Group 2 innate lymphoid cells (ILC2s) promote type 2 cytokine-dependent immunity, inflammation, and tissue repair. Although epithelial cell-derived cytokines regulate ILC2 effector functions, the pathways that control the in vivo migration of ILC2s into inflamed tissues remain poorly understood. Here, we provide the first demonstration that expression of the prostaglandin D2 (PGD2) receptor CRTH2 (chemoattractant receptor-homologous molecule expressed on Th2 cells) regulates the in vivo accumulation of ILC2s in the lung. Although a significant proportion of ILC2s isolated from healthy human peripheral blood expressed CRTH2, a smaller proportion of ILC2s isolated from nondiseased human lung expressed CRTH2, suggesting that dynamic regulation of CRTH2 expression might be associated with the migration of ILC2s into tissues. Consistent with this, murine ILC2s expressed CRTH2, migrated toward PGD2 in vitro, and accumulated in the lung in response to PGD2 in vivo. Furthermore, mice deficient in CRTH2 exhibited reduced ILC2 responses and inflammation in a murine model of helminth-induced pulmonary type 2 inflammation. Critically, adoptive transfer of CRTH2-sufficient ILC2s restored pulmonary inflammation in CRTH2-deficient mice. Together, these data identify a role for the PGD2–CRTH2 pathway in regulating the in vivo accumulation of ILC2s and the development of type 2 inflammation in the lung.
Group 2 innate lymphoid cells (ILC2s) are innate immune cells found in multiple tissues of humans and mice that can promote expulsion of helminth parasites, allergic inflammation, tissue repair, and metabolic homeostasis.1, 2, 3 ILC2s in the lung, skin, and gut are activated by the predominantly epithelial cell-derived cytokines interleukin (IL)-25, IL-33, and thymic stromal lymphopoietin to produce T helper type 2 (Th2)-associated cytokines such as IL-5, IL-9, and IL-13 and the growth factor amphiregulin.1, 3, 4, 5, 6, 7 Despite advances in our understanding of the factors that control the development, activation, and effector function of ILC2s, the pathways that regulate their migration into inflamed tissues remain poorly characterized.
In humans, ILC2s have been identified in the peripheral blood, lung, gut, skin, and nasal polyps as lineage marker-negative (lin−) cells that express the IL-7 receptor-α (IL-7Rα) (CD127) and the IL-33R.1, 3, 4, 5, 6, 7, 8 A proportion of human ILC2s also express the prostaglandin D2 (PGD2) receptor chemoattractant receptor-homologous molecule expressed on Th2 cells (CRTH2).8, 9, 10 In Th2 cells, eosinophils, basophils, and mast cells, PGD2 ligation of CRTH2 causes receptor internalization and downregulation and promotes migration of cells.11, 12, 13 However, although human CRTH2+ ILC2s migrate and produce IL-13 in response to PGD2 in vitro,14, 15, 16 the influence of the PGD2–CRTH2 pathway on the in vivo activation, accumulation, and/or effector function of human or murine ILC2s is unknown.
In this report we provide the first demonstration that the PGD2–CRTH2 pathway promotes the in vivo accumulation of ILC2s in the lung in the context of type 2 inflammation. Although a significant proportion of ILC2s in the blood of previously healthy adult human organ donors were CRTH2+, a smaller proportion of ILC2s isolated from lung tissue expressed CRTH2, suggesting that the tissue localization of ILC2s and CRTH2 expression may be linked. Consistent with this, the PGD2–CRTH2 pathway promoted the in vitro migration of murine ILC2s and their in vivo accumulation in lung tissue. Furthermore, employing a murine model of helminth-induced type 2 pulmonary inflammation, we identify a previously unrecognized role for ILC2-intrinsic expression of CRTH2 in mediating the accumulation of ILC2s in the inflamed lung. Collectively, these findings identify that expression of CRTH2 on ILC2s has a critical role in promoting their accumulation in vivo and the development of type 2 inflammation in the lung.
Tissue-specific expression of CRTH2 by human ILC2s
To begin to investigate whether the PGD2–CRTH2 pathway might be associated with ILC2 responses or accumulation in tissues in vivo, we first compared CRTH2 expression on human ILC2s isolated from the peripheral blood vs. lung parenchyma from previously healthy deceased adult organ donors at the time of organ procurement for transplantation. ILC2s were identified using flow cytometry as negative for expression of known cell lineage markers and positive for expression of CD127 and the IL-33R (Figure 1a,b; see Supplementary Figure S1a,b online for staining controls).8, 17 Consistent with previous studies,8 a significant proportion of ILC2s in peripheral blood mononuclear cells (PBMCs) were CRTH2+ (Figure 1a,c). In contrast, a lower frequency of ILC2s in the lung was CRTH2+ when CRTH2 expression by ILC2s in the PBMCs and lung parenchyma from the same deceased adult organ donor were compared (Figure 1b,c). Given that PGD2 ligation results in the downregulation of CRTH2 on immune cells,15, 18 these data suggest that CRTH2-expressing ILC2s in the peripheral blood may encounter PGD2 and downregulate surface CRTH2 expression, associated with their accumulation in the lung.
Murine ILC2s express CRTH2 and accumulate in the lung in vivo in response to PGD2
To experimentally test the role of the PGD2–CRTH2 pathway in regulating ILC2 responses and accumulation in the lung in vivo, we first sought to characterize expression of CRTH2 on murine ILC2s. As there is currently no antibody available to detect murine CRTH2, expression of CRTH2 on murine ILC2s has not been reported previously. Therefore, we employed single-cell RNA transcript staining for Gpr44 (the gene encoding CRTH2) and flow cytometry to assess CRTH2 expression on murine ILC2s from the peripheral blood and lung. Murine ILC2s isolated from PBMCs (see Supplementary Figure S2a for staining controls) expressed Gpr44 (Figure 2a). Similar to results observed when examining human ILC2s (Figure 1), murine ILC2s isolated from the lung (see Supplementary Figure S2b for staining controls) expressed very low levels of Gpr44 compared with those in the peripheral blood (Figure 2b), although nonquantitative reverse transcriptase-PCR for Gpr44 on sort-purified murine lung ILC2s confirmed that ILC2s isolated from the murine lung do indeed express this transcript (Figure 2c). These data suggest that expression of CRTH2 and tissue-specific regulation of CRTH2 expression patterns are conserved in human and murine ILC2s.
Previous in vitro studies demonstrated that the PGD2–CRTH2 pathway promotes cytokine production from human ILC2s,14, 15, 16 provoking the hypothesis that CRTH2 expression by murine ILC2s may also be associated with cytokine production in response to PGD2. Following culture of sort-purified murine lung ILC2s with recombinant murine (rm) IL-25, IL-33, and/or PGD2, rmIL-33 exposure induced robust IL-5, IL-9, and IL-13 production, and rm-IL-25 exposure induced robust IL-5 and IL-13 production from ILC2s (Supplementary Figure S3a,b). However, PGD2 alone did not elicit cytokine production from murine lung ILC2s and did not significantly augment cytokine production elicited by IL-25 or IL-33 (Supplementary Figure S3a,b). These observations suggest that PGD2 does not elicit production of effector cytokines from murine lung ILC2s, consistent with their low expression of CRTH2.
The PGD2–CRTH2 pathway has also been shown to promote chemotaxis of human ILC2s,14, 15 suggesting that CRTH2-expressing murine ILC2s may migrate in vitro or accumulate in tissues in vivo in response to PGD2. Using an in vitro chemotaxis assay, we observed that sort-purified murine lung ILC2s exhibited limited migration to increasing doses of PGD2 (Figure 2d). In contrast, murine ILC2s isolated from the spleen migrated toward PGD2 more robustly (Figure 2d), and linear regression of the dose–response curves of spleen-derived compared with lung-derived ILC2s to PGD2 resulted in statistically different best-fit lines (Supplementary Figure S4). These data are consistent with the hypothesis that ILC2s in the periphery could respond to PGD2 to accumulate in the lung. To directly test whether PGD2 signaling through CRTH2 promotes accumulation of ILC2s in the lung in vivo, wild-type (WT) mice and mice deficient in CRTH2 (Gpr44−/− mice) were treated intranasally for 3 days with PGD2. Following PGD2 treatment, ILC2s accumulated in the lungs of WT but not Gpr44−/− mice (Figure 2e). Together, these data provide the first in vivo evidence of a role for the PGD2–CRTH2 pathway in regulating the migration and/or accumulation of ILC2s in the lung.
Accumulation of ILC2s and type 2 inflammation in the murine lung are dependent on CRTH2
The data shown above, in conjunction with studies showing that ILC2-derived Th2 cytokine-associated responses can contribute to allergic airway inflammation and chronic pulmonary inflammation,3, 7, 10, 19, 20, 21 support the hypothesis that CRTH2 expression may regulate ILC2 accumulation in the context of type 2 cytokine-associated inflammation in the lung. To test this, we employed a murine model of helminth-induced pulmonary type 2 inflammation.22, 23, 24, 25 In this model, larvae of the gastrointestinal nematode Nippostrongylus brasiliensis migrate through the lung of mice and elicit severe, pulmonary type 2 inflammation, associated with infiltration of CD4+ T cells and alternatively activated macrophages and the development of emphysema that persists long after all helminths are expelled from the intestine.22, 23, 24, 25 Following infection with N. brasiliensis, WT and Gpr44−/− mice had similar numbers of larvae in the lung 50 h post infection (p.i.) (Supplementary Figure S5a), and both WT and Gpr44−/− mice efficiently cleared parasites from the small intestine by day 10 p.i. (Supplementary Figure S5b), suggesting that CRTH2 deficiency does not significantly impact the lifecycle of N. brasiliensis at these time points in the murine host.
However, when helminth-induced accumulation of ILC2s in the inflamed lung was examined at day 32 p.i. in WT and Gpr44−/− mice, we observed a helminth-induced increase in the total number of ILC2s in the lung of WT mice but not Gpr44−/− mice, as determined using flow cytometry (Figure 3a). In addition, WT mice exhibited severe histopathological changes (Figure 3b,c), extensive goblet cell hyperplasia (Figure 3d), increased expression of genes associated with type 2 inflammation (Il4 and Il13) (Figure 3e), an increase in the total number of infiltrating cells (Supplementary Figure S6a), and an increase in the total number of CD4+ T cells (Figure 3f) and CD11b+CD11cint macrophages (Figure 3g) in the lung parenchyma. Remarkably, these responses were significantly diminished in Gpr44−/− mice (Figure 3b–g and Supplementary Figure S6a). Notably, the decreased expression of Il4 and Il13 in Gpr44−/− mice compared with WT mice was not accompanied by changes in expression of IL-17A (Supplementary Figure S6b), and levels of interferon-γ could not be detected in any naive or infected animals (data not shown). In addition, in agreement with previous findings,26 expression of Il5 was not altered in Gpr44−/− mice (Supplementary Figure S6c). These analyses suggest that CRTH2 deficiency does not promote the development of a type 1 or type 17 cytokine milieu in the lung following N. brasiliensis infection, but rather selectively regulates expression of specific type 2 cytokines. Together, these data indicate that genetic deletion of CRTH2 is associated with reduced accumulation of ILC2s, less severe pathological changes, and decreased expression of Il4 and Il13 and immune cell infiltrate in the lung following N. brasiliensis infection.
A CRTH2-specific inhibitor limits accumulation of ILC2s and type 2 inflammation in the murine lung following helminth infection
Small-molecule inhibitors of CRTH2 have recently been developed,27 and studies are ongoing to determine whether these drugs could be used to treat allergic disease in humans.27, 28, 29 To complement our studies of mice genetically deficient in Gpr44, we sought to determine whether chemical inhibition of CRTH2 using the CRTH2-specific inhibitor OC000459 could also limit helminth-induced accumulation of ILC2s and type 2 inflammation in the lung. Mice infected with N. brasiliensis were treated daily with 1 mg kg−1 OC000459 (ref. 28) or vehicle, starting 2 days before infection, and examined at day 32 p.i. Consistent with our observations in Gpr44−/− mice, mice treated with OC000459 had lower total numbers of ILC2s in the lung following infection than control mice treated with vehicle (Figure 4a). In addition, OC000459-treated mice exhibited less severe helminth-induced histopathological changes (Figure 4b,c), decreased expression of Il4 and Il13 (Figure 4e), and significantly decreased total numbers of CD4+ T cells (Figure 4f) and CD11b+CD11cint macrophages (Figure 4g) in the lung following N. brasiliensis infection compared with vehicle-treated control mice. Interestingly, OC000459-treated mice and vehicle-treated controls demonstrated similar goblet cell hyperplasia in the lung following infection (Figure 4d). These data suggest that chemical inhibition of CRTH2, similar to genetic deletion of Gpr44, results in reduced accumulation of ILC2s, pathological changes, expression of Il4 and Il13, and immune cell infiltrate in the lung following N. brasiliensis infection.
Hematopoietic cell expression of CRTH2 is required for accumulation of ILC2s and type 2 inflammation in the murine lung
Although CRTH2 expression is enriched in inflammatory cells, nonhematopoietic cells have also been reported to express CRTH2.11, 30, 31 To assess the role of hematopoietic cell-intrinsic expression of CRTH2 in promoting ILC2 responses and pulmonary inflammation, lethally irradiated WT mice were reconstituted with congenic WT or Gpr44−/− bone marrow (BM) and subjected to the N. brasiliensis-induced model of pulmonary type 2 inflammation. WT hosts reconstituted with WT BM (WT-WT BM mice) exhibited significantly increased total numbers of ILC2s (Figure 5a), helminth-induced histopathological changes (Figure 5b,c), goblet cell hyperplasia (Figure 5d), significantly increased expression of Il4 and Il13 (Figure 5e), and significantly increased total numbers of CD11b+CD11cint macrophages (Figure 5g) in the lung. In contrast, all of these parameters were reduced in WT hosts reconstituted with Gpr44−/− BM (WT-KO BM mice) (Figure 5a–e,g). Notably, WT-WT BM and WT-KO BM mice had similar total numbers of CD4+ T cells in the lung following N. brasiliensis infection (Figure 5f), suggesting that elevated numbers of CD4+ T cells alone do not result in histopathological changes in the lung. These data indicate that hematopoietic CRTH2 expression mediates parameters of helminth-induced pulmonary inflammation in mice.
CRTH2 expression on murine ILC2s promotes their preferential accumulation in the lung and associated type 2 pulmonary inflammation
Next, we assessed the role of ILC2-intrisic CRTH2 expression in regulating the accumulation of ILC2s in the lung by employing mixed BM chimeras in which 50% of donor cells were WT and 50% of donor cells were Gpr44−/− (WT-50/50 mice). Following induction of the N. brasiliensis-induced model of type 2 inflammation in the lung, the majority of ILC2s present in the lung of infected chimeras were of WT origin (Figure 5h,i), suggesting that ILC2-intrinsic CRTH2 expression is required for efficient accumulation of ILC2s in the lung in a competitive environment. Finally, to test whether CRTH2 expression on ILC2s is sufficient to promote pulmonary inflammation, Gpr44-sufficient ILC2s were sort-purified from CD45.1+ WT mice (Figure 6a; see Supplementary Figure S7 for staining controls) and adoptively transferred once weekly into congenic CD45.2+ Gpr44−/− mice subjected to the N. brasiliensis-induced model of type 2 pulmonary inflammation. At day 32 p.i., congenic donor-derived ILC2s could be detected in the lung, retained expression of CD127 and the IL-33R, and were capable of producing IL-13 (Figure 6b). These donor-derived ILC2s constituted ∼5% of the total ILC2 population in the lung of the recipient mice (Supplementary Figure S8). Despite this relatively low frequency, Gpr44−/− mice that received these WT ILC2s exhibited increased helminth-induced histopathological changes (Figure 6c,d), increased goblet cell hyperplasia (Figure 6e), elevated expression of Il4 and Il13 (Figure 6f), and significantly increased total numbers of CD4+ T cells (Figure 6g) and CD11b+CD11cint macrophages (Figure 6h) in the lung parenchyma compared with Gpr44−/− mice that did not receive WT ILC2s. Collectively, these data provide evidence that ILC2-intrinsic CRTH2 regulates the accumulation of murine ILC2s in the lung that is associated with histopathological changes, expression of specific type 2 cytokines, and infiltration of immune cells.
Previous studies have reported that ILC2s play a critical role in promoting Th2 cytokine-associated inflammation or tissue repair in the lung,1, 3, 7, 17, 19, 20, 21 but the factors that influence the in vivo migration and accumulation of ILC2s in the lung and other tissues are poorly characterized. By assessing differential expression of CRTH2 by human ILC2s isolated from distinct anatomical compartments, we observed tissue-specific surface expression of CRTH2 that may be associated with ILC2 accumulation in the lung. Studies employing a murine model of type 2 pulmonary inflammation showed that the PGD2–CRTH2 pathway functions in vivo to regulate the accumulation of ILC2s in the murine lung and the development of associated type 2 inflammation. Together, these findings identify a previously unappreciated role for the PGD2–CRTH2 pathway in regulating the in vivo accumulation of ILC2s that supports type 2 cytokine-associated inflammation in the lung.
The observation that there is differential expression of CRTH2 by ILC2s isolated from human or murine peripheral blood and lung could also mean that lung tissue-resident ILC2s and circulating peripheral ILC2s are in fact distinct populations. Additional work is required to carefully dissect how the ILC2 population in the lung is regulated, particularly regarding whether the population expands during inflammation via migration of new cells into the tissue or by proliferation of tissue-resident cells. Regardless, our data may indicate that there could be heterogeneity within the ILC2 population that might be determined by anatomical location or following exposure to activating factors. Notably, our data showing that only a small proportion of CRTH2-sufficient ILC2s are needed to drive helminth-induced type 2 inflammation in the lung in CRTH2-deficient mice suggest that this heterogeneity may have profound functional consequences.
Notably, Gpr44−/− mice do not display defects in the population size of ILC2s in the lung in the steady state, suggesting that although CRTH2-dependent pathways promote accumulation of ILC2s in the lung in the context of inflammation, the seeding of ILC2s in the lung during development and in the steady state does not require CRTH2. These findings indicate that other pathways, including selective expression of chemokine receptors or adhesion molecules, may regulate the recruitment and retention of ILC2s in tissues during development, the steady state, and ongoing inflammation. Further studies will be required to delineate how CRTH2-dependent and -independent pathways differentially regulate the migration of ILC2s in tissues in the context of health and multiple disease states.
ILC2s can interact with a variety of innate and adaptive cell types to orchestrate inflammation.1, 3, 7, 32 In particular, recent work has focused on the role of ILC2s in supporting CD4+ T-cell function and accumulation.33, 34, 35, 36 Our data demonstrating that N. brasiliensis-induced pulmonary accumulation of CD4+ T cells is dependent on CRTH2-expressing ILC2s (Figure 6g) support these findings. Interestingly however, our studies of chimeric mice show that CD4+ T-cell accumulation in the lung following N. brasiliensis infection is not dependent on hematopoietic expression of CRTH2 (Figure 5f). Together, these data suggest that the accumulation of CD4+ T cells in this model may be dependent on CRTH2 expression by both ILC2s and nonhematopoietic cells. Alternatively, reconstituted CD4+ T cells in radiation chimeras may be more readily activated than those in normal mice, allowing them to overcome the requirement for CRTH2-expressing ILC2s in mediating their accumulation in the lung. Further studies will be required to understand the complex mechanisms that control CD4+ T-cell population size in the lung following N. brasiliensis infection.
As the accumulation of ILC2s associated with the development of type 2 inflammation in the lung was CRTH2 dependent using genetic deletion of Gpr44 and chemical inhibition of CRTH2, our studies also support the concept that the PGD2–CRTH2 pathway may be a viable drug target for the treatment of multiple chronic inflammatory diseases of the airways that are associated with ILC2 responses including allergic rhinitis, asthma, and chronic obstructive pulmonary disease.3, 13, 27, 28, 29 A number of inhibitors of CRTH2 have already been tested in the treatment of various disease states. Although some studies reported that inhibition of CRTH2 was unsuccessful in ameliorating symptoms of chronic obstructive pulmonary disease or asthma and allergic rhinitis in patients,31, 37, 38 other clinical trials targeting CRTH2 have shown promising efficacy data in the treatment of asthma and allergic rhinitis.28, 39, 40 Notably, our results showed that chemical inhibition of CRTH2 ameliorated some, but not all, effects of helminth infection in the lung, as OC000459 treatment did not appear to decrease helminth-induced pulmonary goblet cell hyperplasia. Thus, further trials that include clinically stratified patient cohorts based on disease activity and assessment of multiple parameters of disease may be required to determine whether CRTH2 is an appropriate target to treat inflammatory diseases in the lung. Notwithstanding this, our findings are the first to describe a mechanism by which ILC2s accumulate in the lung during inflammation and suggest that the PGD2–CRTH2–ILC2 pathway could be targeted to treat inflammatory disease states that are associated with CRTH2-expressing ILC2s.
PBMCs and lung tissue were obtained from deceased adult organ donors at the time of organ procurement for transplantation through the New York Organ Donor Network (NYODN). All NYODN subjects were ≤65 years of age, free of chronic infections and cancer, and HIV− and HBV/HCV−. As donors were deceased at the time of tissue collection, this work does not qualify as “human subjects” as confirmed by the institutional review board of Columbia University. PBMCs were prepared by separating lymphocytes with a Ficoll-Paque (GE Healthcare, Pittsburgh, PA) gradient and lysing remaining red blood cells (RBCs) with ammonium-chloride-potassium (ACK) buffer (Lonza, Basel, Switzerland). Single-cell suspensions of lung were prepared by incubating the finely chopped tissue for 1 h with 2 mg ml−1 collagenase D (Roche, Indianapolis, IN) and 20 μg ml−1 DNase I (Roche), mashing through a wire mesh sieve and a 70 μm cell strainer, lysing RBCs with ACK buffer (Lonza), and separating lymphocytes with a Ficoll-Paque (GE Healthcare) gradient. For flow cytometric analysis, matched PBMCs and lung from the same deceased adult organ donor were compared.
Male and female C57BL/6 WT, Thy1.1 C57BL/6, and CD45.1 C57BL/6 mice were purchased from the Jackson Laboratories (Bar Harbor, ME). Gpr44−/− mice were provided by Amgen (Seattle, WA). All mice were used at 8–12 weeks of age, and all experiments used age- and sex-matched controls. All animals were housed in specific pathogen-free conditions at the University of Pennsylvania (Philadelphia, PA) or Weill Cornell Medical College (New York, NY). WT and Gpr44−/− female mice were cohoused, and WT and Gpr44−/− male mice shared soiled bedding. All experiments were performed under protocols approved by the University of Pennsylvania or Weill Cornell Medical College Institutional Animal Care and Use Committees.
PBMCs were prepared by separating lymphocytes with a Ficoll-Paque (GE Healthcare) gradient and lysing remaining RBCs with ACK buffer (Lonza). Single-cell suspensions of murine spleen were prepared by mashing through a 70 μm cell strainer and lysing RBCs with ACK buffer (Lonza). Single-cell suspensions of perfused murine lung tissue (right superior lobe) were prepared by incubating finely chopped tissue for 30 min with 2 mg ml−1 collagenase D (Roche) and 20 μg ml−1 DNase I (Roche), mashing through a 70 μm cell strainer, lysing RBCs with ACK buffer (Lonza), and counting total cells.
Type 2 pulmonary inflammation
The N. brasiliensis life cycle was maintained as previously described.41 Mice were infected with 500 L3 N. brasiliensis larvae subcutaneously, and analyses were performed at day 32 p.i. Lung larvae were quantified at 50 h p.i. by allowing viable larvae to migrate through agarose in a 37 °C water bath, and adult worms in the small intestine were quantified directly from intestinal tissues on day 10 p.i., as described previously.41 Serum antibody titers for N. brasiliensis-specific IgG1 were quantified by enzyme-linked immunosorbent assay (ELISA) as previously described,42 and any animals that lacked specific IgG1 were omitted. Mice were treated intranasally with 2.5 mg kg−1 PGD2 (Cayman Chemical, Ann Arbor, MI) dissolved in 50 μl 1:10 dimethyl sulfoxide in phosphate-buffered saline43 for 3 days. Untreated mice were treated intranasally with 50 μl vehicle (dimethyl sulfoxide) as a control, diluted 1:10 in phosphate-buffered saline. Mice were treated intraperitoneally (i.p.) once daily with 1 mg kg−1 of the CRTH2-specific inhibitor OC000459 (Cayman Chemical) dissolved in 1:100 dimethyl sulfoxide in phosphate-buffered saline, starting 2 days before infection with N. brasiliensis and until analysis at day 32 p.i. Untreated mice were injected i.p. with vehicle (dimethyl sulfoxide) as a control, diluted 1:100 in phosphate-buffered saline.
Flow cytometry, single-cell RNA transcript staining, and cell sorting
Single-cell suspensions were incubated with Aqua Live/Dead Fixable Dye (Life Technologies, Grand Island, NY) and fluorochrome-conjugated monoclonal antibodies (mAbs) against mouse CD3 (145-2C11), CD4 (GK1.5), CD5 (53-7.3), CD11b (M1/70), CD11c (N418), CD19 (eBio1D3), CD25 (PC61.5), CD45 (30-F11), CD45.1 (A20), CD45.2 (104), CD127 (A7R34), CD90.1 (HIS51), CD90.2 (53-2.1), IL-33R (DJ8, MD Bioproducts, St Paul, MN), NK1.1 (PK136), or Siglec-F (E50-2440, BD Biosciences, San Jose, CA), or fluorochrome-conjugated mAbs against human CD3 (OKT3), CD4 (OKT4), CD5 (UCHT2), CD14 (61D3), CD16 (CB16), CD19 (HIB19), CD56 (B159), CD25 (BC96), CD45 (HI30), CD127 (eBioRDR5), CRTH2 (BM16, BD Biosciences), FcɛR1α (AER-37), or IL-33R (B4E6, MD Bioproducts) (eBioscience, San Diego, CA, unless specified otherwise). For RNA staining analyses, cells were treated according to the manufacturer’s instructions using a commercially available kit (PrimeFlow RNA Assay, eBioscience) and compatible commercially available probes for β2m (used as a positive control for RNA staining) and Gpr44 (eBioscience). For intracellular staining, cells were fixed in 2% paraformaldehyde, permeabilized using BD Perm/Wash buffer (BD Biosciences) according to the manufacturer’s instructions, and stained with fluorochrome-conjugated mAbs against mouse IL-5 (TRFK5), IL-9 (RM9A4), and IL-13 (eBio13A) (eBioscience). ILC2s are gated as live, CD45+lin−CD4−CD90.2+CD25+CD127+IL-33R+ or as live, β2m+lin−CD90.2+CD127+IL-33R+ in RNA staining analyses. Samples were run on a 4-laser LSR II (BD Biosciences), and FlowJo 8.7.1 (Tree Star, Ashland, OR) was used to analyze data. Gates were set using FMO controls with <5% background accepted. Analysis and presentation of intracellular cytokine staining distributions were performed using SPICE version 5.1 (National Institute of Allergy and Infectious Diseases, Bethesda, MD), downloaded from http://exon.niaid.nih.gov.44
For cell sorting, single-cell suspensions were prepared from tissues of female mice that had been treated i.p. for 7 days with 300 ng rmIL-33 (R&D Systems, Minneapolis, MN) or treated 3 times i.p. every other day with 2.5 ng rmIL-7 (R&D Systems) plus 15 μg anti-human IL-7 (M25) (Amgen). For ILC2s, depletions were performed using biotin-conjugated mAbs against mouse CD5 (53-7.3), CD19 (eBio1D3), and CD11b (M1/70) (eBioscience) and M-280 streptavidin Dynabeads (Life Technologies) according to the manufacturer’s instructions. Cells were incubated with Aqua Live/Dead Fixable Dye (Life Technologies) and fluorochrome-conjugated mAbs as indicated. CD45+CD11b+Siglec-F+ eosinophils or CD45+lin−CD4−CD90+CD25+CD127+IL-33R+ ILC2s were sorted using a 4-laser FACSAria II (BD Biosciences) with a 70 μm nozzle.
BM chimeras and cell transfers
Single-cell suspensions from the BM of 8-week-old mice were prepared by flushing the femur and tibia with Dulbecco’s modified Eagle’s medium (Corning, Corning, NY), lysing RBCs with ACK buffer (Lonza), and depleting T cells using a biotin-conjugated mAb against mouse CD5 (53-7.3) (eBioscience) and M-280 streptavidin Dynabeads (Life Technologies) according to the manufacturer’s instructions. Recipients were lethally irradiated with 1,000 CyG using a Nordion Gammacell irradiator (Ottawa, ON, Canada), anesthetized with inhaled isoflurane (Abbott Animal Health, Abbott Park, IL), and given 4 × 106 donor cells intravenously. Sulfamexosone/trimethoprim (Hi-Tech Pharmacal, Amityville, NY) was provided in the drinking water for 2 weeks after reconstitution, and mice were analyzed at 8–12 weeks after reconstitution.
Sorted ILC2s from mice treated with rmIL-33 and cultured in vitro for 3–7 days with rmIL-2 (10 ng ml−1), rmIL-7 (10 ng ml−1), and rmIL-33 (30 ng ml−1) (eBioscience) were transferred every 7 days to mice infected with N. brasiliensis, starting on the day of infection. Mice were anesthetized with inhaled isoflurane (Abbott Animal Health) and given 1–2 × 105 cells transferred intravenously.
Sorted spleen or lung ILC2s from mice treated with rmIL-33 were allowed to rest for 2 h at 37 °C in media. Media with 0–100 nM of PGD2 was placed in the bottom chamber of Costar 6.5 mm, 5.0 μm Transwell 24-well plates (Corning), and 5 × 104 ILC2s were placed in the top chamber. Cells were incubated for 90 min at 37 °C, and the number of cells that had migrated was quantified using CountBrite Absolute Counting Beads (Life Technologies). Counts were normalized as fold increase over media.
In vitro cultures
Sorted lung ILC2s from mice treated with rmIL-33 or mouse IL-7 complexes were cultured for 48 h in media (Dulbecco’s modified Eagle’s medium with 10% fetal bovine serum (Denville Scientific, Metuchen, NJ), 1% L-glutamine (Corning), 1% penicillin/streptomycin (Corning), 25 mM HEPES buffer, and 55 μM 2-β-mercaptoethanol (Sigma-Aldrich, St Louis, MO)) with or without 50 ng ml−1 rmIL-25 (R&D Systems) and/or 30 ng ml−1 rmIL-33 (R&D Systems) and/or 100 nM PGD2. Cell-free supernatants were collected for ELISA, and cells were used for intracellular cytokine staining following 4 h culture with 50 ng ml−1 phorbol 12-myristate 13-acetate (Sigma-Aldrich), 500 ng ml−1 ionomycin (Sigma-Aldrich), and 10 μg ml−1 brefeldin A (Sigma-Aldrich).
ELISA and real-time PCR
Cytokine levels in cell-free supernatants were assessed using standard sandwich ELISA for IL-5 and IL-13 (eBioscience) or using a commercially available ELISA kit for IL-9 (R&D Systems). For real-time PCR, RNA was isolated from lung tissue using an RNeasy Mini Kit (Qiagen, Valencia, CA) or from sort-purified cells using an RNeasy Micro Kit (Qiagen) according to the manufacturer’s instructions. Real-time PCR was performed on complementary DNA generated using a Superscript II reverse transcription kit (Life Technologies) using SYBR green master mix (Applied Biosystems) or Taqman Gene Expression Mastermix (Life Technologies) and commercially available primer sets (Qiagen Quantitect or Life Technologies Taqman primer assays). Samples were run on the ABI 7500 real-time PCR system (Life Technologies). Real-time PCR products were run on a 3% agarose gel and visualized using a Bio-Rad Gel Doc 1000 (Bio-Rad Laboratories, Hercules, CA) and Quantity One software (Bio-Rad Laboratories).
At necropsy, the left lung lobe was inflated with 4% paraformaldehyde administered through tubing inserted through the trachea and stored in 4% paraformaldehyde. Tissues were then paraffin-embedded, and 5 μm sections were stained with hematoxylin and eosin or periodic acid–Schiff/Alcian blue. Image acquisition was performed using a Nikon Eclipse Ti microscope, a Nikon Digital Sight DS-Fi2 camera, and NIS-Elements AT version 4.2 acquisition software (Nikon, Tokyo, Japan). Adobe Photoshop (Adobe Systems Incorporated, San Jose, CA) was used to adjust brightness, contrast, and color balance (changes were applied to the whole image). Blind scoring was performed by a board-certified veterinary pathologist. Scoring reflects emphysema (1–5) and accumulation of macrophages/multinucleated giant cells (1–5), for an overall maximum score of 10.
Results are shown as mean±s.e.m. Linear regression was used to calculate the best-fit line for chemotaxis in response to a dose curve of PGD2. Statistical significance was determined using an unpaired two-tailed Student’s t-test with Welch’s correction if needed, a paired two-tailed Student’s t-test for paired observations, or a one-way analysis of variance test followed by Bonferroni post hoc testing. Statistical outliers were identified in normal Gaussian data sets using the extreme studentized deviate method, and outliers were uniformly omitted. Results were considered significant at *P≤0.05; **P≤0.01; ***P≤0.001. Statistical analyses were performed using Prism version 4.0a (GraphPad Software, San Diego, CA).
We thank members of the Artis laboratory and Dr Garret Fitzgerald for discussions and critical reading of the manuscript. Research in the Artis lab is supported by the NIH (AI061570, AI095608, AI087990, AI074878, AI095466, AI106697, AI102942, and AI097333 to D.A.; T32-AI060516 and F32-AI098365 to E.D.T.W.; T32-AI007532 to L.A.M.; and K08-DK093784 to T.A.), the Burroughs Wellcome Fund Investigator in Pathogenesis of Infectious Disease Award to D.A., the Crohn’s and Colitis Foundation of America to T.A. and D.A., the Irvington Institute Edmond J. Safra Postdoctoral Fellowship of the Cancer Research Institute to L.C.O., and the NIAID Mucosal Immunology Studies Team (MIST) consortium (U01-AI095608). Research in the Farber lab is supported by the NIH (AI106697 to D.L.F. and F31-AG047003 to J.J.T.). We thank the Matthew J. Ryan Veterinary Hospital Pathology Lab and the Abramson Cancer Center Flow Cytometry and Cell Sorting Resource Laboratory (P30-CA016520). We thank Peggy Just, Castle Funatake, and Matt Schifano at eBioscience for reagents, support, and invaluable technical advice.
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