- Open Access
PKA and Epac cooperate to augment bradykinin-induced interleukin-8 release from human airway smooth muscle cells
Respiratory Research volume 10, Article number: 88 (2009)
Airway smooth muscle contributes to the pathogenesis of pulmonary diseases by secreting inflammatory mediators such as interleukin-8 (IL-8). IL-8 production is in part regulated via activation of Gq-and Gs-coupled receptors. Here we study the role of the cyclic AMP (cAMP) effectors protein kinase A (PKA) and exchange proteins directly activated by cAMP (Epac1 and Epac2) in the bradykinin-induced IL-8 release from a human airway smooth muscle cell line and the underlying molecular mechanisms of this response.
IL-8 release was assessed via ELISA under basal condition and after stimulation with bradykinin alone or in combination with fenoterol, the Epac activators 8-pCPT-2'-O-Me-cAMP and Sp-8-pCPT-2'-O-Me-cAMPS, the PKA activator 6-Bnz-cAMP and the cGMP analog 8-pCPT-2'-O-Me-cGMP. Where indicated, cells were pre-incubated with the pharmacological inhibitors Clostridium difficile toxin B-1470 (GTPases), U0126 (extracellular signal-regulated kinases ERK1/2) and Rp-8-CPT-cAMPS (PKA). The specificity of the cyclic nucleotide analogs was confirmed by measuring phosphorylation of the PKA substrate vasodilator-stimulated phosphoprotein. GTP-loading of Rap1 and Rap2 was evaluated via pull-down technique. Expression of Rap1, Rap2, Epac1 and Epac2 was assessed via western blot. Downregulation of Epac protein expression was achieved by siRNA. Unpaired or paired two-tailed Student's t test was used.
The β2-agonist fenoterol augmented release of IL-8 by bradykinin. The PKA activator 6-Bnz-cAMP and the Epac activator 8-pCPT-2'-O-Me-cAMP significantly increased bradykinin-induced IL-8 release. The hydrolysis-resistant Epac activator Sp-8-pCPT-2'-O-Me-cAMPS mimicked the effects of 8-pCPT-2'-O-Me-cAMP, whereas the negative control 8-pCPT-2'-O-Me-cGMP did not. Fenoterol, forskolin and 6-Bnz-cAMP induced VASP phosphorylation, which was diminished by the PKA inhibitor Rp-8-CPT-cAMPS. 6-Bnz-cAMP and 8-pCPT-2'-O-Me-cAMP induced GTP-loading of Rap1, but not of Rap2. Treatment of the cells with toxin B-1470 and U0126 significantly reduced bradykinin-induced IL-8 release alone or in combination with the activators of PKA and Epac. Interestingly, inhibition of PKA by Rp-8-CPT-cAMPS and silencing of Epac1 and Epac2 expression by specific siRNAs largely decreased activation of Rap1 and the augmentation of bradykinin-induced IL-8 release by both PKA and Epac.
Collectively, our data suggest that PKA, Epac1 and Epac2 act in concert to modulate inflammatory properties of airway smooth muscle via signaling to the Ras-like GTPase Rap1 and to ERK1/2.
Asthma and chronic obstructive pulmonary disease (COPD) are chronic inflammatory diseases characterized by structural and functional changes of the airways [1, 2]. The underlying pathogenic processes of asthma and COPD include the production and release of chemokines and cytokines by inflammatory and structural cells . Airway smooth muscle cells have recognized as immunomodulatory cells able to synthesize multiple inflammatory mediators such as cytokines, including interleukin-8 (IL-8) [4–6].
IL-8 represents one of the best characterized members of the family of chemokines known to attract and activate leukocytes and plays a major role in the initiation and maintenance of inflammatory responses . In particular, IL-8 is a potent chemoattractant for neutrophils and eosinophils [8, 9], that have been implicated in inflammatory airway diseases . Indeed, enhanced IL-8 has been detected in blood and bronchial mucosa  and in bronchial epithelial cells of patients with asthma , in bronchoalveolar lavage fluid (BALF) of asthmatic and chronic bronchitis patients , in BALF and sputum from patients with COPD [14, 15]. IL-8 levels correlate with the number of airway neutrophils, which are strongly associated with severe asthma and are increased during acute exacerbations of chronic bronchitis . Airway smooth muscle are a rich source of IL-8 . The gene expression of IL-8 is tightly regulated by inflammatory and pro-contractile agonists [6, 17, 18] acting on the large superfamily of G-protein-coupled receptors (GPCRs).
Bradykinin is a pluripotent nonapeptide generated by plasma and tissue kallikreins, and is upregulated in patients with asthma . It has been reported that bradykinin stimulates the expression of IL-8 in human lung fibroblasts and airway smooth muscle [6, 18]. This response is coupled to activation of extracellular signal-regulated protein kinases 1 and 2 (ERK1/2) [18, 20] and appears to involve cyclooxygenase-dependent and -independent signals [6, 21].
Gs-protein-coupled receptor activation (e.g. β2-adrenergic or prostanoid receptors) modulates the release of cytokines from airway cells , probably via activation of adenylyl cyclase and subsequent increase in intracellular cyclic AMP (cAMP). Importantly, a synergism between bradykinin and the cAMP-elevating agents salmeterol and prostaglandin E2 (PGE2) has been reported at the level of IL-6 production from airway smooth muscle . Although these studies clearly indicate a role for cAMP in pro-inflammatory cytokine production, the engagement of distinct cAMP-regulated effectors has not been yet addressed in the airways. Given the importance of the bradykinin- and the cAMP-driven pathways in both the pathophysiology and the treatment of pulmonary diseases, insights into the cellular mechanisms of their interaction are warranted.
Indeed, increasing evidence suggests that cAMP actively regulates transcription and gene expression events in several airway cells [23, 24], and that such mechanism may regulate local cytokine production in human airway smooth muscle . Until recently, intracellular effects of cAMP have been attributed to the activation of protein kinase A (PKA) and subsequent changes in PKA-mediated protein expression and function . In the last decade, exchange proteins directly activated by cAMP (Epac1 and Epac2) have been identified as cAMP-regulated guanine nucleotide exchange factors for Ras-like GTPases, such as Rap1 and Rap2 . Epac controls a variety of cellular functions including integrin-mediated cell-adhesion , endothelial integrity and permeability , exocytosis and insulin secretion [28, 29]. Epac also signals to ERK although the outcome of this particular signalling appears to depend on the cell type and specific cellular localization of Epac and their effectors [30–33]. Epac has been shown to act alone [34, 35] or to either antagonize [32, 36] or synergize with PKA [37, 38]. Although a role of Epac in lung fibroblasts and airway smooth muscle proliferation has recently been addressed [34, 35, 39], the impact of both PKA and Epac on the production of inflammatory mediators in the airways is presently unknown. Here, we report on novel cAMP-driven molecular mechanisms inducing augmentation of bradykinin-induced release of IL-8 from human airway smooth muscle and we demonstrate that Epac1 and Epac2 act in concert with PKA to modulate this cellular response via signaling to the Ras-like GTPase Rap1 and ERK1/2.
1,4-diamino-2,3-dicyano-1, 4-bis [2-aminophenylthio]butadiene (U0126) and forskolin were purchased from Tocris (Bristol, UK). 6-Bnz-cAMP, 8-pCPT-2'-O-Me-cAMP, Rp-8-CPT-cAMPS, Sp-8-pCPT-2'-O-Me-cAMPS and 8-pCPT-2'-O-Me-cGMP were from BIOLOG Life Science Institute (Bremen, Germany). Fenoterol was from Boehringer Ingelheim (Ingelheim, Germany). Bradykinin, Na3VO4, aprotinin, leupeptin, pepstatin and mouse anti-β-actin antibody (A5441), peroxidase-conjugated goat anti-rabbit (A5420) and peroxidase-conjugated rabbit anti-mouse (A9044) antibodies were purchased from Sigma-Aldrich (St. Louis, MO). The anti-phospho-ERK1/2 (P-ERK1/2) (9101), anti-ERK1/2 (9102) and anti-VASP which also binds to phospho-VASP (P-VASP) (3112) were from Cell Signaling Technology (Beverly, MA). The antibodies against Rap1 (121, sc-65), Rap2 (124, sc-164) and caveolin-1 (N-20, sc-894) were purchased from Santa Cruz Biotechnology (Santa Cruz, CA), and the antibody against Rac-1 (Mab 3735) was from Millipore (Billerica, MA). The mouse monoclonal antibodies against Epac1 and Epac2 were generated and kindly provided by Dr. J. L. Bos . Clostridium difficile toxin B-1470 was kindly provided by Drs C. von Eichel-Streiber and H. Genth. DMEM, FBS, penicillin/streptomycin solution were obtained from GIBCO-BRL Life Technologies (Paisley, UK). Alamar Blue solution was from Biosource (Camarillo, CA), the dyazo die trypan blue from Fluka Chemie (Buchs, Switzerland) and the Pierce BCA protein assay kit from Thermo Scientific (Rockford, IL). siRNA probes were purchased from Dharmacon Inc. (Lafayette, CO) and the transfection vehicle lipofectamine 2000 was from Invitrogen (Carlsbad, CA). The western lightning ECL solution was from PerkinElmer Inc. (Waltman, MA) and the IL-8 ELISA kit from Sanquin (Amsterdam, The Netherlands). All used chemicals were of analytical grade.
Cell culture, toxin treatment, cell number and viability measurements
Human bronchial smooth muscle cell lines, immortalized by stable ectopic expression of human telomerase reverse transcriptase enzyme were used for all the experiments (hTERT-airway smooth muscle cells). The primary human bronchial smooth muscle cells used to generate these cells were prepared as described previously . All procedures were approved by the human Research Ethics Board of the University of Manitoba. As described previously , each cell line was thoroughly characterized to passage 10 and higher. Passage 10 to 25 myocytes, grown on uncoated dishes in DMEM supplemented with antibiotics and 10% FBS, were used. Before each experiments, cells were serum deprived for one day in DMEM supplemented with antibiotics. For toxin B-1470 treatment, cells were treated for 24 hrs with 100 pg/ml toxin B-1470. Toxin-induced glucosylation of Ras-like GTPases was monitored by using a specific anti-Rac1 antibody , and changes in cell morphology were monitored by phase-contrast microscopy, using an Olympus IX50 microscope equipped with a digital image capture system (Color View Soft Imaging System). The toxicity of used drugs as well as their vehicle (DMSO) towards hTERT-airway smooth muscle cells was determined by an Alamar Blue assay. Briefly, cells were incubated with HBSS containing 10% vol/vol Alamar blue solution and then analyzed by fluorimetric analysis. Fluorescence derives from the conversion of Alamar blue into its reduced form by mitochondrial cytochromes and is therefore a measure of the number of cells. Viability was set as 100% in control cells. Viability of cells was also measured by resuspending cells 1:1 in the diazo dye trypan blue, which is absorbed by non viable cells, and the number of blue cells was then measured.
Cells were lysed in 50 mM Tris (pH 7.4) supplemented with 1 mM Na3VO4, 1 mM NaF, 10 μg/ml aprotinin, 10 μg/ml leupeptin and 7 μg/ml pepstatin and then fractioned as described earlier . The protein amount of all the fractions was determined using Pierce protein determination according to the manifacturer's instructions. Membrane, cytosolic and nuclear enriched fractions were subsequently used for detection of Epac1, Epac2, Rap1 and Rap2 expression.
Silencing of Epac1 and Epac2 expression using siRNAs
Cells were transfected with siRNA probes targeted to either Epac1 or Epac2; the target sequences for human Epac1 siRNA mixture were: sense: 5'-CGUGGGAACUCAUGAGAUG-3' (J-007676-05), sense: 5'-GGACCGAGAUGCCCAAUUC-3' (J-007676-06), sense: 5'-GAGCGUCUCUUUGUUGUCA-3' (J-007676-07), sense: 5'CGUGGUACAUUAUCUGGAA-3' (J-007676-08) and for the Epac2 siRNA mixture: sense: 5'-GAACACACCUCUCAUUGAA-3' (J-009511-05), sense: 5'- GGAGAAAUAUCGACAGUAU-3' (J-009511-06), sense: 5'-GCUCAAACCUAAUGAUGUU-3' (J-009511-07), sense: 5'-CAAGUUAGCACUAGUGAAU-3' (J-009511-08). Non-silencing siRNA control was used as a control in all siRNA transfection experiments. Cells were transfected with 200 pmol of appropriate siRNA by using lipofectamine 2000 (1 mg/ml) as vehicle. 6 hrs after transfection, cells were washed with DMEM supplemented with antibiotics to reduce toxicity effects of the transfection reagent. Cells were subsequently analyzed for Epac1 and Epac2 expression, GTP-loading of Rap1 or IL-8 production.
Activation of Rap1, phosphorylation of ERK1/2-VASP and immunoblot analysis
The amount of activated Rap1 and Rap2 was measured with the pull-down technique by using glutathione S-transferase (GST)-tagged RalGDS (Ras-binding domain of the Ral guanine nucleotide dissociation stimulator) as previously described . For the measurement of the phosphorylation of ERK1/2 and VASP, cell were lysed followed by determination of the protein concentration. Equal amounts of protein (or samples) were loaded on 10-15% polyacrylamide gels and analyzed for the protein of interest by using the specific first antibody (dilution Rap1 and Rap2 1:250, P-ERK 1:1000, ERK 1:500, VASP 1:1000) and the secondary HRP-conjugated antibody (dilution 1:2000 anti-rabbit or 1:3000 anti-mouse). Protein bands were subsequently visualized on film using western lightning plus-ECL and quantified by scanning densitometry using TotalLab software (Nonlinear Dynamics, Newcastle, UK). Results were normalized for protein levels by using specific control proteins.
The concentration of IL-8 in the culture medium was determined by ELISA according to the manifacturer's instructions (Sanquin, the Netherlands). Results were normalized for cell number according to Alamar Blue measurement. Basal IL-8 levels ranged between 0.3 and 18,8 pg/ml.
Data were expressed as the mean ± SEM of n determinations. Statistical analysis was performed using the statistical software Prism. Data were compared by using an unpaired or paired two-tailed Student's t test to determine significant differences. p values < 0.05 were considered to be statistically significant.
Cyclic AMP-regulated PKA and Epac augment bradykinin-induced IL-8 release from human airway smooth muscle
Given the importance of IL-8 in airway inflammatory processes , we examined the role of the cAMP-elevating agent β2-agonist fenoterol in bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells. As illustrated in Fig. 1A, bradykinin induced an increase in the release of IL-8 from the cells. The concentration of 10 μM bradykinin appeared to be most effective (~2-fold increase, P < 0.001) and was chosen for further experiments. The β2-agonist fenoterol at the concentration of 1 μM further enhanced bradykinin-induced IL-8 release of about 2 fold (P < 0.05), whereas it did not alter basal IL-8 production (Fig. 1B). These data suggest that bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells may be augmented by cAMP signaling.
To study whether cAMP-regulated effectors PKA and Epac participate in this response, we analyzed the role of the cAMP analogs 6-Bnz-cAMP and 8-pCPT-2'-O-Me-cAMP known to preferentially activate PKA or Epac, respectively [46, 47]. As shown in Fig. 2, direct activation of PKA by 6-Bnz-cAMP induced a concentration-dependent augmentation of bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells. 500 μM 6-Bnz-cAMP induced about a 3.5-fold (P < 0.01) increase on bradykinin-induced IL-8 release (Fig. 2). As shown for fenoterol, 6-Bnz-cAMP did not enhance basal cellular IL-8 production at any concentration measured (Fig. 2). We report here that hTERT-airway smooth muscle cells express Epac1 and Epac2 (See later). Therefore, we also used the Epac activator 8-pCPT-2'-O-Me-cAMP to modulate bradykinin-induced IL-8 release. As shown in Fig. 3A, treatment of the cells with 8-pCPT-2'-O-Me-cAMP induced a concentration-dependent augmentation of this response. 100 μM 8-pCPT-2'-O-Me-cAMP increased bradykinin-induced IL-8 release by about 2-fold (P < 0.01) (Fig. 3A). Similar to both the β2-agonist fenoterol and the PKA activator 6-Bnz-cAMP, the Epac activator 8-pCPT-2'-O-Me-cAMP did not increase basal IL-8 production at any concentration used (Fig. 3A). To validate the data obtained with the Epac activator 8-pCPT-2'-O-Me-cAMP, 8-pCPT-2'-O-Me-cGMP, a cGMP analogue with substitutions identical to those in 8-pCPT-2'-O-Me-cAMP which is known to neither activate protein kinase G nor Epac , was used as a negative control. Moreover, Sp-8-pCPT-2'-O-Me-cAMPS, a phosphorothioate derivative of 8-pCPT-2'-O-Me-cAMP that is resistant to phosphodiesterase hydrolysis [47, 48], was used as an additional Epac activator. Importantly, Sp-8-pCPT-2'-O-Me-cAMPS (100 μM) mimicked the effects of the Epac activator 8-pCPT-2'-O-Me-cAMP on bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells (P < 0.05), whereas the negative control 8-pCPT-2'-O-Me-cGMP (100 μM) did not alter this response (Fig. 3B). Again, as shown for the Epac activator 8-pCPT-2'-O-Me-cAMP, Sp-8-pCPT-2'-O-Me-cAMPS and 8-pCPT-2'-O-Me-cGMP did not alter basal IL-8 release (Fig. 3B). Collectively, these data indicate that augmentation of bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells is regulated by cAMP, likely through both PKA and Epac.
To further validate our findings, we analyzed the phosphorylation of VASP, known to be phosphorylated at Ser-157, a PKA-specific site , by using a VASP-specific antibody that recognizes both phospho-VASP (upper band) and total VASP (lower band). Phosphorylation of VASP was not altered by any of the Epac-related cAMP compounds being studied (each 100 μM) (Fig. 4A). In contrast, 1 μM fenoterol, 100 μM forskolin and 500 μM 6-Bnz-cAMP induced VASP phosphorylation (Fig. 4A). In addition, treatment of the cells with the pharmacological selective PKA inhibitor Rp-8-CPT-cAMPS blocked phosphorylation of VASP by 6-Bnz-cAMP (P < 0.05) and largely reduced VASP phosphorylation by forskolin (P = 0.067) and fenoterol (P < 0.05) (Fig. 4B). Bradykinin also induced VASP phosphorylation (P = 0.055) (Fig. 4B). All together, these data indicate that the cyclic nucleotides used in our study specifically activate their primary pharmacological targets PKA and Epac, and thereby induce augmentation of bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells.
Role of Ras-like GTPases in cAMP-dependent bradykinin-induced IL-8 release from human airway smooth muscle
PKA and Epac have been reported to modulate GTP-loading of the Ras-like GTPase Rap1 and Rap2 [45, 50, 51]. In hTERT-airway smooth muscle cells, Rap1 and Rap2 were both present at membrane-associated and cytosolic compartments (Fig. 5). As shown in Fig. 5A, activation of Epac by 8-pCPT-2'-O-Me-cAMP induced about a 2-fold increase in GTP-loading of Rap1 in hTERT-airway smooth muscle cells (P < 0.01). Activation of PKA by 6-Bnz-cAMP activated Rap1 by about 1,5-fold (P < 0.05) (Fig. 5A). In contrast, activation of Epac or PKA did not induce GTP-loading of Rap2 (Fig. 5B). To study whether activation of Ras-like GTPases by cAMP is required for the augmentation of bradykinin-induced IL-8 release, cells were treated with Clostridium difficile toxin B-1470 known to inactivate Ras family members, including Rap1 . We analyzed cell morphology and immunoreactivity of the toxin-substrate GTPase Rac1 to monitor the functionality of toxin B-1470 . Treatment of the cells with 100 pg/ml toxin B-1470 profoundly altered cell morphology, as demonstrated by the occurrence of a high number of rounded cells (Fig. 6A). Toxin B-1470 also completely abolished Rac1 immunoreactivity under any experimental condition studied (not shown). Although hTERT-airway smooth muscle cells were toxin B-1470 sensitive, toxin treatment lowered cell number only of about 20% (Fig. 6B, upper panel) and did not alter cell viability (not shown). Importantly, toxin treatment completely reversed the augmentation of bradykinin-induced IL-8 release by 8-pCPT-2'-O-Me-cAMP and 6-Bnz-cAMP (each P < 0.05), without affecting IL-8 release by bradykinin alone (Fig. 6B, lower panel). As we show that PKA and Epac induce GTP-loading of Rap1 and that inhibition of Ras-like GTPases, including Rap1, largely affect augmentation of bradykinin-induced IL-8 release by both PKA and Epac, our data point at Rap1 as an important modulator of this response.
Role of ERK1/2 in cAMP-dependent bradykinin-induced IL-8 release from human airway smooth muscle
Although the activation of ERK1/2 by Epac and PKA still remain controversial [51, 53], some reports have shown that this might occur via Rap1 [32, 51, 54]. Current evidence also indicates that ERK1/2 regulates the expression of cytokines induced by several stimuli, including bradykinin, via activation of specific transcription factors [18, 22]. To investigate whether ERK1/2 is required for the Epac- and PKA-mediated augmentation of bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells, we first studied the phosphorylation of ERK1/2 in these cells by 8-pCPT-2'-O-Me-cAMP and 6-Bnz-cAMP. As shown in Fig. 7A, activation of Epac and PKA induced marked phosphorylation of both ERK1 and ERK2. In agreement with earlier studies [18, 20], treatment with bradykinin also induced ERK1/2 phosphorylation and such stimulatory effect was further enhanced by co-stimulation with 8-pCPT-2'-O-Me-cAMP and 6-Bnz-cAMP (P = 0.06 and P = 0.11, respectively) (Fig. 7B). Importantly, as shown in Fig. 7C, treatment with toxin B-1470 significantly reduced ERK1/2 phosphorylation by 8-pCPT-2'-O-Me-cAMP (P < 0.05) and 6-Bnz-cAMP (P < 0.01). Thus, it is reasonable to assume that cAMP-dependent GTPase activation lies upstream of ERK1/2 activation in hTERT-airway smooth muscle cells. To investigate the impact of ERK1/2 on the augmentation of bradykinin-induced IL-8 release by PKA and Epac, cells were treated with U0126, a selective pharmacological inhibitor of the upstream kinase of ERK1/2, mitogen-activated protein kinase kinase (MEK) . As expected, U0126 largely diminished phosphorylation of ERK1/2 under any experimental condition used (P < 0.001) (Fig. 8A). As illustrated in Fig. 8B, augmentation of bradykinin-induced IL-8 release by 6-Bnz-cAMP and 8-pCPT-2'-O-Me-cAMP was drastically impaired (P < 0.01 and P < 0.05, respectively) by MEK inhibition. As expected, treatment with U0126 also reduced bradykinin-induced IL-8 release (Fig. 8B), confirming that ERK1/2 is an important effector regulating IL-8 production. More important, our data highlight the role of ERK1/2 in augmenting bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells by PKA and Epac.
PKA and Epac cooperate to activate Rap1 and to augment bradykinin-induced IL-8 release from human airway smooth muscle
Studies on the molecular mechanisms of cAMP-related signaling demonstrate that the classical cAMP effector PKA acts alone or in concert with the novel cAMP sensor Epac [25, 56, 57]. To study whether cAMP-regulated PKA and Epac might cooperate to augment bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells, we stimulated the cells with 6-Bnz-cAMP in the presence of 8-pCPT-2'-O-Me-cAMP and vice versa. The effect of 50 μM 6-Bnz-cAMP on bradykinin-induced IL-8 release was modulated by 8-pCPT-2'-O-Me-cAMP (Fig. 9A), the most prominent effect being observed at 30 μM 8-pCPT-2'-O-Me-cAMP. In addition, the effects of 10 μM 8-pCPT-2'-O-Me-cAMP on bradykinin-induced IL-8 release were enhanced in the presence of 6-Bnz-cAMP and the maximal response was observed at 100 μM 6-Bnz-cAMP (Fig. 9B). To further validate PKA and Epac cooperative effects, we used different approaches to specifically inhibit the two cAMP-driven effectors and we studied the impact of these inhibitions on GTP-loading of Rap1 and IL-8 release from hTERT-airway smooth muscle cells.
As shown before, Rp-8-CPT-cAMPS acts as a specific inhibitor of PKA in hTERT-airway smooth muscle cells. Interestingly, treatment of cells with Rp-8-CPT-cAMPS reduced GTP-loading of Rap1 by both 8-pCPT-2'-O-Me-cAMP and 6-Bnz-cAMP (Fig. 10A). In addition, in the presence of Rp-8-CPT-cAMPS, augmentation of bradykinin-induced IL-8 release by the PKA activator 6-Bnz-cAMP and the Epac activator 8-pCPT-2'-O-Me-cAMP was largely diminished (P < 0.05), whereas basal and bradykinin-induced IL-8 release were not significantly altered (Fig. 10B). These data suggest that PKA and Epac pathways work in concert both at the level of Rap1 activation and the downstream production of IL-8.
At present, highly specific pharmacological inhibitors of individual Epac isoforms, Epac1 and Epac2, are not available . Thus, to more precisely study the role of Epac1 and Epac2 in specific functions, siRNA is generally used to suppress their endogenous expression [31, 34–36]. As illustrated in Fig. 11A, the siRNA approaches were effective in reducing expression of membrane-associated Epac1 and cytosolic Epac2 of about ~40% (P < 0.01 for Epac1 and for Epac2) leaving the expression of the cell fraction-specific marker proteins caveolin-1 and β-actin unaffected. Silencing of Epac1 and Epac2 was most efficient 72 hrs after transfection, indicating that the proteins exhibit a slow turn-over rate in hTERT-airway smooth muscle cells. As illustrated in Fig. 11B, silencing of Epac1 and Epac2 did not only reduced GTP-loading of Rap1 by 8-pCPT-2'-O-Me-cAMP, but also its activation by 6-Bnz-cAMP. In addition, silencing of Epac1 and Epac2 severely impaired augmentation of bradykinin-induced IL-8 release by 8-pCPT-2'-O-Me-cAMP (each P < 0.05), whereas basal and bradykinin-induced IL-8 release were again not significantly changed (Fig. 11C). Intriguingly, silencing of Epac1 also significantly reduced augmentation of bradykinin-induced IL-8 release by 6-Bnz-cAMP (P < 0.05) (Fig. 11C). Silencing of cellular Epac2 appeared to modestly reduce the PKA-mediated IL-8 response, although this effect was not significant (P = 0.075) (Fig. 11C). Taken together, these data indicate that cAMP-regulated PKA and Epac (Epac1 and Epac2) are interconnected with regard to the activation of Rap1 and the cellular production of IL-8 in hTERT-airway smooth muscle cells.
Bradykinin is known to enhance the expression of several cytokines in airway smooth muscle [18, 58]. cAMP-elevating agents also modulate release of cytokines from airway sources including airway smooth muscle . For example, prostaglandin E2 (PGE2) was shown to increase IL-8 production in airway smooth muscle cells . Interestingly, salmeterol and PGE2 have been reported to augment bradykinin-induced production of IL-6 by airway smooth muscle , but the cAMP-regulated targets responsible for this cellular response have not been identified. Here we report on novel cAMP-dependent mechanisms that augment bradykinin-induced release of IL-8 from airway smooth muscle. We demonstrate that augmentation of bradykinin-induced IL-8 production by cAMP signaling requires the cooperative action of PKA and Epac, leading subsequently to the activation of Ras-like GTPases such as Rap1 and ERK1/2 (Fig. 12).
The use of cyclic nucleotide analogs as pharmacological tools to study the specific effects of cAMP-driven signaling is now widely accepted . However, studies indicated that various cyclic nucleotide analogs, including 6-Bnz-cAMP and 8-pCPT-2'-O-Me-cAMP might, in addition to their primary effects, also cause elevation of cAMP or cGMP upon inhibition of phosphodiesterases  or act upon production of cAMP hydrolysis products . We did not observe indirect activation of the PKA-dependent effectors such as VASP by any of the Epac-related analogs. Moreover, phosphorylation of VASP by forskolin, fenoterol and 6-Bnz-cAMP was sensitive to the PKA inhibitor Rp-8-CPT-cAMPS. Both the PKA activator 6-Bnz-cAMP and the Epac activators used (8-pCPT-2'-O-Me-cAMP and Sp-8-pCPT-2'-O-Me-cAMPS) augmented bradykinin-induced IL-8 release in the cells, whereas no alteration of the cellular IL-8 levels was observed with the cGMP analog 8-pCPT-2'-O-Me-cGMP. Hence, it is reasonable to assume that PKA- and Epac-related cyclic nucleotides act via their primary pharmacological targets. Collectively, our results indicate that cAMP-dependent augmentation of bradykinin-induced IL-8 release from hTERT-airway smooth muscle cells is regulated by both PKA and Epac.
In agreement with studies in human airway smooth muscle , the β2-agonist fenoterol and the distinct PKA/Epac-related cyclic nucleotide analogs used in our studies solely alter the release of IL-8 from hTERT-airway smooth muscle in the presence of bradykinin, suggesting that this GPCR ligand might also directly affect the cAMP pathway. Previous studies have shown that bradykinin can increase intracellular levels of cAMP in airway smooth muscle via induction of cyclooxygenase and subsequent production of PGE2 . As we observed phosphorylation of VASP by bradykinin already ≤ 15 minutes, such prostanoid-driven indirect effects may not account for the bradykinin responses observed in our study. Protein kinase C, a major downstream effector of bradykinin, has been reported to activate type II adenylyl cyclase (AC) in intact cells and to elicit activation of basal AC activity . The type II AC isoform is abundantly expressed in airway smooth muscle and is activated by both Gαs and PKC probably leading to synergistic cAMP formation [62, 63]. Moreover, PKC may cooperate in assembling the prostanoid synthetic machinery . In addition, it has been reported that bradykinin inhibits approximately 60% of the total cAMP phosphodiesterase activity in guinea-pig airway smooth muscle . The above mentioned mechanisms could therefore contribute to the increase of cAMP levels by bradykinin in distinct subcellular compartments and subsequently trigger the activation of PKA and Epac in airway smooth muscle.
Here we also focused on the Ras-like GTPase family members Rap1 and Rap2 as the main effectors of Epac being identified [25, 64] and so far the best described in their functional association to Epac . Indeed, both Rap1 and Rap2 are present in hTERT-airway smooth muscle cells in both membrane and cytosolic compartments. Interestingly, activation of PKA and Epac induced GTP-loading of Rap1 in hTERT-airway smooth muscle; both cAMP effectors did not alter basal Rap2 activity. In contrast to Epac1, activation of Rap1 by PKA has been reported to occur mostly indirectly. Evidence suggests that PKA might either activate the Rap1 exchange factor C3G (Crk Src homology domain 3) and Src [51, 54, 65] or inhibit the Rap1-GTPase activating protein . However, it is presently unknown whether such mechanisms are operational in hTERT-airway smooth muscle. To address the role of Ras-like GTPases in bradykinin-induced IL-8 release we used the bacterial toxin B-1470. Toxin B-1470, which is produced by C. difficile strain 1470, inhibits exclusively the Rac protein from the Rho family and, in addition, Rap and Ral proteins from the Ras family of GTPases via glucosylation . Such GTPases are important regulators of cellular adhesion and migration. Indeed, treatment with the toxin induced morphological changes and also caused cell detachment probably associated with inhibition of those GTPases. Toxin treatment only slightly reduced cell number and did not alter cell viability. Importantly, we observed a drastic reduction of bradykinin-induced IL-8 release by PKA and Epac after incubation with Toxin B-1470. Hence, our results suggest that cAMP-dependent augmentation of bradykinin-induced IL-8 requires PKA- and Epac-dependent activation of GTPases, and based on the results presented herein, Rap1 represents a very attractive candidate.
The production and release of IL-8 from airway smooth muscle upon stimulation of pro-inflammatory agonists is regulated by gene transcription and protein expression events . Bradykinin has been shown to modulate the release of IL-8 generally upon activation of distinct signals including ERK1/2 [18, 20]. Phosphorylation of ERK1/2 by bradykinin occurs acutely between 5-30 min in both human airway smooth muscle cells  and human lung fibroblasts . It is generally believed that cAMP modulates transcription and protein expression [23, 67], and its effects have been attributed to the phosphorylation of cAMP response element binding (CREB) protein by PKA and its subsequent binding to the CRE promoter of the specific genes . Although the human IL-8 promoter does contain a CRE region, activation of CREB has not been related to the regulation of IL-8 expression in airway cells. Moreover, recent studies indicate that Epac1 also modulates gene transcription and protein expression by inducing the transcription factors CCAAT/Enhancer-binding Proteins (C/EBPs) in COS-1 cells . Interestingly, both PKA and Epac have been reported to activate ERK1/2 in a cell-type specific manner . Once activated, ERK1/2 signals to the nucleus, promoting transcription of genes usually associated with inflammation and proliferation. Activation of Epac and PKA in hTERT-airway smooth muscle cells increased basal ERK1/2 phosphorylation (1-30 min) and enhanced bradykinin-induced ERK1/2 phosphorylation measured after 10 min. Hence, these findings indicate that ERK1/2 activation may be an important mechanism by which β2-agonists augment IL-8 production in airway smooth muscle. This was confirmed by the fact that treatment with the pharmacologic inhibitor U0126 reduced the IL-8 release by bradykinin alone and even in a more pronounced way, by the combination of bradykinin with both 8-pCPT-2'-O-Me-cAMP and 6-Bnz-cAMP. The fact that toxin B-1470 treatment largely impaired ERK1/2 phosphorylation by PKA and Epac, most likely places ERK1/2 downstream of toxin B-1470-sensitive GTPases.
Previous studies in human lung fibroblasts have shown that Epac1, Epac2 and PKA act independently on distinct cellular functions [34, 35]. For example, the anti-proliferative signalling properties in human lung fibroblasts have been assigned to Epac1, but not to Epac2 [34, 35]. The diverse effects of Epac proteins and PKA could be explained by their different subcellular localization  or downstream effector availability [70, 71]. Indeed, we observed that Epac isoforms Epac1 and Epac2 exhibit different cellular localization in hTERT-airway smooth muscle cells, the former being more expressed at the plasma membrane and the latter in the cytosolic fraction of the cells. However, we here demonstrate that silencing of Epac1 or Epac2 expression in hTERT-airway smooth muscle cells abolished the augmentation of bradykinin-induced IL-8 release by the Epac activator 8-pCPT-2'-O-Me-cAMP, and also largely diminished the enhancement of this cellular response by the PKA activator 6-Bnz-cAMP. These data point at a positive cooperativity between cAMP-regulated Epac1-Epac2 and PKA, which was confirmed by pharmacological approaches using the PKA inhibitor Rp-8-CPT-cAMPS and the combinations of the the PKA and Epac activators. Importantly, activation of Rap1 by either PKA or Epac appeared to be sensitive to inhibition of PKA by Rp-8-CPT-cAMPS or to silencing of Epac1 and Epac2 by siRNA. This results suggest that Epac and PKA work in concert to activate Rap1 and subsequently augment IL-8 release by bradykinin. Our findings might implicate that both Epac isoforms and PKA bind to the same signalling complex which are then directed to the same target(s). Indeed, distinct intracellular cAMP signaling compartments have been recently identified in primary cultures of neonatal cardiac ventriculocytes  and cAMP-responsive multiprotein complexes including PKA and Epac1-Epac2 seem to confer signaling specificity [73, 74]. Thus, our data indicate that in airway smooth muscle both Epac1 and Epac2 act in concert with PKA to modulate pro-inflammatory signaling properties.
We describe novel cAMP-dependent mechanisms to induce augmentation of bradykinin-induced IL-8 release from airway smooth muscle. Evidence is provided that cAMP-regulated Epac1 and Epac2 cooperate with PKA to induce Ras-like GTPases activation (presumably Rap1) and subsequent activation of ERK1/2. Our findings implicate that PKA, Epac1 and Epac2 exert pro-inflammatory signaling properties in human airway smooth muscle depending on the input of distinct GPCR signals. The relevance of these findings is reflected by the importance of bradykinin- and cAMP-mediated signals in airway disease pathogenesis and treatment and opens new avenues for future therapeutic intervention.
Bousquet J, Jeffery PK, Busse WW, Johnson M, Vignola AM: Asthma. From bronchoconstriction to airways inflammation and remodeling. Am J Respir Crit Care Med 2000, 161:1720–1745.
Jeffery PK: Remodeling in asthma and chronic obstructive lung disease. Am J Respir Crit Care Med 2001, 164:S28-S38.
Barnes PJ: The cytokine network in asthma and chronic obstructive pulmonary disease. J Clin Invest 2008, 118:3546–3556.
Halayko AJ, Solway J: Molecular mechanisms of phenotypic plasticity in smooth muscle cells. J Appl Physiol 2001, 90:358–368.
Panettieri RA Jr: Airway smooth muscle: immunomodulatory cells that modulate airway remodeling? Respir Physiol Neurobiol 2003, 137:277–293.
Pang L, Knox AJ: Bradykinin stimulates IL-8 production in cultured human airway smooth muscle cells: role of cyclooxygenase products. J Immunol 1998, 161:2509–2515.
Baggiolini M, Dewald B, Moser B: Interleukin-8 and related chemotactic cytokines--CXC and CC chemokines. Adv Immunol 1994, 55:97–179.
Kunkel SL, Standiford T, Kasahara K, Strieter RM: Interleukin-8 (IL-8): the major neutrophil chemotactic factor in the lung. Exp Lung Res 1991, 17:17–23.
Shute J: Interleukin-8 is a potent eosinophil chemo-attractant. Clin Exp Allergy 1994, 24:203–206.
Richman-Eisenstat JB, Jorens PG, Hebert CA, Ueki I, Nadel JA: Interleukin-8: an important chemoattractant in sputum of patients with chronic inflammatory airway diseases. Am J Physiol 1993, 264:L413-L418.
Shute JK, Vrugt B, Lindley IJ, Holgate ST, Bron A, Aalbers R, Djukanovic R: Free and complexed interleukin-8 in blood and bronchial mucosa in asthma. Am J Respir Crit Care Med 1997, 155:1877–1883.
Marini M, Vittori E, Hollemborg J, Mattoli S: Expression of the potent inflammatory cytokines, granulocyte-macrophage-colony-stimulating factor and interleukin-6 and interleukin-8, in bronchial epithelial cells of patients with asthma. J Allergy Clin Immunol 1992, 89:1001–1009.
Chanez P, Enander I, Jones I, Godard P, Bousquet J: Interleukin 8 in bronchoalveolar lavage of asthmatic and chronic bronchitis patients. Int Arch Allergy Immunol 1996, 111:83–88.
Tanino M, Betsuyaku T, Takeyabu K, Tanino Y, Yamaguchi E, Miyamoto K, Nishimura M: Increased levels of interleukin-8 in BAL fluid from smokers susceptible to pulmonary emphysema. Thorax 2002, 57:405–411.
Yamamoto C, Yoneda T, Yoshikawa M, Fu A, Tokuyama T, Tsukaguchi K, Narita N: Airway inflammation in COPD assessed by sputum levels of interleukin-8. Chest 1997, 112:505–510.
Gompertz S, O'Brien C, Bayley DL, Hill SL, Stockley RA: Changes in bronchial inflammation during acute exacerbations of chronic bronchitis. Eur Respir J 2001, 17:1112–1119.
Fong CY, Pang L, Holland E, Knox AJ: TGF-beta1 stimulates IL-8 release, COX-2 expression, and PGE(2) release in human airway smooth muscle cells. Am J Physiol Lung Cell Mol Physiol 2000, 279:L201-L207.
Hayashi R, Yamashita N, Matsui S, Fujita T, Araya J, Sassa K, Arai N, Yoshida Y, Kashii T, Maruyama M, Sugiyama E, Kobayashi M: Bradykinin stimulates IL-6 and IL-8 production by human lung fibroblasts through ERK- and p38 MAPK-dependent mechanisms. Eur Respir J 2000, 16:452–458.
Christiansen SC, Proud D, Sarnoff RB, Juergens U, Cochrane CG, Zuraw BL: Elevation of tissue kallikrein and kinin in the airways of asthmatic subjects after endobronchial allergen challenge. Am Rev Respir Dis 1992, 145:900–905.
Pyne NJ, Tolan D, Pyne S: Bradykinin stimulates cAMP synthesis via mitogen-activated protein kinase-dependent regulation of cytosolic phospholipase A2 and prostaglandin E2 release in airway smooth muscle. Biochem J 1997,328(Pt 2):689–694.
Zhu YM, Bradbury DA, Pang L, Knox AJ: Transcriptional regulation of interleukin (IL)-8 by bradykinin in human airway smooth muscle cells involves prostanoid-dependent activation of AP-1 and nuclear factor (NF)-IL-6 and prostanoid-independent activation of NF-kappaB. J Biol Chem 2003, 278:29366–29375.
Huang CD, Tliba O, Panettieri RA Jr, Amrani Y: Bradykinin induces interleukin-6 production in human airway smooth muscle cells: modulation by Th2 cytokines and dexamethasone. Am J Respir Cell Mol Biol 2003, 28:330–338.
Kaur M, Holden NS, Wilson SM, Sukkar MB, Chung KF, Barnes PJ, Newton R, Giembycz MA: Effect of beta2-adrenoceptor agonists and other cAMP-elevating agents on inflammatory gene expression in human ASM cells: a role for protein kinase A. Am J Physiol Lung Cell Mol Physiol 2008, 295:L505-L514.
Penn RB, Benovic JL: Regulation of heterotrimeric G protein signaling in airway smooth muscle. Proc Am Thorac Soc 2008, 5:47–57.
Roscioni SS, Elzinga CR, Schmidt M: Epac: effectors and biological functions. Naunyn Schmiedebergs Arch Pharmacol 2008, 377:345–357.
Rangarajan S, Enserink JM, Kuiperij HB, de RJ, Price LS, Schwede F, Bos JL: Cyclic AMP induces integrin-mediated cell adhesion through Epac and Rap1 upon stimulation of the beta 2-adrenergic receptor. J Cell Biol 2003, 160:487–493.
Cullere X, Shaw SK, Andersson L, Hirahashi J, Luscinskas FW, Mayadas TN: Regulation of vascular endothelial barrier function by Epac, a cAMP-activated exchange factor for Rap GTPase. Blood 2005, 105:1950–1955.
Kashima Y, Miki T, Shibasaki T, Ozaki N, Miyazaki M, Yano H, Seino S: Critical role of cAMP-GEFII--Rim2 complex in incretin-potentiated insulin secretion. J Biol Chem 2001, 276:46046–46053.
Fujimoto K, Shibasaki T, Yokoi N, Kashima Y, Matsumoto M, Sasaki T, Tajima N, Iwanaga T, Seino S: Piccolo, a Ca2+ sensor in pancreatic beta-cells. Involvement of cAMP-GEFII.Rim2.Piccolo complex in cAMP-dependent exocytosis. J Biol Chem 2002, 277:50497–50502.
Dodge-Kafka KL, Soughayer J, Pare GC, Carlisle Michel JJ, Langeberg LK, Kapiloff MS, Scott JD: The protein kinase A anchoring protein mAKAP coordinates two integrated cAMP effector pathways. Nature 2005, 437:574–578.
Fang Y, Olah ME: Cyclic AMP-dependent, protein kinase A-independent activation of extracellular signal-regulated kinase 1/2 following adenosine receptor stimulation in human umbilical vein endothelial cells: role of exchange protein activated by cAMP 1 (Epac1). J Pharmacol Exp Ther 2007, 322:1189–1200.
Kiermayer S, Biondi RM, Imig J, Plotz G, Haupenthal J, Zeuzem S, Piiper A: Epac activation converts cAMP from a proliferative into a differentiation signal in PC12 cells. Mol Biol Cell 2005, 16:5639–5648.
Wang Z, Dillon TJ, Pokala V, Mishra S, Labudda K, Hunter B, Stork PJ: Rap1-mediated activation of extracellular signal-regulated kinases by cyclic AMP is dependent on the mode of Rap1 activation. Mol Cell Biol 2006, 26:2130–2145.
Haag S, Warnken M, Juergens UR, Racke K: Role of Epac1 in mediating anti-proliferative effects of prostanoid EP(2) receptors and cAMP in human lung fibroblasts. Naunyn Schmiedebergs Arch Pharmacol 2008,378(6):617–30.
Huang SK, Wettlaufer SH, Chung J, Peters-Golden M: Prostaglandin E2 Inhibits Specific Lung Fibroblast Functions Via Selective Actions of PKA and Epac-1. Am J Respir Cell Mol Biol 2008. 2008–0080OC
Huston E, Lynch MJ, Mohamed A, Collins DM, Hill EV, MacLeod R, Krause E, Baillie GS, Houslay MD: EPAC and PKA allow cAMP dual control over DNA-PK nuclear translocation. Proc Natl Acad Sci USA 2008, 105:12791–12796.
Petersen RK, Madsen L, Pedersen LM, Hallenborg P, Hagland H, Viste K, Doskeland SO, Kristiansen K: Cyclic AMP (cAMP)-mediated stimulation of adipocyte differentiation requires the synergistic action of Epac- and cAMP-dependent protein kinase-dependent processes. Mol Cell Biol 2008, 28:3804–3816.
Hochbaum D, Hong K, Barila G, Ribeiro-Neto F, Altschuler DL: Epac, in synergy with cAMP-dependent protein kinase (PKA), is required for cAMP-mediated mitogenesis. J Biol Chem 2008, 283:4464–4468.
Kassel KM, Wyatt TA, Panettieri RA Jr, Toews ML: Inhibition of human airway smooth muscle cell proliferation by beta 2-adrenergic receptors and cAMP is PKA independent: evidence for EPAC involvement. Am J Physiol Lung Cell Mol Physiol 2008, 294:L131-L138.
Kooistra MRH, Corada M, Dejana E, Bos JL: Epac1 regulates integrity of endothelial cell junctions through VE-cadherin. FEBS Letters 2005, 579:4966–4972.
Gosens R, Stelmack GL, Dueck G, McNeill KD, Yamasaki A, Gerthoffer WT, Unruh H, Gounni AS, Zaagsma J, Halayko AJ: Role of caveolin-1 in p42/p44 MAP kinase activation and proliferation of human airway smooth muscle. Am J Physiol Lung Cell Mol Physiol 2006, 291:L523-L534.
Gosens R, Dueck G, Gerthoffer WT, Unruh H, Zaagsma J, Meurs H, Halayko AJ: p42/p44 MAP kinase activation is localized to caveolae-free membrane domains in airway smooth muscle. Am J Physiol Lung Cell Mol Physiol 2007, 292:L1163-L1172.
Genth H, Huelsenbeck J, Hartmann B, Hofmann F, Just I, Gerhard R: Cellular stability of Rho-GTPases glucosylated by Clostridium difficile toxin B. FEBS Lett 2006, 580:3565–3569.
Nunes RO, Schmidt M, Dueck G, Baarsma H, Halayko AJ, Kerstjens HA, Meurs H, Gosens R: GSK-3/beta-catenin signaling axis in airway smooth muscle: role in mitogenic signaling. Am J Physiol Lung Cell Mol Physiol 2008, 294:L1110-L1118.
Schmidt M, Evellin S, Weernink PA, von DF, Rehmann H, Lomasney JW, Jakobs KH: A new phospholipase-C-calcium signalling pathway mediated by cyclic AMP and a Rap GTPase. Nat Cell Biol 2001, 3:1020–1024.
Holz GG, Chepurny OG, Schwede F: Epac-selective cAMP analogs: new tools with which to evaluate the signal transduction properties of cAMP-regulated guanine nucleotide exchange factors. Cell Signal 2008, 20:10–20.
Poppe H, Rybalkin SD, Rehmann H, Hinds TR, Tang XB, Christensen AE, Schwede F, Genieser HG, Bos JL, Doskeland SO, Beavo JA, Butt E: Cyclic nucleotide analogs as probes of signaling pathways. Nat Methods 2008, 5:277–278.
Laxman S, Riechers A, Sadilek M, Schwede F, Beavo JA: Hydrolysis products of cAMP analogs cause transformation of Trypanosoma brucei from slender to stumpy-like forms. Proc Natl Acad Sci USA 2006, 103:19194–19199.
Smolenski A, Bachmann C, Reinhard K, Hõnig-Liedl P, Jarchau T, Hoschuetzky H, Walter U: Analysis and regulation of vasodilator-stimulated phosphoprotein serin 239 phosphorylation in vitro and in intact cells using a phosphospecific monoclonal antibody. J Biol Chem 1998, 273:20029–20035.
Kawasaki H, Springett GM, Mochizuki N, Toki S, Nakaya M, Matsuda M, Housman DE, Graybiel AM: A family of cAMP-binding proteins that directly activate Rap1. Science 1998, 282:2275–2279.
Stork PJ, Schmitt JM: Crosstalk between cAMP and MAP kinase signaling in the regulation of cell proliferation. Trends Cell Biol 2002, 12:258–266.
Schmidt M, Voss M, Thiel M, Bauer B, Grannass A, Tapp E, Cool RH, de GJ, von Eichel-Streiber C, Jakobs KH: Specific inhibition of phorbol ester-stimulated phospholipase D by Clostridium sordellii lethal toxin and Clostridium difficile toxin B-1470 in HEK-293 cells. Restoration by Ral GTPases. J Biol Chem 1998, 273:7413–7422.
Enserink JM, Christensen AE, de RJ, van TM, Schwede F, Genieser HG, Doskeland SO, Blank JL, Bos JL: A novel Epac-specific cAMP analogue demonstrates independent regulation of Rap1 and ERK. Nat Cell Biol 2002, 4:901–906.
Obara Y, Labudda K, Dillon TJ, Stork PJ: PKA phosphorylation of Src mediates Rap1 activation in NGF and cAMP signaling in PC12 cells. J Cell Sci 2004, 117:6085–6094.
Favata MF, Horiuchi KY, Manos EJ, Daulerio AJ, Stradley DA, Feeser WS, van Dyk DE, Pitts WJ, Earl RA, Hobbs F, Copeland RA, Magolda RL, Scherle PA, Trzaskos JM: Identification of a novel inhibitor of mitogen-activated protein kinase kinase. J Biol Chem 1998, 273:18623–18632.
Borland G, Smith BO, Yarwood SJ: EPAC proteins transduce diverse cellular actions of cAMP. Br J Pharmacol 2009,158(1):70–86.
Bos JL: Epac proteins: multi-purpose cAMP targets. Trends Biochem Sci 2006, 31:680–686.
Paegelow I, Werner H, Vietinghoff G, Wartner U: Release of cytokines from isolated lung strips by bradykinin. Inflamm Res 1995, 44:306–311.
Ammit AJ, Hoffman RK, Amrani Y, Lazaar AL, Hay DW, Torphy TJ, Penn RB, Panettieri RA Jr: Tumor necrosis factor-alpha-induced secretion of RANTES and interleukin-6 from human airway smooth-muscle cells. Modulation by cyclic adenosine monophosphate. Am J Respir Cell Mol Biol 2000, 23:794–802.
Knox AJ, Corbett L, Stocks J, Holland E, Zhu YM, Pang L: Human airway smooth muscle cells secrete vascular endothelial growth factor: up-regulation by bradykinin via a protein kinase C and prostanoid-dependent mechanism. FASEB J 2001, 15:2480–2488.
Jacobowitz O, Iyengar R: Phorbol ester-induced stimulation and phosphorylation of adenylyl cyclase 2. Proc Natl Acad Sci USA 1994, 91:10630–10634.
Stevens PA, Pyne S, Grady M, Pyne NJ: Bradykinin-dependent activation of adenylate cyclase activity and cyclic AMP accumulation in tracheal smooth muscle occurs via protein kinase C-dependent and -independent pathways. Biochem J 1994,297(Pt 1):233–239.
Pyne NJ, Moughal N, Stevens PA, Tolan D, Pyne S: Protein kinase C-dependent cyclic AMP formation in airway smooth muscle: the role of type II adenylate cyclase and the blockade of extracellular-signal-regulated kinase-2 (ERK-2) activation. Biochem J 1994,304(Pt 2):611–616.
de RJ, Zwartkruis FJ, Verheijen MH, Cool RH, Nijman SM, Wittinghofer A, Bos JL: Epac is a Rap1 guanine-nucleotide-exchange factor directly activated by cyclic AMP. Nature 1998, 396:474–477.
Schmitt JM, Stork PJ: PKA phosphorylation of Src mediates cAMP's inhibition of cell growth via Rap1. Mol Cell 2002, 9:85–94.
McAvoy T, Zhou MM, Greengard P, Nairn AC: Phosphorylation of Rap1GAP, a striatally enriched protein, by protein kinase A controls Rap1 activity and dendritic spine morphology. Proc Natl Acad Sci USA 2009, 106:3531–3536.
Mayr B, Montminy M: Transcriptional regulation by the phosphorylation-dependent factor CREB. Nat Rev Mol Cell Biol 2001, 2:599–609.
Borland G, Bird RJ, Palmer TM, Yarwood SJ: Activation of protein kinase C alpha by EPAC1 is required for the ERK- and C/EBPbeta-dependent induction of the SOCS-3 gene by cyclic AMP in COS1 cells. J Biol Chem 2009,284(26):17391–403.
Niimura M, Miki T, Shibasaki T, Fujimoto W, Iwanaga T, Seino S: Critical role of the N-terminal cyclic AMP-binding domain of Epac2 in its subcellular localization and function. J Cell Physiol 2009, 219:652–658.
Li Y, Asuri S, Rebhun JF, Castro AF, Paranavitana NC, Quilliam LA: The RAP1 guanine nucleotide exchange factor Epac2 couples cyclic AMP and Ras signals at the plasma membrane. J Biol Chem 2006, 281:2506–2514.
Wang Z, Dillon TJ, Pokala V, Mishra S, Labudda K, Hunter B, Stork PJ: Rap1-mediated activation of extracellular signal-regulated kinases by cyclic AMP is dependent on the mode of Rap1 activation. Mol Cell Biol 2006, 26:2130–2145.
Di Benedetto G, Zoccarato A, Lissandron V, Terrin A, Li X, Houslay MD, Baillie GS, Zaccolo M: Protein kinase A Type I and II define distinct intracellular signaling compartments. Circ Res 2008, 103:836–844.
Dodge-Kafka KLSJ, Pare GC, Michel JJC, Langeberg LK, Kapiloff MS, Scott JD: The protein kinase A anchoring protein mAKAP coordinates two integrated cAMP effector pathways. Nature 2005, 437:574–578.
Nijholt IM, Dolga AM, Ostroveanu A, Luiten PGM, Schmidt M, Eisel ULM: Neuronal AKAP150 coordinates PKA and Epac mediated PKB/Akt phosphorylation. Cell Signal 2008, 20:1715–1724.
We thank J. Schuur and I.S.T. Bos for technical assistance. We also thank Drs. C. von Eichel-Streiber and H. Genth for providing Clostridium difficile toxin B-1470. This work was supported by a Ubbo Emmius Fellowship from the School of Behavioral and Cognitive Neurosciences to S.S. Roscioni and a Rosalind Franklin Fellowship from the University of Groningen to M. Schmidt. R. Gosens is the recipient of a Veni grant (916.86.036) from the Dutch Organisation for Scientific Research (NWO). A.J. Halajko is supported by the Canada Research Chairs Program and Canadian Institutes of Health Research. We are grateful to Dr. W.T. Gerthoffer (University of Nevada-Reno) for preparation of the hTERT-airway smooth muscle cell lines.
The authors declare that they have no competing interests.
SSR designed, coordinated and carried most of the work, in particular the siRNA transfections, the statistical analysis, drafted the manuscript and contributed to its design and conception. LEMK and MM performed ELISA and western blot analysis. CRSE carried out the toxin experiments. RG contributed to draft the manuscript and its design, AH and HM helped to improve the study design and the final manuscript. MS conceived of the study, participated in its study design and coordination, helped to draft and improve the manuscript. All authors read and approved the final manuscript.
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Roscioni, S.S., Kistemaker, L.E., Menzen, M.H. et al. PKA and Epac cooperate to augment bradykinin-induced interleukin-8 release from human airway smooth muscle cells. Respir Res 10, 88 (2009). https://doi.org/10.1186/1465-9921-10-88
- Airway Smooth Muscle
- Human Lung Fibroblast
- Human Airway Smooth Muscle