Differential effects of cytokines and corticosteroids on Toll-like receptor 2 expression and activity in human airway epithelia
© Winder et al. 2009
Received: 10 February 2009
Accepted: 16 October 2009
Published: 16 October 2009
The recognition of microbial molecular patterns via Toll-like receptors (TLRs) is critical for mucosal defenses.
Using well-differentiated primary cultures of human airway epithelia, we investigated the effects of exposure of the cells to cytokines (TNF-α and IFN-γ) and dexamethasone (dex) on responsiveness to the TLR2/TLR1 ligand Pam3CSK4. Production of IL-8, CCL20, and airway surface liquid antimicrobial activity were used as endpoints.
Microarray expression profiling in human airway epithelia revealed that first response cytokines markedly induced TLR2 expression. Real-time PCR confirmed that cytokines (TNF-α and IFN-γ), dexamethasone (dex), or cytokines + dex increased TLR2 mRNA abundance. A synergistic increase was seen with cytokines + dex. To assess TLR2 function, epithelia pre-treated with cytokines ± dex were exposed to the TLR2/TLR1 ligand Pam3CSK4 for 24 hours. While cells pre-treated with cytokines alone exhibited significantly enhanced IL-8 and CCL20 secretion following Pam3CSK4, mean IL-8 and CCL20 release decreased in Pam3CSK4 stimulated cells following cytokines + dex pre-treatment. This marked increase in inflammatory gene expression seen after treatment with cytokines followed by the TLR2 ligand did not correlate well with NF-κB, Stat1, or p38 MAP kinase pathway activation. Cytokines also enhanced TLR2 agonist-induced beta-defensin 2 mRNA expression and increased the antimicrobial activity of airway surface liquid. Dex blocked these effects.
While dex treatment enhanced TLR2 expression, co-administration of dex with cytokines inhibited airway epithelial cell responsiveness to TLR2/TLR1 ligand over cytokines alone. Enhanced functional TLR2 expression following exposure to TNF-α and IFN-γ may serve as a dynamic means to amplify epithelial innate immune responses during infectious or inflammatory pulmonary diseases.
The airway epithelium plays an important role in orchestrating pulmonary innate and adaptive immune responses. This mucosal surface is a site of first contact with the environment and has evolved many mechanisms to recognize and respond to inhaled or aspirated microorganisms. Epithelial responses to microbes are initiated via pattern recognition receptors including the Toll-like receptors (TLRs) . TLRs are a family of 10 receptors in humans that recognize a variety of microbial molecular patterns and regulate immune responses. Airway epithelial cell responses to a number of TLRs, including TLR2 [2–4], TLR3 , TLR4 , TLR5 [7, 8], and TLRs 6 through 9 [9, 10] have been investigated in human cells and animal models. TLR activation initiates signaling that culminates in a number of host defense responses including the secretion of antimicrobial peptides, cytokines, and chemokines by epithelial cells [11, 12].
TLR expression is regulated in a cell and tissue specific manner [11, 13–15]. Experimental evidence in humans  and animal models [17–20] indicates that the expression and function of several TLRs is developmentally regulated. Here we focus on TLR2 expression and function in well-differentiated human respiratory epithelia. TLR2 forms heterodimers with either TLR6 or TLR1; these heterodimers recognize diacyl and triacyl lipopeptides, respectively [21, 22]. TLR2 signaling occurs via a MyD88-dependent pathway leading to the nuclear translocation of NF-κB , and induction of various inflammatory cytokines, including IL-8, and antimicrobial peptides, such as human beta-defensin 2 (HBD-2) [4, 23].
We hypothesized that first response cytokines would influence both the array of functional TLRs and their responses to stimuli. Further, dexamethasone, when co-administered with pro-inflammatory cytokines, was reported to synergistically enhance TLR2 expression in the human alveolar and bronchial epithelial cell lines A549  and BEAS-2b . We therefore investigated the effects of both cytokine and glucocorticoid exposure on TLR2 expression in primary cultures of human airway epithelia.
Culture of human airway epithelia
Primary cultures of human airway epithelia were grown at an air-liquid interface as described previously . Human donor lungs were obtained from individuals without primary pulmonary diseases whose lungs were determined to be unsuitable for organ transplantation. The use of human tissues was approved by the University of Iowa Institutional Review Board. Well-differentiated (> 2 weeks in culture) tracheal and bronchial epithelia were used in all studies. Epithelia were maintained in DMEM/F-12 with 1% penicillin-streptomycin, 50 μg/ml gentamicin, and 2% Ultroser G. In a microarray experiment (described below), epithelia were incubated for 24 hours in 2% Ultroser G media containing 100 ng/ml each of recombinant interleukin-1-beta (IL-1β; Sigma, St. Louis, MO), tumor necrosis factor-alpha (TNF-α; Sigma), and interferon-gamma (IFN-γ; Sigma). For all other experiments, epithelia were placed in serum free DMEM/F-12 for 48 hours, then incubated overnight (18 hr) in media containing cytokines (100 ng/ml each of TNF-α and IFN-γ), 1 μM water-soluble dexamethasone (D2915; Sigma), cytokines plus dexamethasone, or control serum-free media (100 μl volume applied apically, and 500 μl basolaterally). Cell viability was similar under all experimental conditions.
In TLR2 receptor agonist experiments, epithelia were rinsed with media, then incubated for an additional 24 hours in media containing 25 μg/ml Pam3CSK4 (tlrl-pms; InvivoGen, San Diego, CA), a synthetic bacterial lipoprotein TLR2/TLR1 ligand, or control serum-free media. Where specified, media containing cytokines ± dexamethasone or Pam3CSK4 were applied to only the apical or basolateral surface, with control serum-free media applied contralaterally. Prior to assays of airway surface liquid antimicrobial activity (see Antimicrobial Assays, below), epithelia were incubated for 5 days in antibiotic-free media and washed daily with antibiotic-free media to remove residual antibiotics.
RNA isolation and quantitative reverse transcription-PCR (RT-PCR)
RNA was extracted using an RNeasy Mini Kit (Qiagen Inc., Valencia, CA) according to manufacturer's protocol. For each sample, 1 μg of total RNA was used as a template for first-strand cDNA synthesis. Quantitative PCR (ABI 7900) was used to amplify the TLR or HBD-2 PCR products along with GAPDH transcripts in a single reaction. Forward and reverse primers and TaqMan probes were designed using Primer Express software (P-E Applied Biosystems, Foster City, CA). Primers and probes were: TLR2 forward, 5'-GGCCAGCAAATTACCTGTGTG-3'; TLR2 reverse, 5'-AGGCGGACATCCTGAACCT-3'; TLR2 probe, 5'-TCCATCCCATGTGCGTGGCC-3'; TLR1 forward, 5'-CAGTGTCTGGTACACGCATGGT-3'; TLR1 reverse, 5'-TTTCAAAAACCGTGTCTGTTAAGAGA-3'; TLR1 probe, 5'-TGCCCATCCAAAATTAGCCCGTTC-3'; TLR6 forward, 5'-GAAGAAGAACAACCCTTTAGGATAGC-3'; TLR6 reverse, 5'-AGGCAAACAAAATGGAAGCTT-3'; TLR6 probe, 5'-TGCAACATCATGACCAAAGACAAA-3'; HBD-2 forward, 5'-CCTGTTACCTGCCTTAAGAGTGGA-3'; HBD-2 reverse, 5'-ACCACAGGTGCCAATTTGTTTA-3'; HBD-2 probe: 5'-CCATATGTCATCCAGTCTTTTGCC-3'. The TLR and HBD-2 probes were labeled with the fluorophore FAM, and the GAPDH probe with the fluorophore JOE. C T for the TLR or HBD-2 PCR product was normalized against the C T for GAPDH.
Five micrograms of total RNA was processed using the Affymetrix GeneChip one-cycle target labeling kit (Affymetrix, Inc., Santa Clara, CA) following the manufacturer's protocols. The resultant biotinylated cRNA was hybridized to a custom GeneChip Human Airway Array (HsAirway, Affymetrix, Inc.). Tracheal and bronchial epithelial cells from seven donors were used in this study. The custom Affymetrix array (HsAirway) was comprised of approximately 23,000 probe sets derived from sequencing of cDNA libraries prepared from human lung, primary airway epithelial cells, and human alveolar macrophages . The arrays were washed, stained, and scanned using the Affymetrix Model 450 Fluidics Station and Affymetrix Model 3000 scanner. Each sample and hybridization underwent quality control evaluation, including cRNA amplification of more than 4-fold, percentage of probe sets reliably detecting between 40 and 60 percent present call, and 3'-5' ratio of GAPDH gene less than 3.
The hybridizations were normalized using the RMA (robust multi-chip averaging)  method from Bioconductor  to obtain summary expression values for each probe set. Gene expression levels were analyzed on a logarithmic scale. Differentially expressed genes were identified using a 1-factor ANOVA test. Heat-map visualizations were generated with GenePattern . Global scaling of the expression levels was used to allow experiment-wide comparison of gene expression.
Protein quantification by ELISA
IL-8 and CCL20 protein abundance in the basolateral media was measured by ELISA (Duoset DY208 (IL-8) and DY360 (CCL20); R&D Systems, Minneapolis, MN).
Apical washings from epithelia were obtained after a 24-hour incubation with the TLR2 agonist Pam3CSK4 or control serum-free, antibiotic-free media. Airway surface liquid (ASL) was obtained by adding 100 μl of sterile 1× PBS to the apical surface and immediately pipetting off the fluid. We used a modified radial diffusion assay to quantify ASL antimicrobial activity as described previously . Briefly, 4 × 106 bacteria in mid-log phase were suspended in an underlay gel. 2.5 mm diameter wells were punched into the gel and filled with 0.04-5 μl of ASL, with 0.02% acetic acid with 0.1% human serum albumin (Sigma) to equal 5 μl, or control antibiotic (gentamicin, 0.4-50 μg/ml). The plates were then incubated for 3 hours at 37°C. Nutrient rich gels were then overlaid, and the plates incubated at 37°C overnight. Zones of clearance were manually measured and plotted on a semi-log graph where the X-intercept represents the minimal inhibitory concentration (MIC) . Test organisms included Escherichia coli DH5α, Pseudomonas aeruginosa PA01, and a clinical strain of Listeria monocytogenes.
Whole cell protein extract preparation and immunoblot analysis were performed as described previously [32, 33]. Primary antibodies used to detect specific cellular and nuclear proteins were: mouse IgG1 mAb clone L35A5 against human IκBα, rabbit polyclonal IgG 9171 against human Stat1 phosphorylated on tyrosine-701, rabbit polyclonal IgG 9172 against human total Stat1, rabbit IgG mAb clone 3D7 against human p38 MAP kinase phosphorylated on threonine-180 and tyrosine-182, rabbit IgG mAb clone 7D6 against human total p38 MAP kinase from Cell Signaling Technology (Beverly, MA); mouse IgG2α mAb clone AC-74 against human β-actin from Sigma-Aldrich (St. Louis, MO); rabbit polyclonal antiserum against human heat shock protein (HSP)-90 from Assay Designs (Ann Arbor, MI). Primary antibody binding was detected using goat antirabbit or antimouse IgG conjugated to horseradish peroxidase (Santa Cruz Biotechnology, Santa Cruz, CA or Cell Signaling Technologies) and an enhanced chemiluminescence detection system (Amersham Biosciences, Uppsala, Sweden). Reprobing of membranes was done after washing twice in Restore™ buffer (Pierce, Rockford, IL) for 15 min at 37°C. In some experiments, radiographic film images were analyzed using ImageJ software . To generate an integrated density level, band area was multiplied by the band mean gray value, and the integrated density for IκBα or phosphorylated p38 was divided by the corresponding β-actin or HSP-90 level creating a ratio for each sample.
NF-κB Activation Assay
NF-κB-dependent gene activation was determined using a recombinant adenoviral vector that expresses a luciferase gene driven by four tandem NF-kB enhancer sequences as described previously [32, 35]. Photinus pyralis luciferase activity was determined using a commercial luciferase reporter assay kit (Promega) and a Lumat LB 9501 luminometer (Berthold, Bad Wildbad, Germany).
Assessment of statistical significance for quantitive PCR and ELISA data was performed using one-tailed Student's t tests with Microsoft Excel. P values < 0.05 were considered significant. Luciferase assays and densitometry analysis were analyzed for statistical significance using ANOVA for a factorial experimental design. The multicomparison significance level for the ANOVA was 0.05. If significance was achieved by one-way analysis, post-ANOVA comparison of means was performed using Tukey's test .
Results and Discussion
Microarray profiling of TLR expression in airway epithelia
Induction of TLR2 mRNA expression in airway epithelia
TLR2 expression was previously documented in human airway cell lines, passaged cells in submersion culture, or in lung tissues [2, 4, 9, 10, 37]. Although these studies noted TLR2 expression in several model systems, the functional consequences of combined cytokine and glucocorticoid treatment were not investigated, nor were the polarity of TLR2 responses. We focused on functional TLR2 responses in well-differentiated primary airway epithelia. With the exception of studies by Becker et al  and Hertz and colleagues , TLR2 expression and function has been little studied in this model that closely mimics the in vivo airways.
As cell-surface TLR2 exists as a heterodimer with either TLR1 or TLR6 [21, 22], we next investigated the effects of cytokine and dexamethasone exposure on TLR1 and TLR6 mRNA expression. As shown in Figure 2B, TLR1 mRNA abundance remained unchanged following cytokine ± dexamethasone treatment. Unlike TLR2, TLR6 mRNA decreased modestly following cytokine treatment, both in the presence, and absence, of dexamethasone (P < 0.05).
Treatment with cytokines ± dexamethasone alters effects of TLR2 receptor ligation in airway epithelia
To determine the functional effects of increased TLR2 expression, epithelia pre-treated with cytokines ± dexamethasone were stimulated with the TLR1/2 ligand Pam3CSK4 for 24 hours. Two different concentrations of Pam3CSK4, 10 and 25 μg/ml, were studied initially. As greater changes in IL-8 abundance were seen with 25 μg/ml (data not shown), this concentration was used for further studies.
Since epithelia may preferentially express proteins on either their apical or basolateral membrane domains, we asked whether cells exhibited polarized responses to Pam3CSK4. As shown in Figure 3B, IL-8 abundance increased following either apical or basolateral Pam3CSK4 application. In control cells, mean IL-8 production was over 3-fold higher following apical, compared to basolateral application (P < 0.05). A similar trend was seen in cytokine pre-treated cells, but did not reach statistical significance. These functional data suggest that TLR2 protein abundance is greater on the apical surface of polarized airway epithelia; however airway epithelia can respond to a TLR2 ligand from either surface.
The changes in TLR2 mRNA abundance were similar in pattern, though less pronounced, than those reported in epithelial cell lines. Prior studies in BEAS-2b  and A549  cells demonstrated similar increases in TLR2-mediated IL-8 production following pre-treatment with cytokines plus dexamethasone, but did not compare findings to pre-treatment with cytokines alone. While we detected TLR2 protein in cell lines overexpressing the protein, we were unable to conclusively localize TLR2 protein expression in primary cells using commercially available antibodies and methods including immunohistochemistry and surface biotinylation (data not shown). We conclude that TLR2 protein is functionally present in this model but below the limits of immunodetection.
Effects of Cytokines on Pam3CSK4 Signaling Responses
Human airway epithelial cells respond to cytokines and bacterial products through induction of specific signaling pathways. The functional expression of TLR2 may be regulated by more than one receptor-mediated signaling pathway prominent in the early responses to bacterial and viral pathogens . Several groups have studied the mechanisms by which dexamethasone enhances TLR2 expression. Glucocorticoids synergistically enhanced nontypeable Haemophilus influenzae-induced TLR2 expression via induction of MAPK phosphatase-1, leading to inhibition of p38 MAPK . The results of Hermoso et al  suggest that TNF-α and dexamethasone cooperatively regulate the TLR2 promoter, through the involvement of NF-kB and STAT transcription factors, as well as a 3'-glucocorticoid response element.
TLR2 receptor ligation enhances expression of inducible host defense proteins and increases antimicrobial activity in airway surface liquid
We also assayed expression of CCL20, a peptide with both innate and adaptive immune functions produced by airway epithelia. CCL20 stimulates B-cell migration and has antimicrobial activity comparable to the β-defensins . Following Pam3CSK4 stimulation, CCL20 increased 25- to 30-fold over baseline in cells pre-treated with cytokines (Figure 7B). Dexamethasone significantly blunted this response, as CCL20 abundance in epithelia pre-treated with cytokines plus dexamethasone was approximately one-third that of cells treated with cytokines alone (P < 0.05).
We conclude that TLR2 is an inducible component of airway epithelial defenses. Enhanced functional TLR2 expression following TNF-α and IFN-γ exposure may serve as a dynamic means to amplify innate immune responses during infectious or inflammatory pulmonary diseases. Under conditions where first response cytokines are present, enhanced TLR2 signaling allows for further amplification of mucosal immunity. This increase in signalling does not correlate well with NF-κB, Stat1, or p38 MAP kinase pathway activation. The importance of lipopeptide recognition in airway defense is further demonstrated by the upregulation of several host defense proteins/peptides following receptor engagement. Our finding that glucocorticoids can act as a negative regulator of functional TLR2 expression in well-differentiated human airway epithelia has clinical implications in settings of systemic or inhaled corticosteroid use. Since TLR2-mediated responses may occur early in the host response to infection, any factors that negatively impact TLR2 expression or signaling might influence disease outcomes.
We thank Tim Starner and Ariadna Arias for their guidance and technical assistance with the antimicrobial assays. We acknowledge the support of NIH T32 AI007343 (A.W.), P50 HL-61234 (P.B.M.), N01 AI-30040 (P.B.M.), the Roy J. Carver Charitable Trust (P.B.M.), a Career Development Award from Research to Prevent Blindness (T.E.S.), HL-082505 (D.C.L.), and HL-075559 (D.C.L.). We also acknowledge the support of the Cell and Tissues and Cell Morphology Cores, partially supported by the Center for Gene Therapy for Cystic Fibrosis (NIH P30 DK-54759) and the Cystic Fibrosis Foundation.
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