat IgG (H plus L) diluted in PBS (Jackson ImmunoResearch Laboratories) for 20 min. Cells were subsequently washed twice in PBS and then stained with streptavidin-APC (BD PharMingen). Staining was performed in the presence of purified anti-CD16/32 at saturation to block unspecific staining. Propidium iodide (Sigma, St Louis, MO) was added prior to analysis to exclude dead cells. All analytical flow cytometry was done on a modified dual laser LSRScan (BD Immunocytometry Systems, San Diego, CA) in the Shared FACS Facility, Center for Molecular and Genetic Medicine at Stanford using FlowJo software (TreeStar, Ashland, OR) for data analysis.

Cell isolation and sorting

Single cell-suspensions from cervical lymph nodes (cLN), axillary lymph nodes (aLN), inguinal lymph nodes (iLN), mesenteric lymph nodes (mLN) and spleens were enriched for CD25+ cells after sequential staining with anti-CD25 PE (BD PharMingen) and anti-PE magnetic beads using the autoMACS system (POSSEL program, Miltenyi Biotec, Auburn, CA). CD25+ cells were then stained with anti-CD4 APC and sorted on a MoFlow cell sorter (Becton Dickinson, Mountain View, CA) for the CD25high population (15–20% of the enriched CD25+ cells) or for CD4+CD25 cells. The CD4+CD25+ population was routinely greater than 95% Foxp3+. T-cell–depleted bone marrow (TCD BM) was obtained through negative depletion using anti-CD4 and anti-CD8 magnetic beads (Miltenyi Biotech). For isolation of lymphocytes from the liver, the portal vein was perfused with PBS, the organ was removed and homogenized and the lymphocytes were separated by Ficoll gradient centrifugation.

Real time quantitative PCR for Foxp3

Total RNA was isolated from fresh cell pellets using the RNeasy MiniKit (Qiagen, Valencia, CA) and genomic DNA was eliminated by digestion with a modified proprietary Dnase (DNA-free; Ambion, Austin, TX). 500ng total RNA was mixed with dT16 primer in a volume of 11 μl, incubated at 65° C for 10 min and immediately placed on ice. Following addition of 100 units Superscript II reverse transcriptase (GIBCO, Carlsbad, CA) reverse transcription was performed for 2 h at 42° C in 1x RT reaction buffer (GIBCO, Carlsbad CA), 10 μM DTT, 500 μM dNTP (Amersham Biosciences, Pittsburgh, PA) with 2.5 μM dT16 primer in a volume of 20μl PCR reactions were performed in a final volume of 20μl with cDNA prepared from 20ng RNA and a final concentration of 1x SYBR®Green PCR Master Mix (ABI, Foster City, CA, USA) and 200nM of each primer (sequences: FoxP3 forward, GGAGCCGCAAGCTAAAAGC; FoxP3 reverse, TGCCTTCGTGCCCACTG; GAPDH forward, GTCCTGAAGTATGTCGTGGAGTCTAC; and GAPDH reverse, GGCCCCGGCCTTCTC). The reaction was run in an ABI 7700 Sequence Detection System with the following cycling conditions: 50° C for 2 min, 94°C for 10min, then 40 cycles of 94° C for 15 sec and 60° C for 60 sec. For each gene a standard curve was prepared and triplicate measurements were performed for each sample.

GVHD model

Acute GVHD was induced as described previously [25]. Briefly, recipients were given 5 × 106 TCD-BM cells after lethal irradiation with 800 cGy. To induce aGvHD the following numbers of CD4+ T cells were given: 8 × 105 (C57B/6→Balb/c), 2 × 106 (FVB/N→C57Bl/6), 2 × 106 (Balb/c→C57B/6). For Treg trafficking studies in the FVB/N→C57Bl/6 model, 5 × 105 CD4+CD25high luc+ Treg were injected on d0. Transplanted mice were housed in autoclaved cages and kept on antibiotic water (Sulfomethoxazole Trimethoprim, Schein Pharmaceutical, Corona, CA).

In vivo Bioluminescence imaging (BLI)

In vivo bioluminescence imaging (BLI) was performed as previously described [26]. Briefly, mice were injected intraperitoneally with luciferin (10 μg/g bodyweight). Ten minutes later mice were imaged using an IVIS200 charge-coupled device (CCD) imaging system (Xenogen, Alameda, CA) for 5 minutes. Imaging data were analyzed and quantified with Living Image Software (Xenogen) and IgorProCarbon (WaveMetrics, Lake Oswego, OR).


Tissues were fixed with 10% formalin, embedded in paraffin and sections of 5 μm thickness were mounted on positively charged precleaned microscope slides (Superfrost/Plus; Fisher Scientific, Hampton, NH). Hematoxylin/eosin (H/E) staining of paraffin-embedded tissue sections was performed according to standard protocols. Tissues from small bowel, large bowel and liver were evaluated by an experienced pathologist (N.K.) according to a previously published histopathology scoring system [27]. Evaluation of the stained tissue sections was performed on a Nikon microscope (Eclipse, TE 300; Melville, NY). Standard magnifications were 200x/numerical aperture 0.45 and 400x/numerical aperture 0.60. Microscopic photos were obtained using a Spot digital camera (Diagnostic Instruments, Sterling Heights, MI).

In vitro Treg/Tconc activation culture

Treg or Tconv cells (C57Bl/6) were incubated with irradiated (30Gy) CD11c+ cells derived from Balb/c mice. Each cell type in a concentration of 2×105 per flat bottom well. After 48 hours cells were collected, washed and analyzed by FACS for IL-18Rα surface expression in combination with CD4 and intracellular Foxp3 staining.

ELISA for IL-18 and IFN-γ

Serum was collected from Balb/c recipients on days 1, 2, 3, 5 and 8 after transplantation. ELISA Assays were performed according to the manufacturer’s instructions (R&D systems Minneapolis, MN). Briefly, samples were diluted 1:2 to 1:5, and the cytokine was captured by the specific primary mAb pre-coated on the microplate and detected by horseradish peroxidase labeled secondary mAbs. Plates were read at 450 nm using a microplate reader (model Spectra Max 190; Bio-Rad Labs, CA). Recombinant murine cytokines (BD PharMingen) were used as standards. Samples and standards were run in duplicate, and the sensitivity of the assays was 16 to 20 pg/mL for each cytokine, depending on the sample dilution.

Statistical analysis

Differences in animal survival (Kaplan-Meier survival curves) were analyzed by log-rank test. Differences in mean fluorescence intensity (MFI), lymphocyte counts, Foxp3 RNA expression, thymidine incorporation, proliferation of luc transgenic T-cells and serum cytokine levels were analyzed using the two tailed Student’s t test. Error bars indicate the standard deviation from the geometric mean. A p-value <0.05 was considered statistically significant.


CD4 mediated aGvHD severity is enhanced in IL-18 deficient hosts

To investigate the impact of IL-18 deficiency of the host on aGvHD severity in our model, CD4 Tconv (H-2kq) were transplanted into lethally irradiated C57Bl/6 recipients that were either wt or IL-18 deficient. Interestingly, IL-18 deficiency of the host led to increased aGvHD severity as assessed by weight loss (Fig. 1A) and more severe histopathological GvHD damage of the colon with multiple crypt abscesses when the host was IL-18 deficient (Fig. 1B). Histopathology scoring from small bowel, large bowel and liver tissue samples harvested on day 10 after BMT from 5 animals per group, demonstrated the highest GvHD severity (*p<0.05) in IL-18 deficient recipients (Fig. 1B). This translated into a more aggressive course of GvHD in the wt→IL-18−/− combination as compared to the wt→wt combination (Fig. 1C).

Figure 1
IL-18 deficiency of the recipient enhances graft-versus-host disease severity

IL-18Rα expression on Tconv and Treg cells is upregulated in the presence of alloantigen

Based on the observation that the absence of IL-18 led to a more severe course of aGvHD we aimed to study the relevance of IL-18 for Treg which have been shown to promote transplantation tolerance in models of aGvHD [21] and solid organ transplantation [28]. Therefore, in a first step IL-18Rα surface expression was evaluated on conventional CD4+ Tcells (Tconv) and Treg cells from mesenteric (mLN), cervical (cLN), axillary (aLN) and mesenteric (mLN) lymph nodes, spleen, liver and thymus as shown for the respective experiments. Gating on CD4+Foxp3+ versus CD4+Foxp3 demonstrated comparable expression of IL-18Rα on Treg and Tconv cells (Fig 2A). Data are presented as the difference (Δ) between the mean fluorescence intensity (MFI) of the positive stain (anti–IL-18Rα) and the MFI of the negative control (goat Ig alone). Interestingly IL-18Rα surface expression differed with respect to the origin of the cell population being the highest in the lymph nodes (73 and 87) and lowest in liver derived T cells (37 and 39). Activation for 48h with allogeneic APCs led to an upregulation of the IL-18Rα on both Tconv and Treg (Fig 2B) suggesting that IL-18 signaling may be relevant during alloantigen driven T cell responses.

Figure 2
Expression of IL-18Rα on regulatory and conventional T cells

Intact Treg development and function in the absence of IL-18

To study the relevance of intact IL-18 production for the development of Treg we employed mice with a disrupted IL-18 gene which have been previously described [29]. Total lymphocyte counts in IL-18−/− and IL-18−/+ mice were comparable with wildtype animals (Fig. 3A). Foxp3 expression within the CD4+ cell population was comparable in IL-18 deficient as compared to wildtype animals as quantified by real-time PCR (Fig. 3B) and intracellular Foxp3 protein analysis by FACS (Fig. 3C). To further investigate if there was a functional difference, Treg from IL-18−/− and wildtype mice were compared with respect to their capability to suppress alloantigen driven T cell proliferation. Importantly, there were no significant differences with respect to suppressor function by Treg derived from IL-18−/−, IL-18−/+ or wildtype mice (Fig. 3D). These data indicate that Treg that have developed in the absence of IL-18 are functionally suppressive. Furthermore, these findings are in line with the observation that IL-18 deficient mice display a defect in NK cell function but no signs of autoimmunity [29].

Figure 3
CD4+Foxp3+ T cells develop normal and are functionally suppressive in the absence of IL-18

IL-18 production of the donor is non-essential for aGvHD development

To study the impact of donor IL-18 on the course of aGvHD we employed TCD-BM and luc+ CD4 T cells from IL-18 deficient donors. Transplantation of luc+ IL-18−/− donor CD4 T cells into wt animals (C57Bl/6→Balb/c) resulted in a comparable course of aGvHD with no survival difference (Fig. 5A). The expansion kinetics and homing pattern of luc+ IL-18−/− and wt donor CD4 T cells was comparable (Fig. 5B). Histopathological analysis confirmed the survival data, indicating an intact colon mucosa in the TCD-BM group, while crypt abscesses and mucosal denudation as signs of aGvHD tissue damage to the intestinal tract were found to a comparable extend in recipients of wt and IL-18 deficient donor T cells (Fig. 5C). Cumulative histopathology scoring from small bowel, large bowel and liver tissue derived from 3 animals per group, demonstrated comparable GvHD severity in IL-18 deficient as compared to wt donors (Fig. 5C). These data indicate that donor IL-18 production does not impact aGvHD severity.

Figure 5
IL-18 deficiency of the donor does not impact CD4 T cell expansion and graft-versus-host disease severity

Increased IL-18 levels during aGvHD are mainly host derived and absence of host IL-18 translates into lower IFN-γ production

The observation that the course of CD4 T cell induced aGvHD was independent of donor IL-18 production prompted us to measure the IL-18 serum levels in the situation where either the donor or the recipient was deficient for the cytokine. Serum was collected at the different time points and was significantly reduced when the recipient was IL-18 deficient (Fig. 6A). Interestingly, donor contribution to the IL-18 production in the early phase after transplantation (days 1–5) was minimal as evidenced by IL-18 levels that were comparable to the wt→wt situation (Fig. 6A). At later time points (day 8) there was also a slight decrease of the cytokine when the donor was IL-18 deficient (Fig. 6A). Since IL-18 can induce IFN-γ production in T cells and NK cells [30], we investigated the levels of this cytokine in parallel. Interestingly, IFN-γ levels were significantly reduced when the recipient but not when the donor was IL18 deficient (Fig. 6B).

Figure 6
Host but not donor derived IL-18 is the major contributor to elevated IL-18 serum levels during the early phase of acute graft-versus-host disease

Absence of host IL-18 predicts increased CD4 Tconv but not Treg expansion

Based on the observation that the host has the major contribution to the IL-18 production during aGvHD we next investigated the expansion patterns of Treg and Tconv in the absence of host IL-18 production. Therefore, we transferred luc+ Treg (H-2kq) into lethally irradiated C57Bl/6 recipients that were either wt or IL-18 deficient. Treg expansion was comparable in the presence or absence of host IL-18 production as shown for 3 representative animals at two time points after BMT (Fig. 7A) and as quantified in photons over total body area at serial time points (Fig. 7B). To further evaluate the relevance of increased IL-18 levels during aGvHD for Treg expansion, luc+ CD4 Tconv or Treg (H-2kq) were transplanted into lethally irradiated C57Bl/6 recipients that were either wt or IL-18 deficient. Bioluminescence imaging at serial time points after BMT disclosed an increased expansion of luc+ CD4 Tconv cells in the absence of recipient IL-18 (Fig. 7C, D).

Figure 7
IL-18 deficiency of the recipient increases expansion CD4 T cell but not Treg cells


Allogeneic BMT is a potentially curative therapeutic option for many malignant and non-malignant diseases. However, the beneficial effects of the donor immune system on engraftment and elimination of residual malignant cells are closely linked to the occurrence of aGvHD which leads to treatment related mortality. Treg have been shown to reduce the incidence and severity of aGvHD in rodent models [21, 22, 31] and increased Foxp3+ Treg cells in the hematopoietic graft were shown to predict a reduced risk for aGvHD in human transplant recipients [32]. Expansion and function of Treg relies on IL-2 [25, 3335] while the role of other IL-2Rγ-chain dependent cytokines such as IL-7 and IL-15 are still under investigation [36]. Insight into the cytokine milieu that can favor Treg function may help to manipulate the function of this cell population. In this report we evaluated the role of IL-18 on aGvHD and the differential impact on Tconv and Treg expansion. Interestingly we found that expression of the IL-18Rα was similar in Treg and Tconv isolated from different organs. Since in the in vitro studies IL-18 from the stimulators and irradiated non-Treg responders was present we did not address the functional role of IL-18 on Treg suppressor function but showed that Treg which developed in the absence of IL-18 are equally suppressive as their wt counterparts.

Our in vivo data indicate that ontogeny, function and homeostasis of Treg remain intact in the absence of IL-18 in healthy mice. In a model of oral tolerance induction, IL-18 deficient recipients did not develop Treg in Peyer’s patches after feeding with BLG [23]. The observation of Tsuji et al. that IL-18 was relevant for Treg mediated oral tolerance induction could be due to the requirement of the cytokine for Treg in the situation where an immune response requires regulation [23]. We therefore investigated the relevance of IL-18 for Treg and Tconv during aGvHD as an aberrant immune response. Our observation that donor deficiency for IL-18 did not affect CD4 T cell expansion and the course of aGvHD made us hypothesize that production of IL-18 by the host may be more relevant for the previously reported increased IL-18 levels after BMT [3, 4].

Indeed we found IL-18 levels to be significantly decreased when the recipient but not the donor animals were IL-18 deficient. This suggested that in the early phase after transplantation residual host hematopoietic cells such as macrophages, Kupffer cells and dendritic cells, that can survival the first week after the myeloablative irradiation, produce significant amounts of IL-18. Other recipient type cells with known ability to produce IL-18 are intestinal epithelial cells and keratinocytes [4, 1315]. These recipient cells may secrete IL-18 triggered by tissue damage due to the conditioning regimen. Interestingly, IL-18 in contrast to other cytokines is stored as biologically inactive precursor (pro-IL-18) and is secreted when appropriate cleaving enzymes are present [37, 38]. Previous studies have demonstrated the involvement of a caspase-1-like molecule and caspase-1 for cleavage of IL-18 [4, 39]. Lipopolysaccharide (LPS), that enhances aGvHD severity and leaks into the blood stream after conditioning induced bowel wall damage [40], has been shown to induce caspase-1 which is critical in the process of IL-18 secretion [41]. Our observation that increased IL-18 serum levels after BMT are host derived is compatible with the finding that caspase-1-deficient recipients engrafted with wildtype H-2 disparate splenocytes displayed decreased IL-18 production [4]. Our study is the first to delineate the relative contribution of the host on increased IL-18 cytokine levels during the early phase after BMT that has a functional impact on the aGvHD course. With respect to the clinical situation, the manipulation of GvHD through the cytokine Il-18 may be difficult to achieve based on its opposing effects on CD4 as compared to CD8 T cells [17] and due to the fact that human GvHD is not restricted to either subset as it can be studied in murine models with selective MHC class I or class II differences.

Since IL-18 has been demonstrated to induce IFN-γ production [7], a cytokine with known relevance for downmodulation of aGvHD in the early phase after BMT [8] and for long-term allograft survival [42] we studied the impact of host IL-18 deficiency on IFN-γ secretion. We found that reduced IL-18 production in IL-18 deficient recipients was paralleled by diminished IFN-γ serum levels. This finding may explain why the absence of host IL-18 resulted in more aggressive aGvHD, since IFN-γ was shown to induce death of activated donor CD4 cells [17]. IL-18 may mediate its effects not only directly by augmentation of IFN-γ production [43, 44] but also by increasing the expression of the IL-12R complex, thereby enhancing the effects of IL-12 [45]. Interestingly, IL-12 has been demonstrated to be critical for tolerance induction in solid organ transplantation [46] and to reduce aGvHD [12]. A recent in vivo study demonstrated a unique role for IFN-γ in the functional activity of alloantigen-reactive Treg cells during the development of operational tolerance to donor skin allografts [47]. In our studies the absence of host IL-18 was paralleled by reduced IFN-γ and we did not find any change in Treg proliferation under these conditions. Further studies are needed to address the role of reduced IFN-γ levels on Treg suppressor function in the BMT model.

Since the expansion kinetics of Treg were independent of host IL-18 the protective effect of host IL-18 on aGvHD was not through immunoregulation by increased Treg expansion. In contrast to data from the oral tolerance model [23], we did not find an essential role of IL-18 for the induction of Treg cells which may be due to model specific differences.

We conclude that Treg and Tconv express comparable levels of IL-18Rα which is upregulated in response to alloantigen. Absence of host but not donor IL-18 production translated into lower IFN-γ levels in the early phase after transplantation and resulted in a more rapid course of aGvHD. Host derived IL-18 has a protective effect in CD4+ mediated aGvHD, possibly through increased IFN-γ production. IL-18 is non-essential for Treg expansion in an allogeneic environment however downmodulates CD4+ Tconv expansion. In the absence of IL-18 increased CD4+ T cell proliferation results in more aggressive aGvHD.


The authors are grateful to Ruby M. Wong for expert assistance with statistical analysis and to the members of the Negrin laboratory for helpful discussion. This study was supported by grants from the National Institute of Health (NIH; RO1 CA0800065 and P01 HL075462 to R.S.N.), the Small Animal Imaging Resource Program (SAIRP grant number R24CA92862) and an In Vivo Cellular Molecular Imaging Center (ICMIC) grant (P50 CA114747). R.Z. is supported by the Dr. Mildred-Scheel-Stiftung, Germany.


Competing interests statement: The authors declare that they have no competing financial interests.

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