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Allergic asthma is the most common form of asthma, affecting more than 10 million Americans. Although it is clear that mast cells have a key role in the pathogenesis of allergic asthma, the mechanisms by which they regulate airway narrowing in vivo remain to be elucidated. Here we report that mice lacking αvβ6 integrin are protected from exaggerated airway narrowing in a model of allergic asthma. Expression microarrays of the airway epithelium revealed mast cell proteases among the most prominent differentially expressed genes, with expression of mouse mast cell protease 1 (mMCP-1) induced by allergen challenge in WT mice and expression of mMCP-4, -5, and -6 increased at baseline in β6-deficient mice. These findings were most likely explained by loss of TGF-β activation, since the epithelial integrin αvβ6 is a critical activator of latent TGF-β, and in vitro–differentiated mast cells showed TGF-β–dependent expression of mMCP-1 and suppression of mMCP-4 and -6. In vitro, mMCP-1 increased contractility of murine tracheal rings, an effect that depended on intact airway epithelium, whereas mMCP-4 inhibited IL-13–induced epithelial-independent enhancement of contractility. These results suggest that intraepithelial activation of TGF-β by the αvβ6 integrin regulates airway responsiveness by modulating mast cell protease expression and that these proteases and their proteolytic substrates could be novel targets for improved treatment of allergic asthma.
Mast cells are mainly known for their harmful effects during allergic inflammation and contribute to asthma in several ways (1). Mast cell activation induces degranulation and release of a range of inflammatory substances, including proteases, histamine, cytokines, chemokines, and lipid mediators. Proteases are the most conspicuous products of mast cells and mainly consist of chymases, tryptases, and carboxypeptidase A (CPA) (2). Mast cell degranulation is often seen in asthmatic lungs, and various mast cell mediators can be found in bronchoalveolar lavage (BAL) fluid from asthmatic patients. Infiltration of mast cells into the airway smooth muscle cell layer is a prominent feature of allergic asthma (3) and is associated with airway hyperresponsiveness (AHR) (4). Mice lacking functional mast cells are protected in models of asthma in which allergic airway inflammation is induced by administration of OVA without external adjuvant (5, 6). However, the precise mechanisms by which mast cells regulate airway narrowing in vivo remain to be determined.
The αvβ6 integrin is expressed in epithelial cells, where it plays an important role in activating latent TGF-β. Mice lacking this integrin are protected from pulmonary fibrosis (7, 8) and acute lung injury (9) and develop age-related emphysema (10), effects that all appear to be caused by a lack of active TGF-β. TGF-β is an important regulator of immune responses (11–13), but its role in asthma is controversial. TGF-β affects multiple processes involved in matrix remodeling in the lung (e.g., increased matrix production by fibroblasts, epithelial cell apoptosis, epithelial-mesenchymal transition, and modulation of protease secretion) (14–17) and directs the differentiation of Th17 cells, which can enhance allergic responses (11, 18, 19). On the other hand, TGF-β stimulates differentiation of regulatory T cells that can suppress allergic responses (11, 19, 20), and blocking TGF-β signaling specifically in T cells enhances airway hypersensitivity, airway inflammation, and Th2 cytokine production (21). Thus, in different contexts, TGF-β can either facilitate or inhibit allergic asthma.
Here we show that mice lacking the αvβ6 integrin were protected from AHR in a mast cell–dependent model of allergic asthma and demonstrate that this effect could be explained, at least in part, by specific effects of TGF-β on expression of mast cell proteases that either enhance (mMCP-1) or inhibit (mMCP-4) airway narrowing. mMCP-1 appeared to enhance airway smooth muscle contraction through effects on the epithelium, whereas the effect of mMCP-4 persisted in tracheal rings denuded of epithelium.
β6-deficient mice are protected from AHR, but not from lung inflammation, mucus metaplasia, or airway remodeling. β6 KO and WT control mice on the same genetic background (FvB) were sensitized and challenged by intranasal administration of OVA or saline (as a control) using a regimen that was previously reported to depend on mast cells (5, 6). Airway responsiveness to acetylcholine was the same in saline-challenged WT and β6 KO mice, but β6 KO mice were significantly protected from increased AHR after OVA challenge (Figure (Figure1A).1A). In agreement with previous findings, saline-treated β6 KO mice had low-level baseline lung inflammation, but allergen-induced inflammation — detected by differential counting of cells obtained by BAL — did not differ between genotypes, nor did mucus metaplasia or subepithelial fibrosis (Figure (Figure1,1, B–D). There was also no difference in the degree of sensitization, as determined by OVA-specific serum IgE (data not shown).
To elucidate how loss of this epithelial integrin protects from AHR after allergen challenge, we developed a brushing method to specifically sample the airway epithelial microenvironment. This method harvested airway epithelium from central bronchi, and more than 90% of harvested cells were epithelial cells (Figure (Figure2A).2A). As determined by quantitative real-time RT-PCR (qRT-PCR), expression of 2 epithelial-restricted genes, Cdh1 and Foxj1 (encoding E-cadherin and FOXJ1, respectively), was well-represented in whole lung and brush-harvested epithelial samples, whereas 2 nonepithelial genes, Acta2 and Pecam1 (encoding α-SMA and PECAM-1, respectively), were largely absent only in airway brushing samples (Figure (Figure2C),2C), which confirmed that the samples obtained were highly enriched for airway epithelium.
Expression microarrays identified 119 genes that were significantly differentially expressed in WT and β6 KO mice after saline or chronic allergen challenge (adjusted P < 0.05; Figure Figure3A).3A). Partitioning around mediods (PAM) clustering of the array data revealed 2 interesting clusters (referred to herein as clusters 1 and 2; Figure Figure3,3, B and C) that we had not identified in previous comparisons of whole lung microarrays. Cluster 1 consisted of 6 genes that were increased in saline-treated β6 KO mice; 5 of these encode mast cell proteases (Cma1, encoding mMCP-5; Mcpt4, encoding mMCP-4; Cpa3, encoding CPA3; Mcpt6, encoding mMCP-6; and Tpsab1, encoding mMCP-7), and the sixth, Il1rl1 (encoding IL-33 receptor), is highly expressed in mast cells (22). These 6 transcripts were each among the most highly induced transcripts in saline-treated β6 KO mice compared with WT mice (Supplemental Table 1; supplemental material available online with this article; doi: 10.1172/JCI58815DS1). The 11 genes of cluster 2 (St6galnac2, Hs6st2, Fancd2, Spdef, Cd177, Flt3l, Mcpt1, Qscn6l1, Wnt5b, Itgae, and Mgam) exhibited low expression at baseline in both WT and β6 KO mice and increased in WT mice, but not β6 KO mice, after chronic allergen challenge. The most highly induced gene in this cluster, Mcpt1, encodes another mast cell protease, mMCP-1, which was induced 18-fold in WT mice after allergen challenge, whereas none of the other genes were induced more than 2.5-fold. We also analyzed the most highly induced genes in WT mice after allergen challenge; of these, only Mcpt1 was expressed at a significantly higher level in WT mice than in β6 KO mice (adjusted P < 0.05; Supplemental Table 2).
Thus, the most informative differentially expressed genes identified in microarrays of the epithelial microenvironment were not epithelial genes, but mast cell genes. We also could not find any substantial differential expression of cytokines, chemokines, or growth factors. To confirm these microarray findings of altered mast cell gene expression in brush-harvested airway epithelium, we reanalyzed samples by qRT-PCR (Figure (Figure4A).4A). We also analyzed the expression of the related mast cell gene Mcpt2, which encodes a proteolytically inactive gene product and is often coregulated with Mcpt1. Levels of Mcpt1 and Mcpt2 expression were low at baseline in epithelial samples from both WT and β6 KO mice and were significantly increased in WT mice, but not in β6 KO mice, after chronic allergen challenge. Expression of Mcpt4, Mcpt5, Mcpt6, and Cpa3 transcripts were significantly increased at baseline in the β6 KO mice. As expected, in most cases, qRT-PCR gave a larger estimate of the magnitude of the increase in expression than did microarray, but the relative expression of each gene was similar by both methods. Importantly, none of these differences were apparent from qRT-PCR of RNA from whole lung (Supplemental Figure 1).
These results raised the possibility that mast cells might be more abundant, even in the absence of allergen challenge, within the epithelium of β6 KO mice. Cytospin preparation of brushing samples were stained for chloroacetate esterase activity to identify mast cells, and the ratio of mast cells to total cells was significantly increased in airway samples from β6 KO mice (Figure (Figure4,4, B and C). The increase in intraepithelial mast cells was confirmed by toluidine blue staining of tracheal sections from unchallenged mice, with mast cell numbers increased 7-fold in the epithelium of β6 KO mice (Figure (Figure4,4, D and E).
The increase in the number of intraepithelial mast cells at baseline in β6 KO mice likely contributed to the increase in Mcpt4, Mcpt5, Mcpt6, and Cpa3 seen in epithelial brushings from these animals. To determine whether the increase in mast cell number was the sole cause of these changes in gene expression, we normalized the gene expression level for number of intraepithelial mast cells. After normalization, the levels of Mcpt4, Mcpt5, Mcpt6, and Cpa3 remained significantly higher in untreated β6 KO mice than in WT control mice (Supplemental Figure 2), which suggests that both increased mast cell numbers and changes in gene expression in each mast cell likely contribute to the overall increase observed in the expression of these mast cell protease genes.
mMCP-1 and mMCP-2 have previously been shown to be induced by TGF-β (23, 24), but previous studies have not described effects of TGF-β on mMCP-4, mMCP-5, mMCP-6, or CPA3. We thus evaluated whether TGF-β might fully explain differences in mast cell protease expression in β6 KO mice by differentiating BM-derived cultured mast cells (BMCMCs) in the presence or absence of TGF-β. After 3 weeks of culture, qRT-PCR analyses revealed TGF-β–dependent induction of Mcpt1 (171-fold) and Mcpt2 (47-fold) and suppression of Mcpt4 (11-fold) and Mcpt6 (6-fold) (Figure (Figure5A).5A). Expression of Mcpt5 and Cpa3 (data not shown) was not affected by TGF-β. Western blotting of BMCMC lysates confirmed that TGF-β induced the expression of mMCP-1 and mMCP-2 and suppressed the expression of mMCP-4 and mMCP-6 (Figure (Figure5B).5B). BMCMCs from β6 KO mice secreted comparable levels of mMCP-1 when differentiated in the presence of recombinant TGF-β and secreted comparable levels of mMCP-6 when differentiated in the absence of recombinant TGF-β to WT BMCMCs (Supplemental Figure 4), which suggests that the differences we observed in vivo are not caused by unresponsiveness of mast cells in these mice to active TGF-β. Although the recombinant TGF-β–induced increase in Mcpt1 mRNA appeared to be reduced in BMCMCs from β6 KO mice, recombinant TGF-β still increased mMCP-1 expression by more than 100-fold. Together with comparable induction of mMCP-1 protein secretion, these observations lead us to believe that this apparent difference is unlikely to have biological meaning.
To determine whether differences in mast cell protease expression could explain the protection of β6 KO mice from allergen-induced AHR, we evaluated effects of supernatants from activated BMCMCs differentiated in the presence or absence of TGF-β on the contractility of mouse tracheal rings. Degranulation in response to DNP-IgE and DNP was similar in both types of BMCMCs, as determined by β-hexosaminidase release (Figure (Figure5C),5C), and TGF-β did not differentially affect mast cell numbers, as determined by flow cytometry with c-kit antibody (data not shown). mMCP-1 was only detected in the supernatant of activated BMCMCs differentiated in the presence of TGF-β, and mMCP-6 was only detected from BMCMCs differentiated in the absence of TGF-β (Figure (Figure5D).5D). mMCP-2 was also detected in the supernatant in which TGF-β was present, but mMCP-4 was not detected in the supernatant lacking TGF-β (data not shown), perhaps because of low sensitivity of the only available antibody to mMCP4. We added supernatants to tracheal rings and assessed contractile responses after 30-minute incubations (Figure (Figure6A).6A). Whereas supernatant lacking TGF-β had no effect on methacholine-induced contraction, supernatant containing TGF-β significantly increased responses to methacholine. To determine the role of proteases in this response, we added various protease inhibitors to the supernatants (Figure (Figure6B).6B). Only the chymotrypsin inhibitor chymostatin, an effective inhibitor of mast cell chymases (25), inhibited enhanced contractility, whereas the cysteine and trypsin-like protease inhibitor leupeptin and the metalloprotease inhibitor marimastat did not. Supernatant with TGF-β contained 2 chymase family members, mMCP-1 and mMCP-2 (Figure (Figure5D),5D), but mMCP-2 does not have protease activity (23). To determine whether enhancement of airway contractility was induced specifically by mMCP-1, we evaluated the effects of TGF-β–containing supernatant from mMCP-1 KO mice (Figure (Figure6C).6C). The absence of Mcpt1 transcripts in BMCMCs derived from mMCP-1 KO mice was confirmed by qRT-PCR (Supplemental Figure 3A). Supernatants from mMCP-1 KO BMCMCs were completely devoid of contractility-enhancing activity. Moreover, direct incubation of activated recombinant mMCP-1 (rmMCP-1) with tracheal rings enhanced methacholine-induced contractility to the same extent as did WT mouse supernatant with TGF-β (Figure (Figure6,6, C and D).
β6 KO mice have increased numbers of intraepithelial mast cells at baseline that specifically express mMCP-4 and mMCP-6. Given the protection of these mice from AHR induced by allergen challenge, we wondered whether these proteases specifically inhibit allergen challenge–induced enhanced airway smooth muscle contractility. One of the central mediators of allergen-induced AHR is IL-13, which has previously been shown to directly increase contractility of tracheal rings (26). We therefore incubated tracheal rings for 12 hours with either IL-13 or saline, washed out the cytokine, and then examined the effects of 30-minute incubation with supernatants of degranulated BMCMCs from WT mice (Figure (Figure7A).7A). As expected, IL-13 enhanced methacholine-induced contraction, and this augmented contractility was significantly inhibited by supernatant in which TGF-β was absent. This suppressive effect was significantly inhibited by chymostatin, but not by other protease inhibitors with less effect on chymases (Figure (Figure7B).7B). Supernatant lacking TGF-β contained a single chymase (mMCP-4), 1 elastase (mMCP-5), 2 tryptases (mMCP-6 and mMCP-7), and a metalloexopeptidase (CPA3). Our finding that chymostatin, but not leupeptin or marimastat, blocked this protective effect suggested it might be caused by mMCP-4. We thus differentiated BMCMCs from mMCP-4 KO mice, confirmed the absence of Mcpt4 by qRT-PCR (Supplemental Figure 3B), and found that supernatants from BMCMCs derived from mMCP-4 KO mice were completely devoid of this suppressive activity (Figure (Figure7A).7A). Activated rmMCP-4 also significantly suppressed IL-13–induced enhancement of contractility, without effects on baseline responses (Figure (Figure7C).7C). In mice, there are several expressed mast cell chymase-like proteases, but there is only 1 chymase in humans, and its functional homolog is thought to be mMCP-4 (27). We therefore evaluated the effect of recombinant human chymase on IL-13–enhanced contraction and found significant suppression, similar to the effects of rmMCP-4 (Figure (Figure7,7, C and D).
Tracheal rings include a number of cell types, including a layer of epithelial cells. To evaluate whether mast cell products act directly on epithelial cells, we removed epithelium from tracheal rings (Figure (Figure8A)8A) and examined the effects of mMCP-1 and mMCP-4 on contraction. As expected, epithelium removal enhanced the magnitude of force generation in response to methacholine. In tracheal rings with epithelium removed, supernatant in which TGF-β was present was completely devoid of contractility-enhancing activity, and a similar effect was seen for activated rmMCP-1 (Figure (Figure8,8, B and C). In contrast, supernatants of mast cells differentiated in the absence of TGF-β significantly suppressed IL-13–induced contractility in rings that were completely denuded of epithelium, and a similar effect was seen for rmMCP-4 (Figure (Figure8,8, D and E).
TGF-β has been previously shown to exert pleiotropic, context-specific effects on allergic asthma, mostly through effects on T cells, fibroblasts, and potentially smooth muscle cells (14, 18–21, 28). Our findings suggest novel roles for TGF-β as a potent switch regulating mast cell protease expression and as an inhibitor of mast cell accumulation within the airway epithelium. These effects appear to play an important role in regulating contractile responses of airway smooth muscle and in vivo AHR after chronic allergen challenge. Previous studies using mast cell–deficient mice have shown that mast cells contribute to AHR development when mice are sensitized and challenged with an adjuvant-free regimen (5, 6), as we used here. Our results suggest that these effects are probably caused by TGF-β–dependent differentiation of intraepithelial mast cells expressing mMCP-1, but not those expressing mMCP-4. Our results also suggest that mast cell–dependent induction of AHR might be prevented by inhibition of the αvβ6 integrin within the airway epithelium.
Although previous work suggested that expression of mMCP-1 and mMCP-2 in intestinal intraepithelial mast cells depends on TGF-β activation through the αvβ6 integrin and that TGF-β is required for differentiation of mMCP-1– and mMCP-2–expressing mast cells in vitro (23), to our knowledge, our finding that mMCP-4 and mMCP-6 expression was inhibited by TGF-β is novel. We were also surprised to find significant accumulation of mMCP-4– and mMCP-6–containing mast cells within the epithelium in the absence of αvβ6-mediated TGF-β activation. Previous studies of intraepithelial mast cells in the intestinal epithelium of β6 KO mice identified mast cells by mMCP-1 immunostaining (29), and might thus have missed these intraepithelial mast cells that do not express mMCP-1. In the present study, we did not determine the mechanisms that lead to accumulation of these mast cells in the absence of local TGF-β activation. TGF-β has been reported to promote mast cell proliferation and migration (30). Mitogen-activated protein kinase activity and integrins have previously been shown to be involved in TGF-β–regulated mast cell migration (31–33). However, TGF-β1 has also been reported to act as a negative regulator of mast cell function (34), and it is well accepted that mast cell proliferation and migration can be regulated by different mechanisms in different locations (35). Mast cells are also known to accumulate at sites of inflammation (36), so it is possible that the increase in baseline intraepithelial mast cells in β6 KO mice is caused by their low-level baseline inflammation, as we have previously described (37).
It is noteworthy that the significant differences in intraepithelial mast cell numbers and mast cell protease expression we describe here were not at all apparent from microarray or qRT-PCR analysis of whole lung samples. These effects could only be identified by sampling the airway epithelial microenvironment. The simple airway brush we have developed should thus be a useful tool for future investigations of cellular and gene expression changes that are restricted to the epithelium.
The protective effects of mMCP-4 on airway smooth muscle contractility were somewhat surprising, given the extensive literature describing the contributions of mast cells to the pathophysiology of allergic asthma and AHR (1, 4, 5, 38, 39). However, our findings are consistent with a previous report of enhanced AHR after allergen challenge in mice lacking mMCP-4 (40). Furthermore, mMCP-4 is the closest functional homolog of human mast cell chymase (27), and epithelial chymase expression has been suggested to be protective against asthma severity in human subjects with asthma (41, 42). Given the increased number of intraepithelial mast cells we observed in β6 KO mice, it seems likely that the increased levels of Mcpt4 and Mcpt6 we observed were caused by the combined effects of increased mast cell accumulation and increased Mcpt4 and Mcpt6 expression in these cells.
Interestingly, mMCP-1 and mMCP-4 not only exert opposite effects on airway contractility, they do so by acting on distinct cell types. Our observation that the contractility-enhancing effect of mMCP-1 was completely abrogated by removal of airway epithelium suggests that mMCP-1 is released within the epithelium and acts directly on a substrate within the epithelial compartment to enhance airway smooth muscle contraction and airway narrowing. In contrast, the inhibitory effects of mMCP-4 on IL-13–enhanced airway contractility were completely preserved in tracheal rings denuded of epithelium, which suggests that mMCP-4 is acting on substrates outside of the epithelial compartment. One attractive hypothesis is that mMCP-4 acts directly on substrates on airway smooth muscle cells. However, given the cellular complexity of tracheal rings, the evidence presented here cannot exclude effects on substrates on other cells or extracellular compartments in the airway wall.
One obvious issue not addressed by the current work is the precise nature of the proteolytic substrates for mMCP-1 and mMCP-4 that regulate the opposing effects of these proteases on airway smooth muscle contractility. Although not much is known about substrates for mMCP-1, several substrates have been described for mMCP-4, including angiotensin I, pro-gelatinase, hepatocyte growth factor, thrombin, and fibronectin (27, 43–46). However, the in vivo relevance of these substrates to airway responsiveness is unclear. Identification of the substrates responsible for the effects described herein could lead to new strategies for protection against AHR and human asthma. Although there is no precise human ortholog for mMCP-1, once the proteolytic substrate and downstream molecular cascade responsible for enhancement of airway smooth muscle contractility is identified, the potential relevance of this pathway to human asthma could be more readily evaluated.
Rat anti–mMCP-1 monoclonal antibody (RF6.1) (47) and sheep anti–mMCP-2 polyclonal antibody (23) were provided by A. Pemberton (University of Edinburgh, Edinburgh, United Kingdom). Goat anti–mMCP-4 polyclonal antibody and rat anti–mMCP-6 monoclonal antibody were purchased from Abcam and R&D, respectively. Mouse anti–β-actin monoclonal antibody was purchased from Abcam. Marimastat, chymostatin, and leupeptin were from Tocris, Sigma-Aldrich, and Roche, respectively. Recombinant pro–mMCP-1 was purchased from R&D and activated by recombinant mouse active cathepsin C/DPPI (R&D). rmMCP-4 was expressed by ligation-independent cloning of the catalytic domain cDNA into the pIEx 3 insect expression vector (Novagen), which encodes an N-terminal signal/pseudopropeptide incorporating glutathione S-transferase, the S-Tag sequence, a poly-His segment for use in nickel affinity purification, and an enteropeptidase cleavage site immediately preceding the catalytic domain sequence. Expression of the full-length chimera resulted in precipitation of the recombinant preprotein, which was resolved by reengineering the pseudopropeptide by replacing the portion of the expression plasmid encoding glutathione S-transferase with a short linker sequence encoding the amino acid sequence PERWA. The plasmid was transfected into Sf-9 insect cells grown in serum-free media. Recombinant protein was partially purified by heparin chromatography, activated by digestion with enteropeptidase, and further purified by cation exchange chromatography, which separated active mMCP-4 from enteropeptidase. Recombinant human pro-chymase was expressed, activated, and purified as described previously (48).
Mice functionally deficient in β6 integrin have been previously characterized (37). All of the experiments using β6 KO mice were conducted in mice backcrossed 5–10 generations to FVB/NJ background. mMCP-4 KO mice have been previously described (49). mMCP-1 KO mice were purchased from the mutant mouse regional resource center at University of Missouri. Mice used for all the experiments were 6–8 weeks old and housed under specific pathogen–free conditions in the Animal Barrier Facility of UCSF.
Mice were sensitized on days 1, 4, and 7 by intraperitoneal injection of 10 μg OVA in a total volume of 200 μl saline. Control animals received an equal volume of saline only. Mice were lightly anesthetized with isoflurane inhalation and intranasally challenged with OVA (20 μg in 30 μl saline) or saline every 7 days during days 14–70.
24 hours after the last challenge, pulmonary resistance was measured in response to a range of concentrations of intravenous acetylcholine using the forced oscillation technique with the FlexiVent system (SCIREQ) as previously described (50).
Total and differential cell percentages were determined by counting in a hemocytometer and by light microscopic evaluation of more than 300 cells per slide as previously described (50). After lavage, lungs were inflated with 10% buffered formalin to 25 cm H2O and transferred to 10% buffered formalin. 5-μm sections were stained with H&E for morphology, periodic acid–Schiff reagent for evaluation of mucus production, and Sirius red for evaluation of fibrosis.
Brushes were made from 60-grit sandpaper–polished polyethylene PE-10 tube (BD Biosciences) with an inserted stainless wire (0.095 mm diameter). For epithelial harvesting, mice were anesthetized with ketamine (100 mg/kg body weight) and xylazine (10 mg/kg), the brush was inserted through an incision into the midsection of the trachea, and harvested epithelium was collected into 400 μl phosphate-buffered saline for cytospin preparation or 350 μl RNeasy lysis buffer (Buffer RLT; Qiagen) for RNA preparation. Cytospin cells were stained with a HEMA 3 stain set (Fisher) for checking the morphology of epithelium and with naphthol AS-D chloroacetate esterase staining kit (Sigma-Aldrich) for mast cells according to the manufacturer’s instructions. For counting intraepithelial mast cell numbers in murine trachea, tracheas were fixed in 10% formalin for 48 hours and embedded in paraffin. 5-μm sections were stained with 0.5% toluidine blue (Sigma-Aldrich) in 0.5 M HCl.
24 hours after the last challenge, airway epithelium was brush-harvested, and RNA quality was confirmed by Agilent nanotechnology. Expression microarrays were performed using Agilent Bioanalyzer (Mouse One-Color 4x44K array platform) in the UCSF Sandler Asthma Basic Research Center Functional Genomics Core Facility. Additional information about microarray protocols and complete microarray data are available from Gene Expression Omnibus (accession no. GSE28168; http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE28168).
BMCMC culture was performed as described previously (51), with a slight modification. Briefly, BM cells prepared from femurs of 10- to 12-week-old sex-matched mice were cultured for 21 days in DMEM supplemented with 10% fetal bovine serum, 100 U/ml penicillin, 100 μg/ml streptomycin, 2.5 μg/ml fungizone, 2 mM l-glutamine, and 1 mM sodium pyruvate. Mast cell growth and differentiation were stimulated with mouse IL-3 (1 ng/ml; R&D), mouse IL-9 (5 ng/ml; R&D), and mouse stem cell factor (50 ng/ml; PeproTech) with or without human TGF-β1 (1 ng/ml; R&D).
After 3 weeks of culture, BMCMCs (1 × 106 cells/ml) were sensitized with 1 μg/ml anti–DNP-IgE mAb (SPE7; Sigma-Aldrich) overnight at 37°C, washed, and resuspended at 2.5 × 105 cells/ml in Tyrode buffer (12 mM NaHCO3, 0.4 mM NaH2PO4, 137 mM NaCl, 2.7 mM KCl, 1.8 mM CaCl2, 1 mM MgCl2, 5.6 mM d-glucose, and 0.1% BSA [pH 7.4]). Degranulation was initiated by addition of 10 ng/ml DNP-BSA (Invitrogen) for 30 minutes at 37°C. The degree of degranulation was determined by release of β-hexosaminidase (52). The remaining cells were lysed by addition with Tyrode buffer containing 0.1% Triton X-100. The supernatants and cell lysates (20 μl each) were incubated with 80 μl of 2.9 mM 4-nitrophenyl-N-acetyl-β-D-glucosaminide (Sigma-Aldrich) in 0.1 M sodium citrate buffer (pH 4.8) for 1 hour at 37°C. The reaction was terminated by the addition of 200 μl 0.1 M sodium carbonate buffer (pH 10.2). The release of the product 4-nitrophenol was detected by measuring absorbance at 405 nm. Controls without antigen were used to measure spontaneous release. Release in the supernatant was calculated as percent total cellular (lysate plus supernatant) β-hexosaminidase.
Tracheal ring segments approximately 3 mm in length were suspended in a 15-ml organ bath by 2 stainless steel wires (0.2 mm diameter) passed through the lumen. One wire was fixed to the organ bath, while the other was connected to a force-displacement transducer (FT03; Grass Instrument Co.) for the measurement of isometric force. A resting tension of 0.5 g was applied, and rings were equilibrated for 45 minutes. The buffer solution containing modified Krebs-Henseleit solution (117.5 mM NaCl, 5.6 mM KCl, 2.5 mM CaCl2, 1.18 mM MgSO4, 25 mM NaHCO3, 1.28 mM NaH2PO4, and 5.55 mM glucose) was maintained at 37°C and oxygenated with 95% O2, 5% CO2. After incubation with the supernatant of degranulated BMCMCs (30 μl/ml final concentration) for 30 minutes at 37°C, rings were initially contracted in response to 60 mM KCl, and only rings that could generate more than 2.5 mN tension were used for experiments. Contractile response was evaluated with increasing concentrations of methacholine (10–9 to 10–4 M). For analysis of suppressive effects on IL-13–induced contractility, rings were treated with IL-13 (100 ng/ml; Peprotech) in DMEM, 10 mM HEPES (pH 7.3), 100 U/ml penicillin, and 100 μg/ml streptomycin for 12 hours at 37°C; washed; and then incubated with the supernatant of degranulated BMCMCs (30 μl/ml final concentration) for 30 minutes at 37°C before assessment of contractility. To evaluate whether mast cell products were acting on epithelial cells, we completely removed epithelium in some rings by gentle rubbing with the airway brush. Epithelial removal was confirmed for each individual ring by microscopic observation of H&E-stained sections.
Total RNA was isolated with RNeasy kit (Qiagen). cDNA was analyzed by SYBR-Green real-time PCR with an ABI 7900HT thermocycler and normalized to Gapdh expression. Primers used were as follows: Gapdh forward, TGGTGAAGGTCGGTGTGAAC; Gapdh reverse, GACAAGCTTCCCATTCTCGG; Cdh1 forward, CGTCCATGTGTGTGACTGTG; Cdh1 reverse, GCTCTTTGACCACCGTTCTC; Foxj1 forward, ACCAAGATCACTCTGTCGGC; Foxj1 reverse, TGTTCAAGGACAGGTTGTGG; Acta2 forward, TCCTGACGCTGAAGTATCCG; Acta2 reverse, GTGCCTCTGTCAGCAGTGTC; Pecam1 forward, CAAGCAAAGCAGTGAGCTG; Pecam1 reverse, AGCAGGACAGGTCCAACAAC; Mcpt1 forward, TTCCAGGTCTGTGTGGGAAG; Mcpt1 reverse, TCCAGGGCACATATGCAGAG; Mcpt2 forward, AACGGTTCGAAGGAGAGGTG; Mcpt2 reverse, TCTGCTGTGTGGGTTCGTTC; Mcpt4 forward, TCACCACTGAGAGAGGGTTCA; Mcpt4 reverse, CATGAGCTCCAAGGGTGACA; Cma1 forward, CCTGCAGTGGCTTCCTGATA; Cma1 reverse, GCATGATGTCGTGGACAACC; Tpsb2 forward, GAGCTTGAGGTCCCTGTGAA; Tpsb2 reverse, GATAAGGAGGTGGGAGAGGC; Cpa3 forward, GACCAAACTCTTGGACCGGA; Cpa3 reverse, GTTGAGGTCAGTGCCAATGC.
Lysates of differentiated BMCMCs (2 μg) or the supernatant of degranulated BMCMCs (20 μl) were separated by 12% SDS-PAGE, transferred to a polyvinylidene difluoride membrane (Millipore), and blocked for 30 minutes in Tris-buffered saline containing 5% skim milk. Membranes were incubated with antibodies to mMCP-1, mMCP-2, mMCP-4, or mMCP-6 for 1 hour, then with peroxidase-conjugated secondary antibody for 1 hour, and developed with Plus-ECL reagent (PerkinElmer).
Paired data were evaluated using a 2-tailed Student’s t test. 1-way ANOVA was used for multiple comparisons, and when differences were statistically significant, this was followed with a t test with Bonferroni correction for subsequent pairwise analysis. Data were analyzed with StatView version 5.0 software. Differences with a P value less than 0.05 were considered statistically significant.
All experiments were approved by the Institutional Animal Care and Use Committee of UCSF.
This work was supported by a NIH/NCRR UCSF-CTSI grant and NIH grants AI077439, HL53949, and HL102292 (to D. Sheppard); by Medical Research Council (to M Åbrink); by NIH grant HL024136 (to G. Caughey); and by the UCSF Strategic Asthma Basic Research (SABRE) Program. We thank Rebecca Barbeau, Chris Eisley, and Andrea Barczak (Functional Genomics Core, UCSF) for microarray analyses and Alan Pemberton for providing mMCP-1 and mMCP-2 antibodies.
Conflict of interest: The authors have declared that no conflict of interest exists.
Citation for this article: J Clin Invest. 2012;122(2):748–758. doi:10.1172/JCI58815.