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Androgen signaling negatively controls group 2 innate lymphoid cells
research-article
Author(s):
Sophie Laffont
1 ,
Eve Blanquart
1 ,
Magali Savignac
1 ,
Claire Cénac
1 ,
Gilles Laverny
2 ,
Daniel Metzger
2 ,
Jean-Philippe Girard
3 ,
Gabrielle T. Belz
4
,
5 ,
Lucette Pelletier
1 ,
Cyril Seillet
4
,
5
,
,
Jean-Charles Guéry
1
,
Publication date (Print):
05 June 2017
Journal:
The Journal of Experimental Medicine
Publisher:
The Rockefeller University Press
There is no author summary for this article yet. Authors can add summaries to their articles on ScienceOpen to make them more accessible to a non-specialist audience.
Abstract
At the onset of adolescence, asthma becomes less prevalent in males than in females, suggesting a protective role of male sex hormones. Here, Laffont et al. show that androgens negatively control ILC2 development and ILC2-driven lung inflammation in male mice.
Abstract
Prevalence of asthma is higher in women than in men, but the mechanisms underlying this sex bias are unknown. Group 2 innate lymphoid cells (ILC2s) are key regulators of type 2 inflammatory responses. Here, we show that ILC2 development is greatly influenced by male sex hormones. Male mice have reduced numbers of ILC2 progenitors (ILC2Ps) and mature ILC2s in peripheral tissues compared with females. In consequence, males exhibit reduced susceptibility to allergic airway inflammation in response to environmental allergens and less severe IL-33–driven lung inflammation, correlating with an impaired expansion of lung ILC2s. Importantly, orchiectomy, but not ovariectomy, abolishes the sex differences in ILC2 development and restores IL-33–mediated lung inflammation. ILC2Ps express the androgen receptor (AR), and AR signaling inhibits their differentiation into mature ILC2s. Finally, we show that hematopoietic AR expression limits IL-33–driven lung inflammation through a cell-intrinsic inhibition of ILC2 expansion. Thus, androgens play a crucial protective role in type 2 airway inflammation by negatively regulating ILC2 homeostasis, thereby limiting their capacity to expand locally in response to IL-33.
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Most cited references23
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featureCounts: An efficient general-purpose program for assigning sequence reads to genomic features
Next-generation sequencing technologies generate millions of short sequence reads, which are usually aligned to a reference genome. In many applications, the key information required for downstream analysis is the number of reads mapping to each genomic feature, for example to each exon or each gene. The process of counting reads is called read summarization. Read summarization is required for a great variety of genomic analyses but has so far received relatively little attention in the literature. We present featureCounts, a read summarization program suitable for counting reads generated from either RNA or genomic DNA sequencing experiments. featureCounts implements highly efficient chromosome hashing and feature blocking techniques. It is considerably faster than existing methods (by an order of magnitude for gene-level summarization) and requires far less computer memory. It works with either single or paired-end reads and provides a wide range of options appropriate for different sequencing applications. featureCounts is available under GNU General Public License as part of the Subread (http://subread.sourceforge.net) or Rsubread (http://www.bioconductor.org) software packages.
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Innate lymphoid type 2 cells sustain visceral adipose tissue eosinophils and alternatively activated macrophages
Ari B. Molofsky, Jesse C. Nussbaum, Hong-Erh Liang … (2013)
Diverse immune cells participate in the regulation of visceral adipose tissue (VAT) and metabolic homeostasis. With obesity, pro-inflammatory macrophages, neutrophils, CD8+ T cells, CD4+ Th1 cells, and mast cells accumulate in VAT and contribute to local and systemic inflammation, ultimately promoting insulin resistance and the development of metabolic syndrome and type 2 diabetes; in contrast, normal lean VAT contains eosinophils, alternatively activated macrophages (AAM), invariant natural killer T cells (iNKTs), and regulatory T (T reg) cells that can promote insulin sensitivity and metabolic homeostasis (Chawla et al., 2011; Schipper et al., 2012; Wu et al., 2011). How lean, healthy VAT recruits and sustains these distinct immune cell types remains largely unknown. We previously reported that eosinophils reside in VAT and that eosinophil deficiency impairs Arginase-1+ AAM accumulation. VAT eosinophils are abundant in IL-5 transgenic mice and promote AAM accumulation and insulin sensitivity (Wu et al., 2011; Chawla et al., 2011). Prolonged VAT eosinophilia after helminth infection is also correlated with improved metabolic parameters in animals challenged with high-fat diet (HFD; Wu et al., 2011). Eosinophil production, bone marrow release and tissue recruitment and retention depend on several cytokines, chemokines, and integrins. IL-5 is integral at multiple levels, promoting eosinophil bone marrow production, release, and tissue recruitment, and is required for optimal systemic and local eosinophilia in diverse models of allergic inflammatory responses (Mould et al., 1997; Kopf et al., 1996; Foster et al., 1996). In contrast, IL-5 deficiency in unperturbed animals leads to a modest reduction in bone marrow, blood, and gastrointestinal tract eosinophil levels, indicating eosinophil production and recruitment to certain tissues can occur without IL-5 (Mishra et al., 1999; Kopf et al., 1996). Eotaxins (CCL11 and CCL24) are chemokines that recruit eosinophils, are central to eosinophil maintenance within the gastrointestinal tract, and can be up-regulated by IL-13 during allergic inflammation (Mishra et al., 1999; Rothenberg and Hogan, 2006; Voehringer et al., 2007). Eosinophils also use endothelial cell integrins, which can be increased by IL-4 and IL-13, to traffic into tissues (Blanchard and Rothenberg, 2009). The relative dependence of VAT eosinophils on these factors, including IL-4, IL-5, and IL-13, remains unknown. Innate lymphoid type 2 cells (ILC2s) are recently characterized innate cells widely distributed in mammalian tissues (Spits and Di Santo, 2011). Also, designated innate helper type 2 cells (Price et al., 2010), nuocytes (Neill et al., 2010), or natural helper cells (Moro et al., 2010), ILC2s share features with other populations of innate lymphocytes, including NK cells (ILC1) and ILC3, comprising the RORγt-dependent ILC: lymphoid tissue-inducer cells (LTic), innate IL-22 producing cells (also referred to as NK22, ILC22, NCR22, and NKR+ LTic) and innate IL-17-producing cells (Spits and Di Santo, 2011). ILCs all share a dependence on the transcription factor Id2 and the common-γ chain (γc) cytokine receptor (Spits and Di Santo, 2011). In response to the epithelial cytokines IL-25 and IL-33, ILC2s expand and produce large amounts of type 2 cytokines, particularly IL-13 and IL-5 (Hurst et al., 2002; Price et al., 2010; Moro et al., 2010; Neill et al., 2010), which can promote AAMs and eosinophils, respectively (Blanchard and Rothenberg, 2009; Martinez et al., 2009). Although ILC2s are functionally similar to CD4+ T helper type 2 (Th2) cells (Price et al., 2010), ILC2s are widely distributed within tissues independent of antigenic stimulation and appear poised to respond to epithelial signals. One of the earliest descriptions of ILC2s identified them within lymphoid structures in mouse and human mesenteric adipose tissues (Moro et al., 2010). With this in mind, we sought to quantify ILC2s in metabolically active perigonadal VAT and determine whether these cells and the cytokines they produce, including IL-5 and IL-13, were responsible for the localization of eosinophils and AAMs to this tissue under basal conditions and after their activation by cytokines or in response to intestinal helminth infection. RESULTS Eosinophils and IL-5 promote insulin sensitivity and lean physiology We previously reported metabolic consequences of eosinophil deficiency using dblGata1 mice (Wu et al., 2011). Because IL-5 can promote local and systemic eosinophilia, we compared metabolic parameters in eosinophil-deficient and IL-5–deficient C57BL/6 mice during HFD challenge. We used Red5 mice, which contain a tandem-dimer red fluorescent protein (tdTomato) linked by an internal ribosomal entry site (IRES) to a Cre element, replacing the first exon of the il5 gene (unpublished data), thus marking cells producing IL-5; Red5 homozygous mice are IL-5–deficient and the Cre element facilitates deletional studies based on IL-5 expression. To control for potential genetic or microbiome contributions to these phenotypes, we compared IL-5–deficient Red5 homozygote and IL-5-sufficient Red5 heterozygote mice. Eosinophil-deficient and IL-5-deficient animals fed HFD for 18–20 wk gained more weight (Fig. 1 a), with increased total body adiposity (Fig. 1 b) and perigonadal VAT weight (Fig. 1 c), as compared with IL-5–sufficient mice. Fasting glucose levels were elevated in both strains of mice (Fig. 1 d), and both had impaired glucose (Fig. 1 e) and insulin tolerance (Fig. 1 f and unpublished data). These findings support and extend our previous results (Wu et al., 2011) to implicate IL-5 in metabolic homeostasis. Figure 1. Deficiency of IL-5 or eosinophils promotes obesity and insulin resistance and decreases oxidative respiration and heat production in mice on HFD. (a–c) Mice of the indicated genotype were fed HFD or ND for 18–20 wk, and then total weight (a), percent adiposity by EchoMRI (b), and terminal perigonadal VAT weight (c) were determined. Results are representative of three independent experiments and include four to six animals per cohort. Fasting blood glucose (d), glucose tolerance testing (e) and insulin tolerance testing (f) were performed in mice on ND or HFD for 18–20 wk. Results are representative of three experiments. IL-5+/−, Red5 C57BL/6 R/+ heterozygotes; IL-5−/−, Red5R/R homozygous IL-5 knockouts. (g and h) CLAMS analysis was performed using individually housed groups of six C57BL/6 or C57BL/6 dblGata1 eosinophil-deficient mice after maintenance on HFD for 12 wk. Variations in oxygen consumption (g) and energy expenditure over time (h) were pooled among animals in each group and statistical analysis was performed using pairwise comparisons. Error bars are the mean ± SEM. P-values are shown. To further understand the mechanisms by which eosinophils and IL-5 influence metabolism, we placed eosinophil-deficient and -sufficient animals on HFD for 12 wk in metabolic cages. Although food and water intake and physical activity were not altered (unpublished data), total oxygen consumption (VO2) and energy utilization (heat) were decreased in eosinophil-deficient mice (Fig. 1, g and h); similar results occurred in IL-5–deficient animals (unpublished data). Thus, eosinophils and IL-5 do not alter caloric intake or caloric expenditures by enhancing physical activity. Instead, they may act in metabolically relevant tissue to promote increased oxidative metabolism and limit inflammation. Consistent with these findings, activation of iNKT IL-4 production (Lynch et al., 2012; Ji et al., 2012a) or exogenous IL-4 administration (Ricardo-Gonzalez et al., 2010) each promoted loss of adiposity and insulin sensitivity. ILC2s are the major source of IL-5 and IL-13 in VAT ILC2s have been implicated in promoting eosinophil influx into tissues such as the lung and intestines during allergic inflammation (Neill et al., 2010; Price et al., 2010; Liang et al., 2012). We used flow cytometry to analyze perigonadal VAT to ascertain a potential role for ILC2s in controlling eosinophils in this tissue. Perigonadal adipose tissue was isolated and digested to yield the stromal vascular fraction (SVF) enriched for hematopoietic cells, endothelial cells, and other stromal components, but devoid of adipocytes. After using lineage markers to exclude B cells, T cells, and NK cells, we could readily identify a discrete population of lymphoid cells in the SVF-expressing receptors for IL-2 (CD25), IL-7, and IL-33 (Fig. 2, a and b), as well as intracellular Gata3 (Fig. 2 b). These markers were previously demonstrated for ILC2s (Moro et al., 2010; Neill et al., 2010; Price et al., 2010). Similar to other ILC2s, VAT ILC2s were present in Rag-deficient mice but absent in Rag x γc-deficient and IL-7Rα–deficient mice (Fig. 2, a–c), strains previously shown to lack ILC2s. VAT ILC2s were present in male and female mice and in C57BL/6 and BALB/c mice in both WT and Rag-deficient (T/B cell–deficient) backgrounds, although consistently more abundant in C57BL/6 mice (see also Fig. 4 d, bottom, and not depicted). Thus, the SVF of perigonadal adipose tissue contains innate lymphoid cells with the phenotype of previously described ILC2s (Moro et al., 2010; Neill et al., 2010; Price et al., 2010). Figure 2. ILC2s are resident within VAT and are the primary cells expressing IL-5 and IL-13. (a and b) Representative ILC2s FACS plots (a and b) and frequency (c) of ILC2s from the VAT SVF of Rag2-deficient, WT, IL7Ra-deficient, and Rag2× γc–deficient C57BL/6 mice. Cells were pregated on lin− lymphoid cells (CD11b−, F4/80−, SiglecF−, SSC-lo, FSC-lo, CD45+; a) or lin− CD3e− CD4− (b). (d) Representative flow cytometry plots showing frequencies of IL-13+ and IL-5+ cells among various cell populations in VAT. (e) Expression of the indicated surface markers on VAT IL-5+ lin− cells (ILC2, red line) compared with VAT CD3ε+ T cells (blue line) and isotype controls (gray; a–e) Data are representative of two or more experiments. (f and g) IL-5 and IL-13 expression on the following VAT populations: CD4+ T cells (CD4), iNKT (aGC-loaded tetramer), CD8+ T cells (CD8), NK cells (NK1.1), CD3ε+ double-negative T cells (CD3ε), B cells (CD19), macrophages (CD11b), eosinophils (SiglecF), and lin− cells (SSC). Cells were pregated as shown in Fig. S2. Data are representative of two or more experiments. To assess the contribution of VAT ILC2s to the total IL-5 and IL-13 cytokine production in VAT, we used reporter mice with knock-in fluorescent alleles at various gene loci, thus allowing interrogation of the cytokine expression of these cells without the need for restimulation ex vivo. Both adipose SVF cells from Red5 mice, which mark IL-5–expressing cells with tdTomato expression, and YetCre13 x ROSA-YFP mice, which functionally mark cells that have ever expressed IL-13 by establishing constitutive YFP expression from the ROSA26 locus (Price et al., 2010), each contained cells marked by in situ IL-5 and IL-13 expression (Fig. 2 d). IL-5–expressing cells were negative for the myeloid marker CD11b, and included a small subset of CD4+ CD3e+ IL33R+ (T1/ST2+) Th2 cells (5–15%) and a large population of lineage-negative cells (85–95%). These VAT lineage-negative cells expressed CD25 (IL2Rα), IL33R (T1/ST2), CD122 (IL2Rβ), Thy1.2 (CD90.2), c-Kit, Sca-1, and KRLG1, and were uniformly negative for T cell markers, including CD4, CD8, CD3ε, TCR-β, and TCR-γδ (Fig. 2 e), consistent with previously described ILC2s (Moro et al., 2010; Neill et al., 2010; Price et al., 2010). VAT B cells, CD8+ T cells, CD3ε+ CD4− CD8− “double-negative” T cells, macrophages, eosinophils, and α-galactosylceramide (αGC)-reactive invariant NKT cells (iNKT) did not show IL-5 fluorescence (Fig. 2 f and gating in Fig. S2), consistent with previous studies about lung IL-5+ cells (Ikutani et al., 2012). Similar results were found for VAT IL-13–expressing cells, although small percentages of eosinophils (0.2–0.4%) and iNKT cells (3–5%) expressed IL-13 using lineage-tracked expression (Fig. 2 g). After prolonged IL-33 administration or helminth infection, ILC2s remain the predominant IL-5– and IL-13–expressing cells, with no significant increased expression by macrophages, eosinophils, or other lymphocytes (Figs. S1 and S2 and unpublished data). Together, these results establish that ILC2s are the predominant IL-5– and IL-13–expressing cells in VAT and that rare Th2 cells account for most of the remaining cytokine-expressing cells. As assessed using these reporter alleles, significant proportions of VAT ILC2s spontaneously produced IL-5 and IL-13 (Fig. 3, a and b), and this was particularly striking for IL-5. We could identify no phenotypic differences between cytokine-positive and -negative ILC2s, suggesting a uniform population with variable cytokine expression. IL-13 cytokine-marked cells, the great majority of which are ILC2s (Fig. 2 d), were readily detected in close apposition to the adipose vasculature and dispersed within VAT (Fig. 3c). Unlike ILC2s reported in mesenteric lymph nodes and mesenteric lymphoid clusters (Moro et al., 2010), we were unable to identify discrete lymphoid structures within perigonadal adipose tissue (unpublished data). In contrast to VAT ILC2s, bone marrow ILC2s (lineage− IL7Rα+ T1/ST2+; Brickshawana et al., 2011), which were also described as ILC2 precursors (Hoyler et al., 2012), did not express basal IL-13 as assessed with IL-13 lineage tracking (2.0 ± 0.3%, n = 8), although marrow ILC2s were predominantly IL-4 competent, as assessed using cells from 4get mice (85.5 ± 7.4%, n = 3). Although a subset of VAT ILC2s were competent to make IL-4 (4get+; Fig. 3, a and b), they were unmarked by reporter expression in KN2 mice (unpublished data), whose cells contain an IL-4 replacement allele and reveal cells actively producing IL-4 in situ (Mohrs et al., 2001; Wu et al., 2011), as previously described (Price et al., 2010; Wu et al., 2011). Figure 3. VAT ILC2s spontaneously produce IL-5 and IL-13 in vivo and ex vivo, and respond robustly to IL-33. Reporter cytokine expression by VAT ILC2s (lin− IL7Rα+ T1/ST2+) from 4get (IL-4 competence), Red5 (IL-5), and YetCre13 x ROSA-YFP (IL-13 reporter) mice (a), with percentages of VAT ILC2s positive for each cytokine marker (b) are shown. (c) Representative image shows spontaneous IL-13 reporter+ cells (YetCre13 Y/+ x ROSA-ZsGreen) in freshly isolated, whole mounted VAT. (d) VAT total ILC2s (lin− thy1.2+ CD25+) were sorted and cultured in vitro for 72 h with the indicated combinations of IL-2, IL-7, IL-33, and PMA/ionomycin, and supernatant cytokine levels were determined (picogram per milliliter). (e) VAT IL-5+ ILC2s (lin− thy1.2+ Red5+), IL-5+ (Red5+) CD4+ T cells, and IL-5–negative (Red5−) CD4+ T cells were cultured with IL-7 (first bar) or PMA/Ionomycin (second bar; d and e) Results are representative of two or more experiments. (a) Numbers in brackets or over lines indicate percentage of cells within the gate. Nd, not detected. To confirm the fidelity of the cytokine reporters and confirm additional cytokines secreted by these cells, VAT ILC2s (lineage-negative Thy1.2+ CD25+) were purified by flow cytometry and placed in vitro for 72 h with various cytokines. Low amounts of IL-5, IL-6, IL-13, and GM-CSF spontaneously accumulated in the VAT ILC2 culture supernatants (Fig. 3, d and e, and unpublished data). After addition of IL-33, greater amounts of IL-5, IL-6, IL-9, IL-13, and GM-CSF accumulated (Fig. 3 d), and these cytokines increased further with the addition of IL-2 or IL-7, similar to results reported by ILC2s from other tissues (Moro et al., 2010; Halim et al., 2012). Together, these data suggest that VAT ILC2s spontaneously produce IL-5 and IL-13, and can respond to IL-33 with high levels of cytokine production, as shown for other ILC2s. Although rare in VAT, IL-5+ (Red5+) CD4+ T cells revealed a similar capacity to produce IL-2, IL-5, IL-6, IL-13, and GM-CSF after in vitro culture with PMA/ionomycin (Fig. 3 e). These data indicate IL-5+ ILC2s are numerically predominant within VAT, but otherwise have a similar cytokine capacity to IL-5+ Th2 cells. ILC2s are required to sustain adipose eosinophils and AAMs Eosinophils home to and are sustained in VAT, where they promote AAM maintenance and systemic insulin sensitivity (Wu et al., 2011). As assessed after mitotic labeling during bone marrow differentiation, eosinophils had significantly lower turnover in VAT as compared with spleen and lung, consistent with the presence of recruitment, retention, or survival signals in adipose tissue (Fig. 4 a). Although present in Rag-deficient mice, VAT eosinophils were substantially and tissue-specifically reduced in Rag x γc-deficient mice that lack ILC2s (Fig. 4 b). Prolonged HFD results in a decline of VAT eosinophils, as previously described (Wu et al., 2011), which is associated with a loss of VAT ILC2s but increased numbers of total VAT macrophages and CD8+ T cells (Fig. 4 c). In contrast, lung ILC2s were not reduced after HFD (unpublished data). Indeed, VAT ILC2 cell numbers correlate strongly with VAT eosinophils across multiple mouse WT strains, genetic mutations, and dietary perturbations, whereas total CD4+ T cells show no corresponding correlation (Fig. 4 d). Figure 4. VAT eosinophils and AAMs are dependent on ILC2s. (a) C57BL/6 male mice were injected i.p. for the indicated number of days shown with 250 µg Edu per mouse. FACS analysis was performed after pre-gating on eosinophils (Fig. S1). Data are from one experiment with three animals per group, and are representative of two independent experiments. (b) Frequency of eosinophils among total viable VAT, lung, or spleen cells from WT, Rag2-deficient, and Rag2× γc–deficient C57BL/6 mice. Data are representative of three experiments. (c) WT C57BL/6 mice were fed a ND or HFD for 3–4 mo, and VAT SVF was examined for immune cell composition. Pooled data from three independent experiments are shown. (d) Correlation between VAT ILC2s or VAT CD4+ T cells and VAT eosinophils. Mouse strains shown include Rag x γc (Rag2 deficient x γc deficient), WT B6 (WT C57BL/6), WT BALB (WT BALB/c), Rag1−/− (Rag1 deficient), WT B6 HFD (WT C57BL/6 fed HFD for 3–4 mo), IL-13 deleter (YetCre13 Y/Y x ROSA-DTA BALB/c), and IL-5 deleter (Red5 R/R x ROSA-DTA C57BL/6). Strains were fed ND unless indicated. Each data point represents pooled data from at least five mice over multiple experiments. Pearson correlation coefficient is shown with significance. CD4+ T cell data are not shown for strains on the Rag-deficient background. (e–i) ILC2s, CD4+ T cells, CD8+ T cells, macrophages, and eosinophils were enumerated from the VAT (or indicated compartment) from the indicated strains and tissues on a BALB/c background (e–g) or C57BL/6 background (h and i). Data were pooled from two or more experiments. (j) VAT IL-5+ (Red5+) ILC2s or IL-5+ (Red5+) CD4+ T cells from the strains indicated. (k and l) Arginase-1+ (YFP+) AAMs were enumerated from WT YARG or γc-deficient YARG C57BL/6 basal VAT (k) or WT YARG or YetCre13 x ROSA-DTA YARG (IL-13 deleter) BALB/c (l) homeostatic VAT. Results contain pooled data from two or more experiments with 2–4 mice per experiment. *, P 2), a one-tailed ANOVA was performed with Tukey’s post-test correction. Supplementary Material Supplemental Material
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Group 2 Innate Lymphoid Cells Are Critical for the Initiation of Adaptive T Helper 2 Cell-Mediated Allergic Lung Inflammation
Introduction Allergy is one of the most common health problems in the industrialized world. A type 2 immune response is responsible for most allergen-induced inflammation at mucosal surfaces and is reflected in an overproduction of T helper 2 (Th2) cell-type (type 2) cytokines and immunoglobulin E (IgE) (Pulendran and Artis, 2012). Individuals might be sensitized to specific allergens, which stimulate naive CD4+ T cells to differentiate into Th2 cells. The reexposure of sensitized individuals to the same allergens causes a robust stimulation of memory Th2 cells that secrete the cardinal type 2 effector cytokines interleukin-4 (IL-4), IL-5, IL-9, and IL-13 (Kim et al., 2010; Lloyd and Hessel, 2010). In parallel, antigen crosslinking of IgE bound to FcεRI on mast cells and basophils leads to activation and degranulation, amplifying allergic inflammation of the affected tissues. Currently, the mechanisms by which allergens initiate the differentiation of naive CD4+ T cells into Th2 cells during the sensitization phase are not well understood. It is generally thought that the cytokine environment dictates the differentiation of naive CD4+ T cells into various populations of Th cells. IL-4 in particular is believed to be critical for Th2 cell differentiation, and binding to its receptor activates STAT6, which induces the expression of the key transcription factor GATA3 and drives the production of type-2 cytokines. However, the initial source of IL-4 responsible for the differentiation of naive CD4+ T cells into Th2 cells has been unclear because multiple cell populations, including natural killer T (NKT) cells, γδ T cells, basophils, dendritic cells (DCs), and naive CD4+ T cells can produce IL-4 (Weiss and Brown, 2001; Yamane and Paul, 2013). Moreover, Th2 cell differentiation can also be induced in vitro in the absence of exogenous IL-4 by IL-2, which induces IL-4Rα expression (Liao et al., 2008). Additionally, Th2 cell responses can be induced in vivo in IL-4- or IL-4R-deficient mice, indicating that an IL-4-independent pathway of Th2 cell differentiation exists. Currently, how IL-4-independent development of Th2 cells occurs is not well understood. Notably, epithelial cell-derived cytokines, including IL-33, thymic stromal lymphopoietin (TSLP), and IL-25, are known to promote Th2 cell responses and allergic inflammation (Islam and Luster, 2012). The receptors for these cytokines are expressed by a variety of cell types including DCs, basophils, and NKT cells, but not naive CD4+ T cells. Mice deficient for the IL-33 receptor, ST2, produce reduced amounts of IL-4 and IL-5 in response to challenge with helminth antigen (Townsend et al., 2000) and IL-33 has been reported to activate DCs and induce allergic airway inflammation (Besnard et al., 2011). The stimulation of DCs (Zhou et al., 2005) and basophils (Siracusa et al., 2011) by TSLP is also thought to be critical for allergic inflammation. Nevertheless, the exact mechanisms by which these epithelial cell-derived cytokines promote Th2 cell differentiation are still unclear. Group 2 innate lymphoid cells (ILC2s, previously termed natural helper cells, nuocytes, or Ih2 cells) (Spits et al., 2013), recently discovered in the gut (Moro et al., 2010; Neill et al., 2010; Price et al., 2010) and airway mucosa of mice (Chang et al., 2011; Halim et al., 2012a; Monticelli et al., 2011) and man (Mjösberg et al., 2011), are rapid and potent producers of the type 2 cytokines IL-5 and IL-13. With the discovery of ILC2s, we now understand that type 2 immunity comprises both innate and adaptive components. Papain, a protease known to be allergenic to humans and causes occupational asthma (Novey et al., 1979), is often used as a model allergen. Subcutaneous injection of papain into mice induces Th2 cell-mediated immunity (Tang et al., 2010). We have previously shown that intranasal administration of papain rapidly induces activation of lung IL-5 and IL-13-producing ILC2s, lung eosinophilia, and mucus hyperproduction in RAG-deficient mice. Thus, ILC2 activation can induce T cell- and IgE-independent acute allergic lung inflammation (Halim et al., 2012a). We also found that retinoic acid receptor related orphan receptor alpha (RORα) is critical for ILC2 development, and RORα-deficient Staggerer (Rora sg/sg) bone marrow (BM)-transplanted (BMT) mice are specifically deficient for ILC2s (Halim et al., 2012b; Wong et al., 2012). These mice fail to develop acute type 2 lung inflammation after sensitization with papain. Notably, Rora sg/sg CD4+ T cells are not intrinsically impaired to develop into Th2 cells, and the observed defect in acute type 2 inflammation can be attributed to the lack of functional ILC2s in Rora sg/sg BMT mice. Because ILC2s are a potent and early source of type 2 cytokines, we hypothesized that they could influence the downstream adaptive Th2 cell response. To test this hypothesis, we have examined the effects of ILC2-deficiency on Th2 cell responses to papain. Here we show that ILC2s were required for Th2-cell-mediated allergic lung inflammation. IL-13 produced by activated ILC2s was critical for promoting the migration of activated lung DCs to the draining lymph node (LN), where they induced the differentiation of naive CD4+ T cells into Th2 cells. Thus, our data reveal how innate ILC2 can play a critical role in the generation of adaptive Th2 cell responses to allergens. Results Protease-Allergen Papain Induced a Strong Innate and Adaptive Type-2 Immune Response Mice were sensitized to Th2 cell-mediated allergic responses by the intranasal administration of papain (or heat-inactivated papain as a control) on days 0 and 1, followed by two challenges on days 13 and 20 (Figure 1A). Serum IgE titers increased upon sensitization and subsequent challenges (Figure 1B). Leukocytes, including eosinophils and neutrophils, rapidly infiltrated into bronchoalveolar lavage (BAL) and lung tissue following sensitization, and low amounts of type 2 cytokines were detected in the BAL on day 2 (Figures 1C and D). Activated ILC2s rather than Th2 cells likely mediated these early responses to papain, since similar responses were observed in Rag1 −/− mice that have ILC2s but lack T and B cells (see Figures S1A–S1C available online). The subsequent challenge of papain-sensitized mice induced the infiltration of substantially higher numbers of eosinophils in the BAL (9-fold increase, p = 0.02) and the lung (15-fold increase, p = 0.005) as well as significantly higher concentrations of type 2 cytokines in the BAL (p = 0.0002) on day 21 (Figures 1C and D). Th2 cells likely mediated these latter responses to papain since Rag1 −/− mice did not show the augmented immune response (Figures S1A–S1C). In wild-type (WT) mice, the draining mediastinal lymph nodes (mLN) were enlarged with substantially increased numbers of CD4+ T cells and B cells on day 21 (data not shown). Notably, basophils and mast cells were not detected in substantial numbers at the time-points investigated. To confirm the induction of papain-specific Th2 cells, we isolated lymphocytes from the lungs, peripheral (inguinal) LNs (pLN), and spleens of papain-treated or control mice on day 21 and restimulated them with recall-antigen (Figure 1E) or immobilized anti-CD3ε plus anti-CD28 (Figure S1D). The in vitro-stimulated lung lymphocytes from papain-treated, but not control, mice produced IL-4, IL-5, and IL-13. We also analyzed the expression of GATA3, a critical transcription factor for Th2 cell differentiation (Zheng and Flavell, 1997), in CD4+ T cells on day 21 by flow cytometry (Figures S1E and S1F). Both the percentages and the absolute numbers of GATA3+ CD4+ T cells were higher in the mLNs of the papain-treated mice compared to control mice (Figures 1F and 1G). To identify the cellular source of type 2 cytokines at various time points, we stained for intracellular IL-5 and IL-13 and cell-type-specific surface markers in the lung (Figure 1H) and mLN (Figure S1I). As expected from our previous studies (Halim et al., 2012a), IL-5+IL-13+ cells on day 2 were primarily ILC2s. On day 21, the majority of IL-5+IL-13+ cells were CD4+ T cells (Figure 1H), while ILC2s also expanded and comprised approximately 30% of IL-5+IL-13+ cells in the lung on day 21 (Figure 1H; Figures S1J and S1K). Thus, intranasal administration of papain initially stimulated ILC2s and also induced Th2 cell differentiation, whereas the subsequent challenges with papain stimulated primed Th2 cells, resulting in type 2 cytokine production, increased IgE titers, and eosinophilic lung inflammation. ILC2s Were Required for Induction of the Adaptive Type-2 Immune Response On the basis of the above results, we hypothesized that ILC2s promote Th2 cell differentiation in papain-treated mice. To test this, we investigated the effects of ILC2-deficiency on Th2 cell responses to papain. We have previously shown that the transcription factor RORα is required for ILC2 development and that transplantation of BM from RORα mutant Rora sg/sg mice into irradiated WT mice generates ILC2-deficient mice (Halim et al., 2012b; Wong et al., 2012). Importantly, Rora is not highly expressed in other hematopoietic cells, including naive and memory T cells (Figure S2A). We have also previously shown that Rora sg/sg CD4+ T cells have no inherent defect in their capacity to differentiate into Th2 cells in vitro, indicating that RORα is not intrinsically required for Th2 cell differentiation (Halim et al., 2012b). Thus, WT bone-marrow-transplanted (WT BMT) and ILC2-deficient Rora sg/sg BMT mice were administered papain as in Figure 1A, and Th2 cell responses were compared after the second challenge (day 20). Rora sg/sg BMT mice had strikingly fewer eosinophils in the BAL, lung, and mLN, and fewer neutrophils, DCs, and CD4+ T cells in the lung parenchyma and mLN than WT BMT mice (Figures 2A and 2B). The inability of Rora sg/sg BMT mice to mount strong Th2 cell responses to papain was further supported by the substantially lower amounts of type 2 cytokines and the Th2 cell-associated chemokines CCL22 and CCL17 (Bromley et al., 2008) in the BAL (Figures 2C and 2D) as compared to controls. Papain-challenged Rora sg/sg BMT mice also displayed substantially reduced levels of IgE in the serum (Figure 2E) and substantially lower numbers of GATA3+ CD4+ T cells in the lung compared to WT BMT mice (Figure 2F; Figure S2B). Furthermore, the in vitro restimulation of lymphocytes from the lung and mLN of Rora sg/sg BMT mice with recall-antigen resulted in substantially less type 2 cytokine production than those from WT BMT mice (Figure 2G). Histological analyses also revealed substantially less mucus production and inflammation in the lungs of Rora sg/sg BMT mice than WT BMT mice (Figure 2H; Figures S2C–S2E). Together, these results clearly demonstrate a profound defect in Th2 cell immunity in the absence of ILC2s. IL-4 Was Not Required for an Efficient Adaptive Th2 Cell Immune Response to Inhaled Protease Allergen Because IL-4 is thought to play a critical role in the differentiation of naive CD4+ T cells into Th2 cells (Pulendran and Artis, 2012), the above results suggested that ILC2s might be a source of IL-4 in papain-treated mice. However, purified ILC2s produced large amounts of IL-5 and IL-13 but very little IL-4 (Figures S3A and S3B). To clarify the role of IL-4 in papain-induced Th2 cell responses, we tested the activation of Th2 cells in Il4 −/− mice. Unexpectedly, Il4 −/− mice mounted a strong Th2 cell response to papain and they had comparable levels of eosinophils in the BAL as WT mice, although lung eosinophil numbers were slightly lower (Figure 3A). They also exhibited no substantial difference in the numbers of CD4+ T cells in the lung and mLN (Figure 3B), the amounts of IL-5 and IL-13 in the BAL (Figure 3C), or the number of GATA3+ Th2 cells in the lung and mLN (Figure 3E; Figure S3C) when compared to WT mice. As expected, Il4 −/− mice had no detectable IL-4 in the BAL (Figure 3C), and no detectable serum IgE (Figure 3D), which is known to be IL-4-dependent (Finkelman et al., 1988). Thus, IL-4 was dispensable for papain-induced Th2 cell generation, suggesting that ILC2s promote Th2 cell responses by an IL-4-independent mechanism. ILC2s Were Instrumental for Induction of Th2 Cells in the mLN To elucidate how ILC2s promote Th2 cell-mediated allergic responses to papain, we analyzed the initiation of Th2 cell differentiation from naive CD4+ T cells (Figure S4A). Following papain treatment on days 0 and 1, the numbers of B cells and CD4+ T cells in mLN steadily increased until day 4 (Figure 4A). The induction of Th2 cells was observed by day 6 via intracellular staining for type 2 cytokines in CD4+ T cells (data not shown). CD11c+MHCIIhi activated DCs in the lung rapidly increased in number, followed by their increase in the mLN (Figure 4A; Figures S4B and S4C). Thus, papain-activated lung DCs likely migrated into the draining mLN where they stimulated naive CD4+ cells. We then compared Th2 cell generation in the mLN of WT BMT and Rora sg/sg BMT mice 6 days after the initial papain administration. The in vitro restimulation of mLN lymphocytes resulted in substantially lower IL-4, IL-5, and IL-13 production by Rora sg/sg BMT mouse lymphocytes compared to WT controls (Figures 4B and 4C). Intracellular cytokine staining also demonstrated that the numbers of CD4+ Th2 cells expressing IL-5 and IL-13 in the mLNs and lungs of Rora sg/sg BMT mice were substantially lower than those of WT BMT mice on day 6 (Figure 4D). Similar results were obtained when mice were stimulated with house dust mite (HDM) or a fungal protease-allergen (Figure S4D). Importantly, the adoptive transfer of ILC2s into papain-treated Rora sg/sg BMT mice restored Th2 cell generation (Figures 4E; Figure S4E). These results showed that ILC2s were critical for the differentiation of naive CD4+ T cells into Th2 cells. Lung ILC2 activation is contingent on stimulation via IL-33, an alarmin produced in response to a broad range of allergens (Hardman et al., 2013). We found that papain-driven IL-13 production from ILC2, eosinophilic lung inflammation, and Th2 cell differentiation were all impaired in intranasally challenged IL-33-deficient mice (Figures S4F-H). Moreover, intranasal administration of IL-33 alone directly stimulated lung ILC2s without papain treatment (Figure S4I) as reported (Barlow et al., 2012). We then intranasally administered ovalbumin (OVA) antigen together with IL-33 to WT BMT or Rora sg/sg BMT mice, which were also intravenously injected with carboxyfluorescein succinimidyl ester (CFSE)-labeled CD4+ T cells from the OVA-specific T cell receptor transgenic OT-II mice. Very few OT-II T cells (CFSE+) were recovered in the mLNs of Rora sg/sg BMT mice as compared to WT, and the numbers of IL-4+ IL-13+ Th2 cells generated in Rora sg/sg BMT mice were substantially lower than those in WT BMT mice. Moreover, the impaired Th2 cell differentiation was rescued by ILC2 transplantation (Figure 4F). These results demonstrate that IL-33-mediated ILC2 activation was critical for effective Th2 cell differentiation, likely in response to the intranasal administration of a broad range of antigens. IL-13 from ILC2 Promoted Th2 Cell Differentiation in the Draining LN The above results showed that ILC2s promoted Th2 cell differentiation while producing a large amount of IL-13 but little IL-4. Therefore, we tested whether IL-13 is involved in Th2 cell differentiation in papain-treated mice. Intranasal papain treatment of IL-13-deficient mice generated substantially fewer Th2 cells (IL-5+ CD4+ T cells) in the mLN compared to WT mice (Figure 5A). Moreover, IL-13 neutralization also inhibited Th2 cell differentiation in papain-treated WT mice (Figure 5B), whereas IL-13 injection enabled the generation of Th2 cells in papain-treated Rora sg/sg BMT mice (Figure 5C). The role of ILC2-derived IL-13 for Th2 cell differentiation was confirmed in a TCR-transgenic model, in which CFSE-labeled OT-II T cells were injected into WT or Rora sg/sg BMT mice. The mice then received intranasal administration of OVA and papain, and OT-II T cells in the mLN were analyzed 6 days later. Although OT-II T cells proliferated in both WT and Rora sg/sg BMT mice, the differentiation of naive OT-II T cells into Th2 cells was substantially impaired in Rora sg/sg BMT mice (Figure 5D). Notably, this impaired Th2 cell differentiation in Rora sg/sg BMT mice was rescued by the intranasal injection of IL-13 (Figure 5E). WT ILC2 transplantation also rescued Th2 cell production whereas IL-13-deficient ILC2s did not (Figure 5F). Interestingly, the intranasal administration of OVA alone, without papain, into WT mice that were injected with CD4+ OT-II T cells did not induce detectable Th2 cell differentiation in mLN, whereas the coadministration of OVA plus IL-13 efficiently induced Th2 cell differentiation of OT-II T cells (Figure 5G). Intracellular staining for IL-13 after papain stimulation identified ILC2 as the primary cellular source, and ILC2-deficient mice did not produce IL-13 during the acute inflammatory response (Halim et al., 2012a; 2012b). Analysis of Il13 egfp/+ reporter mice also confirmed that ILC2s are the predominant Il13 expressing cells in papain-treated lungs (Figure S5A). Together, these results indicated that ILC2-derived IL-13 was critical for the differentiation of Th2 cells. IL-13 Promoted CD40+ DC Migration to the Draining LN We detected the IL-13 receptor on activated DCs, but not on CD4+ T cells (Figure S6A), and exogenously added IL-13 did not have a direct effect on in vitro Th2 cell differentiation (Figure S6B). Because DCs are known to play a critical role in Th2 cell induction to inhaled allergens (Kool et al., 2012), we hypothesized that ILC2-derived IL-13 might influence DC function. We first compared DCs in the lungs of WT mice treated with papain and those treated with heat-inactivated papain and found no differences in the expression of CD44, CD86, OX40L, and ICOSL (data not shown). We then analyzed DCs in the lungs and mLNs of WT and Rora sg/sg BMT mice treated with papain. No substantial differences in the number of activated DCs or their phenotype (CD40 and CCR7 expression) was observed in the lung between WT BMT and Rora sg/sg BMT mice (Figures 6A-6C). In contrast, a striking difference in the mLN DC populations was seen between WT BMT and Rora sg/sg BMT mice. More than 50% of activated DCs in the mLNs of WT BMT mice expressed CD40, which has been shown to be critical for efficient Th2 cell differentiation (Jenkins et al., 2008; MacDonald et al., 2002). Rora sg/sg BMT mice showed substantially reduced CD40+ DC numbers in the mLN (Figure 6D). Importantly, this impairment was rescued by IL-13 injection (Figures 6D), whereas IL-13 neutralization substantially reduced CD40+ DCs in the mLN of papain-treated WT mice (Figure 6E). We also coadministered papain and the synthetic antigen DQ-OVA, which becomes fluorescent upon processing by antigen-presenting cells, and analyzed antigen processing by DCs. The processing of antigen by lung DCs was not affected in Rora sg/sg BMT mice, whereas the trafficking of DQ-labeled cells to the draining LN was substantially reduced (Figure 6F). These data suggested that ILC2-derived IL-13 might be critical for the migration of activated antigen-licensed CD40+ DCs from the lung to the draining mLN in papain-treated mice. To further investigate the effect of IL-13 on DC migration, we prepared lung tissue explants from papain-treated WT or Il13 −/− mice and tested the migration of lung tissue-resident DC toward a gradient of the DC chemokine CCL21 in transwell cultures (Figures S6C and S6D). CCL21 (or CCL19) signaling via CCR7 is critical for DC migration to secondary lymphoid organs (Förster et al., 1999). DCs in lung tissue explants prepared from papain-treated WT mice demonstrated robust specific chemotaxis in the presence of CCL21, whereas IL-13 had no effect on its own (Figures S6D and S6E). The migration of Il13 −/− mouse lung DCs toward CCL21 was substantially lower than that of WT DCs but was rescued by the administration of recombinant IL-13 into the mice (Figure 6G). It has been reported that prostaglandin E2 (PGE2) signaling via its receptor, EP4, is necessary to sensitize CCR7+ DCs to a CCL21 chemokine gradient (Kabashima et al., 2003; Luft et al., 2002; Scandella et al., 2002). IL-13 is also known to induce PGE2 production in DCs and macrophages (Legler et al., 2006; Rey et al., 1999). Indeed, IL-13 stimulation of lung leukocytes induced PGE2 production (Figure S6F). Gene-expression analysis indicated high expression of Ptger4 (EP4) by naive lung DCs (Figure S6G). Furthermore, our flow-cytometric analyses showed that intranasal IL-13 treatment of mice upregulated EP4 expression on lung DCs as compared to control PBS-treated mice (Figure S6H). Thus, we tested whether EP4 was involved in DC migration in our system by using lung explant cultures of naive WT mice. The in vitro DC migration was substantially inhibited by IL-13 neutralization but was rescued by simultaneously adding an EP4-agonist (Figure 6H). EP4-antagonist also mimicked IL-13-neutralization and substantially inhibited DC migration (Figure 6I). Overall, these results suggested that IL-13 influenced lung DC migration, in part by modifying the PGE2-EP4 pathway. The migration of activated DCs to the draining LN is thought to be essential for the induction of Th2 cell differentiation (Phythian-Adams et al., 2010; van Rijt et al., 2005). Indeed, papain-stimulated mLN DCs efficiently induced Th2 cell differentiation in vitro (Figure S6I). Furthermore, papain-induced Th2 cell-mediated allergic lung inflammation was impaired in the LN-deficient Rag2 −/− Il2rg −/− mice transplanted with WT or Rora sg/sg BM (Figures S6J–S6M). Thus, the migration of activated lung DCs to the mLN was critical for the initiation of Th2 cell differentiation induced by inhaled allergens. Discussion By using ILC2-deficient mice generated by transplanting BM of the Rora mutant Staggerer mice into irradiated recipients, we have demonstrated that ILC2s were required for efficient Th2 cell-mediated allergic lung inflammation induced by repeated intranasal administration of the protease-allergen papain. The inability of ILC2-deficient mice to mount strong allergic lung inflammation in response to intranasal papain was due to impaired Th2 cell differentiation in the draining mLN, and could be rescued in vivo by reconstituting ILC2s. Therefore, ILC2s played a critical role in the differentiation of naive CD4+ T cells into Th2 cells. Although IL-4 is thought to be critical for Th2 cell differentiation, the Th2 cell-promoting effect of ILC2s appeared to be mediated by IL-13 rather than IL-4, because IL-4-deficient mice mounted a potent Th2 cell-mediated response to papain, whereas IL-13-deficient mice did not. Furthermore, the intranasal administration of IL-13 into ILC2-deficient mice enabled these mice to mount a normal Th2 cell response to papain, whereas IL-13 neutralization in WT mice inhibited the papain-induced Th2 cell response. The transplantation of IL-13-deficient ILC2s into ILC2-deficient mice, unlike WT ILC2 transplantation, did not rescue this impaired Th2 cell differentiation, and the intranasal administration of IL-13 and OVA without papain into WT mice also promoted OVA-specific OT-II T cell differentiation into Th2 cells. Taken together, these results indicate that ILC2-derived IL-13 was critical for the differentiation of naive CD4+ T cells into Th2 cells in the mLN. IL-13 is known to be a pro-Th2 cytokine (Wynn, 2003). The neutralization of IL-13 inhibits asthma symptoms in OVA-sensitized and challenged mice (Grünig et al., 1998), and IL-13-deficient mice have an impaired Th2 cell response to parasite infections (McKenzie et al., 1998). However, the source of IL-13 and the mechanisms by which IL-13 promotes Th2 cell differentiation have remained unclear. In the current study with papain-treated mice, ILC2s were the main source of IL-13. Although basophils and mast cells are also known to be capable of producing IL-13 (Kroeger et al., 2009), they were undetectable in papain-treated mouse lungs or mLNs. The receptor for IL-13 consists of IL-4Rα and IL-13Rα (Mentink-Kane and Wynn, 2004). DCs expressed IL-13Rα1, which was undetectable on naive CD4+ T cells. IL-13 also had no effect on Th2 cell differentiation in vitro (Figure S6, also [McKenzie et al., 1998]), indicating that IL-13 is unlikely to act directly on naive CD4+ T cells. Instead, DCs seemed to be the main target of ILC2-derived IL-13 in papain-treated mice. DCs in the draining mLN of WT and ILC2-deficient mice treated with papain differed substantially in their expression of the costimulatory ligand CD40. The effects of IL-13 administration on ILC2-deficient mice and IL-13 neutralization in WT mice indicated that ILC2-derived IL-13 was likely responsible for CD40+ DCs in the mLN. However, ILC2-derived IL-13 did not appear to directly induce CD40 expression on DCs, because DCs in the lungs of WT and ILC2-deficient mice treated with papain did not differ substantially in their expression of CD40 or their processing of antigen (DQ-OVA). Instead, IL-13 appeared to stimulate the migration of activated DCs expressing CD40 from the lung to the mLN. Our in vitro studies with Il13 −/− lung explants and IL-13-neutralization demonstrated that IL-13 plays an important role for lung DC migration toward the DC chemokine CCL21, which binds to its receptor, CCR7 (Förster et al., 1999). Although CCR7 is known to be critical for DC migration to the draining LN, WT and ILC2-deficient mice treated with papain did not differ in terms of lung DC CCR7 expression. It has been reported that CCR7 expression alone is insufficient for skin DC migration toward a CCL21 chemokine gradient, requiring additional stimuli, which can be provided by the ligation of the PGE2-receptor EP4 (Kabashima et al., 2003; Luft et al., 2002; Scandella et al., 2002). Because IL-13 stimulates the production of PGE2 by DCs and macrophages (Legler et al., 2006; Rey et al., 1999), it is possible that this is the mechanism by which IL-13 promotes DC migration to the draining LN. The effects of a EP4 agonist and antagonist on DC migration in vitro, as well as EP4 upregulation, and PGE2 production by IL-13 treatment further supported the notion that IL-13 promotes CCR7+ DC migration, in part through its influence on the EP4-PGE2 pathway. It is well established that tissue DCs encountering antigens migrate to draining LNs, where they present antigens to naive T cells (Randolph et al., 2005). The current study also highlighted the importance of LNs as the site of Th2 cell differentiation. Repeated intranasal papain treatment induced much weaker allergic lung inflammation in Rag2−/−Il2rg−/− mice transplanted with WT BM cells than that in irradiated congenic WT recipient mice. We have previously shown that the former mice have normal ILC2s and other lymphocytes (Halim et al., 2012b). We believe that the observed differences are due to the lack of LNs in the former mice. Although papain treatment activated lung DCs, antigen presentation within the lung appeared to be very inefficient compared to antigen presentation in the draining mLN, and the migration of activated DCs into the mLN was critical for efficient activation of naive CD4+ T cells. It remains to be determined whether CD40 on DCs is directly responsible for the differentiation of naive CD4+ T cells into Th2 cells in papain-treated mice. Studies with CD40-deficient DCs show that the interaction between CD40 and its ligand (CD154) is required for Th2, but not Th1, cell responses (MacDonald et al., 2002). However, CD154 expression on CD4+ cells is not essential for Th2 cell differentiation (Jenkins et al., 2008). Several other costimulatory receptor-ligand combinations, including ICOS-ICOSL (Tafuri et al., 2001) and OX40-OX40L (Jenkins et al., 2007), are also known to be involved in Th2 cell differentiation. However, how signals generated by these costimulatory receptor-ligand interactions in naive CD4+ T cells lead to GATA3 activation, which is critical for Th2 cell differentiation (Paul, 2010), are currently unknown. While the precise mechanisms by which Th2 cell differentiation is initiated in the mLN of papain-treated mice is still unclear, it should be noted that papain treatment or IL-13 administration does not induce IL-12p40 or IL-12p35 expression, which is thought to be critical for Th1 cell differentiation. IL-12p40 neutralization also had no effect on papain induced DC migration (data not shown). We have also demonstrated that ILC2 activation and Th2 cell differentiation in papain-treated mice was IL-33-dependent. IL-33, which is considered to be an alarmin, is constitutively expressed in the nuclei of airway epithelial cells and rapidly released upon epithelial cell damage. Papain, but not heat-inactivated papain, activated ILC2s in WT mice but not IL-33-deficient mice, indicating that the protease activity of papain likely caused epithelial cell damage and IL-33 release, which in turn activated ILC2s. Indeed, intranasal administration of IL-33 directly stimulated ILC2s to produce IL-13, and coadministration of OVA and IL-33 promoted OVA-specific OT-II T cell differentiation into the Th2 cell pathway. These results suggested that any antigens that cause airway epithelial cell damage and/or activation and induce IL-33 release, and subsequent activation of ILC2s, could be potential allergens. Thus, the cascade of cell activation and cytokine production, initiated by airway epithelial IL-33 release, IL-13 production by ILC2s and downstream Th2 cell differentiation, type 2 cytokine production and IgE production is likely a common pathway of allergic lung inflammation in response to a broad range of allergens. Indeed, we also observed reduced Th2 cell differentiation in responses to both HDM extract and Aspergillus sp. protease allergens in the absence of ILC2s. In summary, this study has revealed a critical role of ILC2s in the differentiation of naive CD4+ T cells into Th2 cells in response to protease allergens in the lung, thus providing an important clue to the long-standing question of why airway allergens induce an adaptive Th2 cell response. Our results redraw the map of type 2 immunity, placing ILC2s at the center of a common pathway of the Th2 cell cascade for a range of allergens. As one of the early and critical “domino tiles,” ILC2s likely exert a profound effect on Th2 cell-mediated inflammatory diseases such as asthma. Experimental Procedures Mice C57Bl/6 (B6), B6-Tg(TcraTcrb)425Cbn/J (OT-II), B6.Pep3b, and B6.Il33 −/− (KOMP) mice were maintained in the BCCRC animal facility, and B6.Il13 egfp/egfp were maintained in the MRC ARES animal facility, under SPF conditions. B6.Il4 tm1Nnt/J, B6.129S7-Rag1 tm1Mom/J and B6.Cg-Rora sg/J mice were purchased from the Jackson Laboratories. B6.Rag2 −/− Il2rg −/− mice were purchased from Taconic Farms. Mice were used at 4–8 weeks of age. All animal use was approved by the animal care committee of the University of British Columbia in accordance with the guidelines of the Canadian Council on Animal Care or the UK Home Office. Bone Marrow Transplantation B6.Rag2 −/− Il2rg −/− or B6.Pep3b mice were lethally irradiated (10 Gy), followed by intravenous transplantation of 107 whole bone-marrow cells from 3- to 4-week-old mice. Mice were given ciprofloxacin and HCl in drinking water for 4 weeks, and used for analysis at 8–16 weeks posttransplant. Primary Leukocyte Preparation Cell suspensions were prepared from the lungs, spleens, LNs, or BM as previously described (Veinotte et al., 2008). Intracellular Staining Intracellular staining for GATA3 was performed with the Foxp3 intracellular staining kit (eBioscience) according to the manufacturer’s protocol. Intracellular staining for IL-4, IL-5, IL-13, and IFN-γ was performed with the Cytofix/Cytoperm kit (BD Biosciences) after 3 hr restimulation of 2 × 106 total live nucleated cells in 500 μl RPMI-1640 media containing 10% FBS, Penicillin/Streptomycin (P+S), 2-mercaptoethanol (2-ME), Brefeldin A (GolgiPlug, BD Biosciences) or eBioscience protein transport inhibitor cocktail (for intracellular IL-4 detection), PMA (30 ng/ml), and ionomycin (500 ng/ml) at 37°C. Dead cells were excluded with eFluor® 450 or eFluor® 780 (eBioscience) fixable viability dye. Isolation of ILC2 Single cells were incubated with 2.4G2 to block Fc receptors and then stained with eFluor® 450-conjugated lineage marker mAbs (CD3ε, CD19, B220, NK1.1, Mac-1, GR-1, and Ter119), APC-eFluor® 780-conjugated B220, PE-conjugated CD127, PerCP-Cy5.5-conjugated CD25, PE.Cy7-conjugated Sca-1, and APC-conjugated CD117, V500-conjugated CD45, FITC-conjugated T1/ST2, PI viability dye, and purified by FACS. Lung Explant Cultures Lung explants were made by injecting mouse lungs with 2% low melting point agarose (in RPMI-1640, kept at 37°C) via intratracheal injection. Lungs were allowed to cool, after which they were dissected. Explants of 300 μm thickness were made using a vibratome (Leica). Explants were cultured in 5.0 μm pore-size hanging-cell-culture inserts (Millipore) in RPMI-1640 media (10% FCS, P+S, 2 ME). Papain (5 μg/ml), anti-IL13 (0.5 μg/ml), rIL-13 (10 ng/ml), EP4-agonist (5 μM), or EP4-antagonist (5 μM) was added to the media. CCL21 or rmIL-13 (100 ng/ml) was added to the bottom compartment of the trans-well culture. Explants were cultured at 37°C for 14 hr. All contents of the trans-well inserts (including explants) were harvested and made to single-cell suspension, followed by Percoll purification of cells. All migrated cells in the bottom compartment were harvested. Cells were FcR-blocked and stained with PI, anti-CD11c, MHCII, B220, and CD45, followed by analysis by flow cytometry for DCs. Total number of cells was calculated with CountBright beads (Invitrogen). The percent of migrated DCs in each culture was calculated. In Vivo Stimulation Mice were anesthetized by isofluorane inhalation, followed by the intranasal administration of rmIL-13 (1 μg), rmIL-33 (0.5 μg), OVA (50 μg), DQ-OVA (50 μg), house dust mite extract (100 μg), Aspergillus oryzae protease allergen (10 μg), papain, or heat-inactivated papain (10 μg) in 40 μl of PBS. Cultured ILC2s were adoptively transplanted (105 cells) on days 0 and 1 by tail vein injection. Mice were sacrificed at indicated times, and spleens, pLNs, lungs, mLNs, and BAL (1 ml PBS) were collected or airways were instilled with 50:50 Tissue-Tek® O.C.T. Compound (Adwin Scientific) and PBS and fixed in formalin. OT-II Adoptive Transplant OT-II cells were purified by CD4+ negative selection (StemCell Technologies) from OT-II mouse spleen. CD4+ OT-II cells were counted and labeled with CFSE (Invitrogen). On day 0, recipient mice were injected with 1 × 106 CFSE labeled OT-II cells by tail vein injection. Statistics Data were analyzed with GraphPad Prism 6 (GraphPad Software). A Student’s t test was used to determine statistical significance between two groups, and ANOVA was performed for multivariable analysis, with p ≤ 0.05 being considered significant. Author Contributions T.Y.F.H. designed and performed the experiments and wrote the paper. I.M.G., C.A.S., and L.M. performed the experiments. M.J.G. designed and performed the experiments. A.N.J.M. and K.M.M. designed experiments and reviewed the paper. F.T. supervised the project, designed the experiments, and wrote the paper. C.A.S. and L.M. contributed equally to this work.
Author and article information
Journal
Journal ID (nlm-ta): J Exp Med
Journal ID (iso-abbrev): J. Exp. Med
Journal ID (publisher-id): jem
Journal ID (hwp): jem
Title:
The Journal of Experimental Medicine
Publisher:
The Rockefeller University Press
ISSN
(Print):
0022-1007
ISSN
(Electronic):
1540-9538
Publication date
(Print):
05
June
2017
Volume: 214
Issue: 6
Pages: 1581-1592
Affiliations
[1
]Centre de Physiopathologie de Toulouse Purpan (CPTP), Université de Toulouse, Institut
National de la Santé et de la Recherche Medicale (INSERM), Centre National de la Recherche
Scientifique (CNRS), UPS, 31300 Toulouse, France
[2
]Department of Functional Genomics and Cancer, Institut de Génétique et de Biologie
Moléculaire et Cellulaire (IGBMC), INSERM U964, CNRS UMR 7104, Université de Strasbourg,
67404 Illkirch, France
[3
]Institut de Pharmacologie et de Biologie Structurale (IPBS), Université de Toulouse,
CNRS, UPS, 31077 Toulouse, France
Author notes
Correspondence to Jean-Charles Guéry:
Jean-Charles.Guery@
123456inserm.fr
; or Cyril Seillet:
seillet@
123456wehi.edu.au
Author information
Claire Cénac
http://orcid.org/0000-0001-6641-7851
Gilles Laverny
http://orcid.org/0000-0002-2666-6877
Daniel Metzger
http://orcid.org/0000-0002-5555-046X
Gabrielle T. Belz
http://orcid.org/0000-0002-9660-9587
Lucette Pelletier
http://orcid.org/0000-0001-5505-109X
Cyril Seillet
http://orcid.org/0000-0002-0941-8679
Jean-Charles Guéry
http://orcid.org/0000-0003-4499-3270
Article
Publisher ID: 20161807DOI: 10.1084/jem.20161807
PMC ID: 5461006
PubMed ID: 28484078
SO-VID: f7fc983e-ec5f-4d80-9fc8-52c8ff2c4cbe
Copyright © © 2017 Laffont et al.
License:
This article is distributed under the terms of an Attribution–Noncommercial–Share Alike–No Mirror Sites license for the first six months after the publication date (see http://www.rupress.org/terms/). After six months it is available under a Creative Commons License (Attribution–Noncommercial–Share Alike 4.0 International license, as described at https://creativecommons.org/licenses/by-nc-sa/4.0/).
History
Date
received
: 26
October
2016
Date
revision received
: 23
February
2017
Date
accepted
: 31
March
2017
Funding
Funded by: Conseil Régional Midi-Pyrénées
Funded by: Fondation pour la Recherche Médicale, DOI http://dx.doi.org/10.13039/501100002915;
Award ID: DEQ2000329169
Funded by: National Health and Medical Research Council, DOI http://dx.doi.org/10.13039/501100000925;
Funded by: Victorian State Government, DOI http://dx.doi.org/10.13039/501100004752;
Funded by: Centre National de la Recherche Scientifique, DOI http://dx.doi.org/10.13039/501100004794;
Funded by: Institut National de la Santé et de la Recherche Médicale, DOI http://dx.doi.org/10.13039/501100001677;
Funded by: Université de Strasbourg, DOI http://dx.doi.org/10.13039/501100003768;
Funded by: Agence Nationale de la Recherche, DOI http://dx.doi.org/10.13039/501100001665;
Award ID: ANR-10-1108-01 Androgluco
Award ID: ANR-10-LABX-0030-INRT
Award ID: ANR-10-IDEX-0002-02
Categories
Subject:
Research Articles
Subject:
Brief Definitive Report
Subject:
311
ScienceOpen disciplines: Medicine
Data availability:
ScienceOpen disciplines: Medicine