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Originally published In Press as doi:10.1074/jbc.M405594200 on June 17, 2004

J. Biol. Chem., Vol. 279, Issue 35, 37201-37207, August 27, 2004
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Pseudomonas aeruginosa Exotoxin A Induces Human Mast Cell Apoptosis by a Caspase-8 and -3-dependent Mechanism*

Christopher E. Jenkins{ddagger}, Ania Swiatoniowski{ddagger}, Andrew C. Issekutz{ddagger}§, and Tong-Jun Lin{ddagger}§

From the Departments of {ddagger}Microbiology and Immunology and §Pediatrics, Dalhousie University, Halifax, Nova Scotia B3J 3G9, Canada

Received for publication, May 19, 2004


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Mast cells play an important role in both allergy and innate immunity. Recently, we demonstrated an active interaction between human mast cells and Pseudomonas aeruginosa leading to the production of multiple cytokines. Here, we show that both primary cultured human cord blood-derived mast cells and the human mast cell line HMC-1 undergo apoptosis as determined by single-stranded DNA (ssDNA) formation after stimulation with P. aeruginosa exotoxin A (ETA), a major toxin produced by this bacterium. ETA-induced ssDNA formation was completely inhibited by Z-VAD (where Z is benzyloxycarbonyl), which blocks multiple caspases, suggesting a role for caspases in this process. Active caspase-3 formation in mast cells after an ETA challenge was detected by both Western blotting and flow cytometry analysis. ETA-induced caspase-3 activity in human mast cells was demonstrated by the detection of a characteristic 23 kDa product of D4-GDI (where GDI is guanine nucleotide dissociation inhibitor), an endogenous caspase-3 substrate. Interestingly, a specific caspase-8 inhibitor, Z-IETD-fmk (where fmk is fluoromethyl ketone), blocked ETA-induced cleavage of D4-GDI, but a caspase-9 inhibitor (Z-LEHD-fmk) did not. Treatment of mast cells with caspase-3 inhibitor Z-DEVD-fmk or caspase-8 inhibitor Z-IETD-fmk reduced the generation of ssDNA induced by ETA, suggesting a role for caspase-8 and -3 in ETA-induced mast cell apoptosis. Furthermore, treatment of mast cells with ETA induced decreases of the short form and a long form (p43) of Fas-associated death domain protein (FADD)-like interleukin-1{beta}-converting enzyme (FLICE) (caspase-8)-inhibitory proteins (FLIPs), which are endogenous caspase-8 inhibitors. Taken together, these results suggest that ETA-induced mast cell apoptosis involves down-regulation of antiapoptotic proteins, FLIPs, and activation of caspase-8 and -3 pathways.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Pseudomonas aeruginosa, a Gram-negative opportunistic pathogen, is a leading cause of infections in people who have cystic fibrosis, burn victims, and immunocompromised individuals (1). P. aeruginosa synthesizes a number of extracellular toxic products believed to be involved in the pathogenesis of these infections. Exotoxin A (ETA),1 a 66-kDa protein, is considered to be the most toxic factor secreted by P. aeruginosa (2-6). Because of its potent cytotoxicity, ETA has been widely used to generate fusion proteins to kill target cells. For example, chimeric cytotoxins have been constructed by the fusion of growth factors or antibodies with the enzymatic region of ETA to specifically target and eliminate cancer cells, virally infected cells, or mast cells (7-12). It is generally accepted that ETA is internalized by the cell surface receptor CD91 (the {alpha}2-macroglobulin receptor/low density lipoprotein receptor-related protein) (13) and asserts its cellular toxicity by blocking protein synthesis through ADP ribosylation of translation elongation factor 2 (14-16). However, protein synthesis inhibition by toxins is not sufficient to mediate target cell lysis (17). In addition, decreased ADP ribosylation activity does not affect ETA-induced cytotoxicity, suggesting a dissociation between protein synthesis and cytotoxicity (18). Thus, additional mechanisms may be involved in ETA-induced cytotoxicity.

Apoptotic cell death has been implicated in ETA-induced cytotoxicity because ETA increases caspase-like activities in monocytic cell lines (19) and induces nuclear morphological changes and DNA fragmentation in these cells (19, 20). The role of apoptosis in ETA-induced cytotoxicity, however, seems controversial because DNA fragmentation and nuclear morphological changes are not specific to apoptosis. Moreover, some cell types such as epithelial respiratory cells and HUT-102 cells that are killed by ETA do not undergo apoptotic cell death (7, 21). Thus, a role for apoptosis in ETA-induced cytotoxicity requires further study.

Caspase activation plays a central role in the execution of apoptosis (22, 23). Depending on the nature of the stimuli and the cell types, two caspase activation pathways have been described, including the receptor-initiated caspase-8-dependent pathway and the mitochondria-initiated caspase-9-mediated pathway (22-24). Activated caspase-8 or -9 initiates a downstream cascade of effector caspases, such as caspase-3, which cleaves various substrates such as D4-GDI, and leads to the execution of cell death (22, 23). The specific roles of caspase-8 and caspase-9 pathways as well as caspase-3 in ETA-induced apoptosis are unclear.

Death receptor caspase 8-induced apoptosis is counteracted by Fas-associated death domain (FADD)-like interleukin-1-converting enzyme (FLICE)-inhibitory proteins (FLIPs) (25). FLIPs structurally resemble caspases but lack proteolytic activity. There are two isoforms of cellular FLIPs, FLIP short (FLIPshort, 26 kDa) and FLIP long (FLIPlong, 55 kDa), of which the latter can be cleaved into FLIP(p43) and FLIP(p12). Both FLIPlong and FLIPshort can be recruited into the death-inducing signaling complex and associate with caspase-8 (26). Accordingly, FLIPs have been proposed as antiapoptotic proteins because activation of caspase-8 is blocked. Modulation of the FLIPs expression level regulates the apoptotic process in various cell types including mast cells (27).

Among granulocytes, mast cells are exceptionally long-lived (up to months), suggesting that they are not normally programmed for spontaneous apoptosis (28). Because mast cells play an essential role in allergy, several approaches have been used to deplete mast cells, including ETA (9, 10). A chimeric protein composed of an Fc fragment of mouse IgE and a truncated form of ETA demonstrates potent mast cell cytotoxicity in vitro and prevents mast cell-dependent passive cutaneous anaphylaxis in mice in vivo (9, 10). Mechanisms of ETA-induced mast cell cytotoxicity have not been reported.

In this study, using an apoptosis-specific marker, the generation of single strand DNA, we demonstrated that human mast cells undergo apoptosis after exposure to pathologically relevant levels of ETA. ETA-induced human mast cell apoptosis is shown to be mediated by caspase-3activation through a caspase-8-dependent but not a caspase-9-dependent pathway. Furthermore, ETA down-regulates FLIPshort and FLIP(p43) levels in human mast cells. Thus, ETA-induced human mast cell apoptosis involves down-regulation of antiapoptotic FLIPs and activation of caspase-8 or -3 pathway.


   MATERIALS AND METHODS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Reagents—Z-VAD-fmk (multiple caspases inhibitor), Z-DEVD-fmk (caspase-3 inhibitor), Z-IETD-fmk (caspase-8 inhibitor), and Z-LEHD-fmk (caspase-9 inhibitor) were purchased from R & D Systems (Minneapolis, MN). Purified P. aeruginosa ETA was purchased from List Biologicals (Campbell, CA). Fetal bovine serum, penicillin/streptomycin, Iscove's modified Dulbecco's medium, and RPMI 1640 medium were purchased from Invitrogen. Mouse anti-single-stranded DNA (ssDNA) monoclonal antibody (mAb) (IgM), rabbit anti-FLIPshort and rabbit anti-FLIPlong antibodies were purchased from Chemicon International (Temecula, CA). Mouse anti-rat neutrophil mAb (RP-3, IgM) isotype control was a gift from F. Sendo (Yamagata University, Japan). Rabbit anti-active caspase-3 IgG was purchased from Cell Signaling Technology, Inc. (Beverly, MA). Rabbit FITC-conjugated anti-active-caspase-3 IgG was purchased from BD Biosciences. Mouse anti-D4-GDI (specific for the 23-kDa form) mAb was purchased from Imgenex (San Diego, CA). Mouse anti-human Bcl-2 (IgG1) and rabbit anti-human Bax were purchased from Upstate Biotechnology (Lake Placid, NY). Goat anti-actin IgG, donkey anti-goat IgG horseradish peroxidase, donkey anti-rabbit IgG horseradish peroxidase, and donkey anti-mouse IgG horseradish peroxidase antibody conjugates were purchased form Santa Cruz Biotechnology (Santa Cruz, CA). Goat phycoerythrin-conjugated IgG to mouse IgM was purchased from Caltag (Burlingame, CA). All other chemicals and reagents were of analytical grade.

Mast Cells and Culture Conditions—HMC-1 5C6 human mast cells were maintained in Iscove's modified Dulbecco's medium in a 5% CO2-humidified atmosphere at 37 °C. Culture medium was supplemented with 10% fetal bovine serum and 50 units/ml each of penicillin and streptomycin.

Highly purified cord blood-derived mast cells (CBMC) (>95% purity) were obtained by long term culture of cord blood progenitor cells as described previously (29). The percentage of mast cells in the cultures was determined with toluidine blue staining (pH 1.0) of cytocentrifuged samples. After >8 weeks in culture, mature mast cells were identified by their morphological features and the presence of metachromatic granules, at which time they were used for this study.

Detection of Single-stranded DNA by Flow Cytometry—Exotoxin-treated mast cells were fixed, permeabilized, and stained with a mAb specific for segments of ssDNA as described previously (30). Briefly, mast cells were fixed for 1-3 days in methanol at -20 °C and subsequently heated in formamide at 70 °C for 10 min. Nonspecific binding was blocked with 1% nonfat dry milk (w/v) in phosphate buffered saline. Cells were stained with anti-ssDNA or IgM isotype control, followed by washing and incubation with a phycoerythrin-conjugated anti-mouse IgM antibody. After washing, cells were analyzed with a FACScaliber flow cytometer (BD Biosciences).

Preparation of Total Cell Lysate—Treated cells (0.25 x 105-2.5 x 106) were homogenized in ice-cold radioimmune precipitation assay buffer (50 mM Tris-HCl, pH 7.5, 150 mM NaCl, 50 mM NaHPO4, 0.25% sodium deoxycholate (w/v), 0.1% Nonidet P-40 (v/v), 1 mM Na3VO4, and 1 mM NaF) containing freshly added protease and phosphatase inhibitors (2 mM phenylmethylsulfonyl fluoride, 1 µg/ml aprotinin, 1 µg/ml leupeptin, 1 µg/ml pepstatin A, 5 mM EDTA, 5 mM EGTA, and 2 mM iodoacetamide). Lysates were typically incubated on ice for at least 20 min prior to centrifugation at 15,000 x g to remove cellular debris. Protein was quantified using a protein quantification reagent according to the manufacturer (Bio-Rad).

Western Blotting for Active Caspase-3, D4-GDI, and FLIPs—Sample lysates containing 75 µg of protein (for caspase-3), 15 µg (for D4-GDI), 5 µg (for FLIPshort), and 30 µg (for FLIPlong, XIAP, Bax, and Bcl-2) were boiled for 5 min and subjected to SDS-10% PAGE. Gels were transferred to polyvinylidene difluoride membrane, and nonspecific binding was blocked using 10% nonfat dry milk. Membranes were then incubated overnight at 4 °C with antibodies to active caspase-3, D4-GDI, FLIPshort, FLIPlong, XIAP, Bax, or Bcl-2 and detected by enhanced chemiluminescence detection reagent (Amersham Biosciences). Membranes were subsequently stripped (62.5 mM Tris-HCl, pH 6.8, 20% SDS (w/v), 100 mM {beta}-mercaptoethanol) and re-probed for actin.

Detection of Active Caspase-3 by Flow Cytometry—Treated mast cells (0.5-1 x 106) were fixed in 4% paraformaldehyde and subsequently stored in 10% dimethyl sulfoxide in phosphate-buffered saline at -80 °C until staining. Cells were thawed and permeabilized with 0.1% saponin in phosphate-buffered saline for 1 h followed by incubation in 3% bovine serum albumin/phosphate-buffered saline for 1 h to block nonspecific binding. Cells were then stained with FITC-conjugated rabbit mAb to active caspase-3, washed, and analyzed by flow cytometry.

Statistical Analysis—Data were analyzed by one way analysis of variance followed by Tukey's post-test, using Instat GraphPad software (version 3.0) to determine the statistical difference between individual treatments. Statistical significance was defined as p < 0.05.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Exotoxin A Induces Mast Cell Apoptosis—To determine whether ETA induces mast cell apoptosis, an antibody specific for ssDNA was used. The generation of ssDNA is a specific indicator of apoptosis (30). Human mast cell line HMC-1 cells were treated with various concentrations of ETA (50, 100, 300, and 1000 ng/ml) for 24 h and subjected to formamide-induced DNA denaturation and ssDNA staining with mAb against ssDNA. ETA induced concentration-dependent mast cell apoptosis (Fig. 1, A and B). An isotype control antibody specific for rat neutrophils (RP3) showed no change in staining with ETA treatment (Fig. 1A). ETA-induced mast cell apoptosis was further confirmed using human primary CBMC. Similarly, using CBMC from two individual donors, ETA-induced mast cell apoptosis was shown to behave in a concentration-dependent manner (Fig. 1, C-E). Examination of ETA-treated mast cells by light microscopy also revealed morphological changes characteristic of apoptosis, including membrane blebbing, condensed nuclei, and extensive vacuole formation (data not shown). In addition, treatment of mast cells with lipopolysaccharide (10 µg/ml, 24 h) did not affect ETA-induced mast cell apoptosis (data not shown).



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  		FIG. 1.
Induction of human mast cell apoptosis by P. aeruginosa ETA. A and B, HMC-1 cells were treated with increasing concentrations of ETA for 24 h prior to flow cytometric analysis for ssDNA. ETA induced the dose-dependent generation of ssDNA in HMC-1 5C6. Results are expressed as the mean percentage of ssDNA-positive cells ± S.E. of five independent experiments (*, p < 0.01 compared with HMC-1 cells treated with medium alone). Cells without ETA treatment served as controls (NT). C-E, CBMC were treated with medium or increasing concentrations of ETA for 24 h and then fixed and stained for ssDNA. A representative flow cytometry histogram from one donor's CBMC is shown (C). Results from two individual donors are expressed as the mean percentage of ssDNA-positive cells ± S.E. (D and E).

 
ETA-induced Caspase-3 Activation in Mast Cells—There are several pathways involved in apoptosis, including caspase-dependent and caspase-independent mechanisms (31, 32). To examine the role of caspases in ETA-induced mast cell apoptosis, HMC-1 cells were pretreated with Z-VAD-fmk for 2 h before ETA treatment (300 ng/ml, 18 h). Treatment with Z-VAD-fmk completely blocked ETA-induced mast cell apoptosis (Fig. 2). The complete inhibition of ETA-induced ssDNA formation by Z-VAD-fmk, which specifically blocks multiple caspases, suggests an essential role of caspases in ETA-induced mast cell apoptosis.



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  		FIG. 2.
ETA-induced mast cell apoptosis is dependent on caspase activation. HMC-1 cells were treated with 100 µM Z-VAD-fmk for 1 h prior to a challenge with 300 ng/ml ETA for 18 h. Cells were analyzed for ssDNA using flow cytometry. A, representative flow cytometry histograms are shown. B, results are expressed as the mean percentage of cells staining positive for ssDNA ± S.E. of four independent experiments (*, p < 0.001 compared with medium-treated cells).

 
Caspase-3 is one of the effector caspases that is central in executing the apoptotic process. To determine whether caspase-3 is involved in ETA-induced apoptosis of mast cells, several approaches were taken. Western blotting analysis using a mAb that specifically recognizes the activated form of caspase-3 demonstrated that ETA treatment induced activation of caspase-3 in mast cells in a dose-dependent manner (Fig. 3A). To further examine the population of caspase-3-positive cells after ETA treatment, flow cytometry analysis was carried out using intracellular staining with a FITC-labeled mAb specific for the activated caspase-3. ETA treatment of HMC-1 cells induced a dose-dependent increase of active caspase-3-positive cells (Fig. 3, B and C). Approximately 22% of the HMC-1 cells were stained positive for the active caspase-3.



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  		FIG. 3.
ETA induces dose-dependent activation of caspase-3 in mast cells. A, HMC-1 cells were treated with increasing concentrations of ETA for 24 h and then lysed in radioimmune precipitation assay buffer. Sample lysates were subjected to SDS-PAGE and analyzed by Western blotting with monoclonal antibodies specific for active caspase-3 or actin. B and C, HMC-1 cells were treated with medium or increasing concentrations of ETA for 24 h and then fixed and permeabilized for staining with FITC-conjugated anti-active caspase-3 antibody for flow cytometric analysis. Representative histograms show ETA-treated HMC-1 5C6 (B) but not medium-treated cells stain for active caspase-3. Results are expressed as the mean percentage of positive staining cells ± S.E. of five independent experiments (*, p < 0.05) (C).

 
D4-GDI has been reported as an endogenous caspase-3 substrate (33). To further confirm ETA-induced caspase-3 activation in HMC-1 cells, D4-GDI cleavage was determined by Western blotting analysis. Treatment of these mast cells with ETA induced cleavage of D4-GDI in a dose- and time-dependent manner to yield a characteristic 23-kDa product (Fig. 4). Pre-treatment of the cells with either Z-VAD-fmk or a specific inhibitor of caspase-3, Z-DEVD-fmk, strongly blocked the cleavage of D4-GDI (Fig. 5), suggesting the cleavage of D4-GDI results exclusively from caspase-3 activity. Together, these results suggest a functionally active caspase-3 in mast cells after ETA stimulation.



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  		FIG. 4.
ETA-induced D4-GDI cleavage. HMC-1 cells were treated with ETA for varied times at the concentration of 1000 ng/ml (A) or were treated with ETA for 24 h at varied concentrations (B). Cells without ETA treatment served as controls (NT). Cell lysates were subjected to SDS-PAGE and Western blotting for the analysis of a 23-kDa cleavage fragment (specifically generated by active caspase-3) of the endogenous caspase-3 substrate D4-GDI. Blots were subsequently stripped and reprobed for actin.

 



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  		FIG. 5.
Caspase blockade inhibits caspase-3-mediated cleavage of D4-GDI in ETA-treated mast cells. A, HMC-1 cells were treated with 100 µM Z-VAD-fmk for 2 h prior to a challenge with 300 ng/ml ETA for 18 h. Lysates were subjected to SDS-PAGE and analyzed by Western blotting with an antibody specific for cleaved D4-GDI. The blot was then stripped and reprobed for actin to ensure equal protein loading. B, HMC-1 cells were treated with 50 µM Z-DEVD-fmk (caspase-3 inhibitor) for 2 h prior to challenge with 100 ng/ml ETA for 18 h. Lysates were analyzed by Western blotting with an antibody specific for cleaved D4-GDI. The blot was then stripped and reprobed for actin. NT, cells without ETA treatment.

 
To examine whether ETA has similar effects on other cell types, HL-60 cells (a promyelocytic cell line) were treated with ETA (500 ng/ml) for 18 h, and D4-GDI cleavage was examined by Western blot. Treatment of ETA also induced cleavage of D4-GDI to yield a 23-kDa product (data not shown), suggesting that ETA may also induce caspase 3 activation in additional cell types.

Caspase-8 but Not Caspase-9 Is Responsible for ETA-induced Caspase-3 Activation—Both caspase-8 and caspase-9 have been implicated in caspase-3 activation in different cell types (22-24). To determine whether these two caspases are involved in ETA-induced caspase-3 activation, HMC-1 cells were pre-treated individually with inhibitors specific for caspase-8 or -9 before stimulation with ETA. Interestingly, a specific caspase-8 inhibitor (Z-IETD-fmk) but not a caspase-9 inhibitor (Z-LEHD-fmk) markedly blocked ETA-induced cleavage of D4-GDI (Fig. 6), suggesting an essential role of caspase-8 but not caspase-9 in ETA-induced caspase-3 activation.



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  		FIG. 6.
Caspase-8 inhibitor blocks ETA-induced D4-GDI cleavage in mast cells. HMC-1 cells were treated with 100 µM each ZDEVD-fmk (caspase-3 inhibitor), Z-IETD-fmk (caspase-8 inhibitor), or Z-LEHD-fmk (caspase-9 inhibitor) for 2 h prior to a challenge with 100 ng/ml ETA for 18 h. Cells without ETA treatment served as control (NT). Lysates were subjected to SDS-PAGE and analyzed by Western blotting with an antibody specific for cleaved D4-GDI. The blot was subsequently stripped and reprobed for actin. Dash (-), cells treated with ETA alone.

 
ETA-induced Mast Cell Apoptosis Is Dependent on Caspase-3 and -8 —To determine the importance of caspase-3 and caspase-8 in ETA-induced apoptosis of mast cells, HMC-1 cells were pretreated for 2 h with specific inhibitors for caspase-3 (Z-DEVD-fmk, 100 µM), or -8 (Z-IETD-fmk) before ETA treatment (300 ng/ml, 18 h). Mast cell apoptosis was determined by flow cytometry for the generation of ssDNA. Treatment of mast cells with Z-DEVD or Z-IETD significantly reduced the generation of ssDNA induced by ETA (Fig. 7), suggesting significant roles for caspase-3 and caspase-8 in ETA-induced mast cell apoptosis.



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  		FIG. 7.
Caspase-8 inhibitor and caspase-3 inhibitor block ETA-induced mast cell apoptosis. HMC-1 cells were treated with 100 µM each of Z-DEVD-fmk (caspase-3 inhibitor) or Z-IETD-fmk (caspase-8 inhibitor) for 2 h prior to a challenge with 300 ng/ml ETA for 18 h. Cells were then fixed and analyzed with flow cytometry for ssDNA generation. Results are expressed as the mean percentage of ETA-induced positive staining for ssDNA ± S.E. of four independent experiments (*, p < 0.05).

 
ETA Down-regulates FLIPshort and FLIP(p43) but Not XIAP, Bax, and Bcl-2—Given that caspase-8 activity can be regulated by its natural inhibitor FLIPs, we determined whether ETA modulates FLIP levels in mast cells. HMC-1 5C6 cells were treated with ETA (50, 100, 300, and 1000 ng/ml) for 24 h. Cell lysates were used to determine the protein level of FLIPs by Western blotting. FLIPshort and FLIP(p43) were down-regulated by ETA treatment (Fig. 8, A and B), but other apoptosis-related molecules including Bcl-2, Bax, and XIAP were not affected by ETA treatment (Fig. 8C).



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  		FIG. 8.
ETA down-regulates FLIPshort and FLIP(p43) in mast cells. HMC-1 cells were treated with ETA (50, 100, 300, and 1000 ng/ml) for 24 h. Cell lysates were examined by Western blotting with antibodies to FLIPshort (A), FLIP(p43) (B), and XIAP, Bax, or Bcl-2 (C). Cells without ETA treatment (NT) or treated with 5 µg/ml camptothecin (Camp) were used as controls.

 
Because FLIPs are involved in regulating Fas-induced apoptosis, we determined whether ETA modulates Fas expression in mast cells. Flow cytometry analysis of ETA-treated HMC-1 cells revealed that there was no change in Fas expression on the cell surface after treatment with ETA for 3 or 24 h (data not shown). Tumor necrosis factor-mediated apoptosis, which shares common signaling pathways with Fas to caspase activation, also does not seem to be involved in the ETA-induced apoptosis because no tumor necrosis factor production can be detected in ETA-treated mast cells. Furthermore, the inclusion of anti-tumor necrosis factor neutralizing antibody (20 µg/ml) (neutralization dose50 = 0.04-0.08 µg/ml, according to the manufacturer, R & D Systems) during culture with ETA did not affect ETA-induced mast cell apoptosis (data not shown).


   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
Mast cells not only play an essential role in allergy, they also have an important role in host defense against bacterial infection (34, 35). Mast cells are abundant in the lung, occupying ~1.6-2.1% of the area of the alveolar wall (36). Importantly, many human lung mast cells directly protrude through the alveolar wall into air space (36), which allows direct interaction between mast cells and pathogens. Recently, we demonstrated active interactions between human mast cells and P. aeruginosa, resulting in the secretion of mast cell-derived cytokines and chemokines that are important in innate immunity (37-39). In the present study, we demonstrate that human mast cells undergo apoptosis in response to P. aeruginosa ETA. Apoptosis has been described as an essential host defense mechanism against P. aeruginosa lung infection, because a deficiency of apoptosis leads to the rapid development of P. aeruginosa-induced sepsis (40). ETA is considered the most dominant and lethal of the virulent factors produced by the majority of clinical isolates (2-6). Whether ETA induces target cell apoptosis is inconclusive because some cells such as lung epithelial cells do not undergo apoptosis after an ETA challenge (21). The involvement of apoptosis is further complicated by the methodologies used to define "apoptosis." Several commonly used methods such as those based on morphological changes, DNA fragmentation, or terminal deoxynucleotidyltransferase-mediated dUTP nick end-labeling assay, which can stain 90-100% of necrotic cells (30), are not specific to apoptosis. A recently developed technique based on formamide-induced DNA denaturation combined with detection of denatured DNA with a monoclonal antibody against ssDNA allows specific detection of apoptotic cells (30). Concentration-dependent human mast cell apoptosis determined by ssDNA formation is supported by a similar pattern of active caspase-3 formation in these cells. Interestingly, the levels of ETA that induce human mast cell apoptosis, ranging from 50 to 1000 ng/ml in this study, are physiologically relevant because ETA concentrations can exceed 100 ng/ml in the sputum of cystic fibrosis patients (41) and can reach over 300 ng/ml in the serum of acute P. aeruginosa septicemia in mice (4).

Given that there are caspase-dependent and caspase-independent pathways leading to apoptotic cell death (31, 32), a role of caspases in ETA-induced human mast cell apoptosis was investigated. We provide compelling evidence of caspase-3 activation in mast cells by demonstrating active caspase-3 formation by Western blotting and flow cytometry analysis and the cleavage of D4-GDI, an endogenous caspase-3 substrate. Complete inhibition of ETA-induced ssDNA formation and D4-GDI cleavage by Z-VAD-fmk suggests an essential role of the caspase-dependent pathway in ETA-induced mast cell apoptosis. This finding is supported by others (7, 42) who demonstrate caspase-3-like activities induced by immunotoxins or chimeric proteins with growth factors such as interleukin-13 (11, 43). These chimeric products, however, may involve additional mechanisms such as Fc receptors (immunotoxins) or growth factor receptors such as interleukin-13 receptors and other factors, in addition to toxin-mediated effects.

Two caspase-dependent pathways leading to caspase-3 activation have been well recognized; these are receptor caspase-8-dependent and mitochondria caspase-9-dependent pathways (22-24). Specific pathways involved in apoptosis are likely cell type-specific (24). In type I cells, such as lymphocytes, the caspase-8 pathway is sufficient to initiate apoptosis and cell death (24). Overexpression of mitochondria pathway-related antiapoptotic factors such as Bcl-2 cannot protect type I cells from death receptor-induced cytotoxicity (44). By contrast, type II cells, such as hepatocytes, require a mitochondria caspase-9 pathway for robust apoptosis (45, 46). Specific apoptotic pathways used in mast cells are unclear, although caspase-3 activity has been detected in mast cells (27, 47-50). We demonstrated that ETA-induced ssDNA formation and D4-GDI cleavage were inhibited by a caspase-8 inhibitor (Z-IETD-fmk) but not by a caspase-9 inhibitor (Z-LEHD-fmk), suggesting a role for a caspase-8 pathway in ETA-induced mast cell apoptosis.

Activation of caspase-8 is counteracted by its natural endogenous inhibitors, FLIPs. Regulation of FLIPs expression modulates the sensitivity of mast cells to apoptosis (27). Accordingly, we examined whether ETA modulates FLIPs expression levels in human mast cells. Our results indicated that FLIPshort and FLIP(p43) were reduced by ETA treatment. FLIPshort is widely recognized as a "dedicated" caspase-8 inhibitor. Although the full length of FLIPlong (55 kDa) may have dual effects on pro-caspase-8 activation, its truncated form FLIP(p43) is considered to be a major inhibitor for caspase-8 activation (51). The down-regulation of FLIPshort and FLIP(p43) may contribute to the ETA-induced caspase-8 or -3 pathway-dependent apoptosis in mast cells.

ETA-mediated responses likely involve both the surface receptor that mediates its internalization and the toxin's intracellular targets. CD91 (the {alpha}2-macroglobulin receptor/low density lipoprotein receptor-related protein) has been identified as a receptor for ETA in mouse fibroblast (13). In an attempt to determine whether CD91 is a receptor for ETA on mast cells, we used flow cytometry to examine CD91 expression on human mast cells. No CD91 was detected on HMC-1 or primary cultured CBMC (data not shown), but confocal microscopic analysis of ETA-treated mast cells showed intense intracellular localization (data not shown), suggesting that additional mechanisms may be involved in ETA internalization.

In conclusion, we demonstrated direct evidence of human mast cell apoptosis induced by ETA through detection of ssDNA formation. Caspase-3 activation through the caspase-8 pathway appears to play a major role in ETA-induced human mast cell apoptosis. ETA-induced down-regulation of FLIPs likely contributes to ETA-induced activation of the caspase-8 or -3 pathway. Given that mast cells are now known to be multi-functional effector cells that have the capacity to mediate both innate and T helper type 2 cell-induced immune responses (28), these data not only provide direct evidence of the roles of caspases in ETA-mediated apoptosis but also have implications for developing strategies for manipulating mast cell homeostasis in allergy or infection.


   FOOTNOTES
 
* This work was supported by grants from Canadian Institutes of Health Research, Canadian Cystic Fibrosis Foundation, Nova Scotia Health Research Foundation, and Isaac Walton Killam Health Center. The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact. Back

Supported by a New Investigator Award from Canadian Institutes of Health Research and an investigatorship from the Isaac Walton Killam Health Center. To whom correspondence should be addressed: I. W. K. Health Center, Dept. of Pediatrics, 5850 University Ave., Halifax, Nova Scotia B3J 3G9, Canada. Tel.: 902-470-8834; Fax: 902-470-7812; E-mail: tong-jun.lin{at}dal.ca.

1 The abbreviations used are: ETA, exotoxin A; GDI, guanine nucleotide dissociation inhibitor; FLIPs, Fas-associated death domain (FADD)-like interleukin-1-converting enzyme (FLICE)-inhibitory proteins; Z, benzyloxycarbonyl; fmk, fluoromethylketone; HMC, human mast cell; ssDNA, single-stranded DNA; mAb, monoclonal antibody; FITC, fluorescein isothiocyanate; CBMC, cord blood-derived mast cells; XIAP, X-linked inhibitor of apoptosis protein. Back



   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

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