Bacteroides fragilis enterotoxin upregulates heme oxygenase-1 in dendritic cells via reactive oxygen species-, mitogen-activated protein kinase-, and Nrf2-dependent pathway.

BACKGROUND: Enterotoxigenic Bacteroides fragilis (ETBF) causes colitis and diarrhea, and is considered a candidate pathogen in inflammatory bowel diseases as well as colorectal cancers. These diseases are dependent on ETBF-secreted toxin (BFT). Dendritic cells (DCs) play an important role in directing the nature of adaptive immune responses to bacterial infection and heme oxygenase-1 (HO-1) is involved in the regulation of DC function. AIM: To investigate the role of BFT in HO-1 expression in DCs.
METHODS: Murine DCs were generated from specific pathogen-free C57BL/6 and Nrf2-/- knockout mice. DCs were exposed to BFT, after which HO-1 expression and the related signaling factor activation were measured by quantitative RT-PCR, EMSA, fluorescent microscopy, immunoblot, and ELISA.
RESULTS: HO-1 expression was upregulated in DCs stimulated with BFT. Although BFT activated transcription factors such as NF-κB, AP-1, and Nrf2, activation of NF-κB and AP-1 was not involved in the induction of HO-1 expression in BFT-exposed DCs. Instead, upregulation of HO-1 expression was dependent on Nrf2 activation in DCs. Moreover, HO-1 expression via Nrf2 in DCs was regulated by mitogen-activated protein kinases such as ERK and p38. Furthermore, BFT enhanced the production of reactive oxygen species (ROS) and inhibition of ROS production resulted in a significant decrease of phospho-ERK, phospho-p38, Nrf2, and HO-1 expression.
CONCLUSION: These results suggest that signaling pathways involving ROS-mediated ERK and p38 mitogen-activated protein kinases-Nrf2 activation in DCs are required for HO-1 induction during exposure to ETBF-produced BFT. ©The Author(s) 2020. Published by Baishideng Publishing Group Inc. All rights reserved.

Core tip: Enterotoxigenic Bacteroides fragilis is associated with non-invasive diarrheal diseases, inflammatory bowel diseases, and colorectal cancers. Bacteroides fragilis enterotoxin (BFT) is responsible for these diseases. The present study demonstrated that signaling pathways involving reactive oxygen species-mediated ERK, p38 mitogen-activated protein kinases and Nrf2 activation in dendritic cells are required for heme oxygenase-1 (HO-1) induction during exposure to BFT. This signaling pathway is different from our previous report that BFT upregulates HO-1 in intestinal epithelial cells via a p38 mitogen-activated protein kinases- and NF-κB-dependent pathway. Therefore, this is the first report concerning the effects of BFT on the HO-1 induction pathway in dendritic cells.

INTRODUCTION

Enterotoxigenic Bacteroides fragilis (ETBF) not only causes colitis and diarrhea but is also implicated in inflammatory bowel diseases and colorectal cancer[1-3]. ETBF secrete a single unique virulence factor called ETBF enterotoxin (B. fragilis toxin; BFT) that causes those diseases[1-3]. The secreted BFT first contacts the intestinal epithelial cells. Since BFT is a metalloprotease, it can destroy the tight junctions in the intestinal epithelium by cleaving E-cadherin, resulting in loss of tight junctions[3-5]. Therefore, after passing through the destroyed area of the intestinal epithelial barrier, BFT may be in direct contact with immune cells distributed in the lamina propria of the gut.

Among immune cells present in the lamina propria, dendritic cells (DCs) play an important role in mucosal immune responses to bacterial pathogens. In addition to antigen uptake through the above methods, luminal bacterial antigens such as virulence factors can enter into the mucosal tissue when lamina propria DCs extend their dendrites into the lumen[6,7]. Therefore, secreted BFT may contact DCs distributed within the intestinal mucosa. Although BFT has been reported not to directly induce maturation in bone marrow (BM)-derived DCs[8], it is presumed that cellular responses may occur after DCs contact BFT. Nevertheless, little is known about BFT-induced DC responses.

Heme oxygenase-1 (HO-1) is an inducible enzyme that catalyzes the degradation of free heme into carbon monoxide, biliverdin, and free iron[9-11]. HO-1 plays a major protective role in various disease models through anti-inflammatory actions[12-14]. In addition, HO-1 has been associated with DC function regulation. For example, the upregulation of HO-1 endues DCs with more potent and durable immunoregulatory properties[15]. In addition, the upregulation of HO-1 in murine Kupffer cells inhibits DC migration in vitro[16]. HO-1-expressing DCs also promote the differentiation of Foxp3+ regulatory T cells and then induce less severe airway inflammation in murine models[17]. We previously demonstrated that BFT upregulates HO-1 expression in intestinal epithelial cells, which may play a role in protection from apoptotic cell death[12]. However, there are no reports regarding BFT-induced HO-1 expression in DCs.

Several studies have demonstrated that HO-1 expression is regulated via signaling pathways from transcription factors, including nuclear factor-kappaB (NF-κB), activator protein-1 (AP-1), and NF-E2-related factor 2 (Nrf2)[9,11,12]. Although BFT can activate such transcription factor signaling in intestinal epithelial cells[12], there is no evidence that signals associated with BFT-induced transcription factors are related to HO-1 induction in DCs. In the studies reported here, we investigated HO-1 induction in response to stimulation of DCs with BFT and found that signaling pathways involving reactive oxygen species (ROS)-mediated mitogen-activated protein kinases (MAPKs)-Nrf2 in DCs are required for HO-1 induction following exposure to BFT.

MATERIALS AND METHODS

Reagents

GIBCO BRL (Gaithersburg, MD, USA) supplied Ca2+ and Mg2+-free Hank's balanced salt solution (HBSS), antibiotics, L-glutamine, and Trizol. LPS-free fetal bovine serum (FBS) was purchased from American Type Culture Collection (ATCC, Manassas, VA, United States). RPMI 1640 media, DMEM media, N-Acetyl-L-cysteine (NAC), sodium pyruvate, non-essential amino acids, collagenase XΙa, dispase, bovine serum albumin (BSA), and soybean trypsin inhibitor were obtained from Sigma Chemical Co. (St. Louis, MO, United States). Rabbit monoclonal antibodies (mAbs) against phospho-IκBα and phospho-IKKα/β, and rabbit polyclonal Abs against phospho-c-jun, phospho-p65, phospho-ERK1/2, phospho-Elk1, pan-extracellular signal-regulated kinase 1/2 (ERK1/2), phospho-p38, pan-p38, phospho-JNK, pan-JNK, and were acquired from Cell Signaling Technology, Inc. (Beverly, MA, United States). Rabbit polyclonal Ab against phospho-Nrf2 was gained from Bioss Antibodies Inc. (Woburn, MA, United States). Santa Cruz Biotechnology (Santa Cruz, CA, United States) supported rabbit polyclonal Abs against Nrf2 and HO-1, and mouse mAbs against actin and lamin B, and goat anti-mouse and anti-rabbit secondary Abs conjugated to horseradish peroxidase. Thermo Fisher Scientific (Waltham, MA, United States) and AbCAM (Cambridge, MA, United States) supplied Alexa Fluor 488 and DyLight 549 secondary Abs, respectively. Chemical inhibitors such as PD98059, SP600125, SB203580, and Bay 11-7085 were acquired from Calbiochem (La Jolla, CA, United States). Tocris Bioscience (Bristol, United Kingdom) supported SR11302. Murine recombinant IL-4 and GM-CSF were gained from PeproTech (Rocky Hill, NJ, United States).

Purification of BFT and cell culture conditions

BFT was purified from culture supernatants of a toxigenic strain of ETBF (ATCC 43858) as described previously[18-20]. An immature murine DC cell line DC2.4 cells was cultured in RPMI 1640 supplemented with 10% FBS, 1% antibiotics, L-glutamine (2 mmol/L), sodium pyruvate (1 mmol/L) and non-essential amino acids (2 mmol/L). These cells were grown at 37°C with 5% CO2 as previously described[9,21].

Generation of primary murine bone marrow-derived DCs and colonic epithelial cells

All animal experiments were approved from the Institutional Animal Care and Use Committee of Hanyang University and Ewha Womans University. Specific pathogen-free C57BL/6 and breeding pairs of Nrf2−/− knockout mice were obtained from Orient Experimental Animals (Seoungnam, South Korea) and RIKEN BioResource Center (Tsukuba, Japan)[22], respectively. Generation of primary murine bone marrow (BM)-derived DCs was performed as previously described[9]. Briefly, femurs, and tibias of male mice (8-12 wk of age, body mass of 20-25 g) were harvested and cells were then cultured in RPMI 1640 media supplemented with 10% FBS, 1% antibiotics, L-glutamine (2 mmol/L), 2-mercaptoethanol (55 μmol/L), murine recombinant GM-CSF (10 ng/mL), and murine recombinant IL-4 (10 ng/mL). After six days in culture, DCs were harvested and stimulated with BFT[9]. The purity of CD11c+ cells was greater than 95% as determined by flow cytometric analysis.

Primary murine colonic epithelial cells were also isolated as described previously[12]. Briefly, intestines were cut into 1-mm fragments and treated with HBSS containing an enzyme solution [dispase (0.02 mg/mL), collagenase XΙa (60 units/mL), soybean trypsin inhibitor (0.2 mg/mL), and BSA (2%)]. Cells were suspended in DMEM containing FBS (10%) with antibiotics, plated on mouse fibronectin-coated dishes, and incubated in 5% CO2 at 37 °C. Cells were then cultivated in medium containing equal volumes of DMEM and Ham's 12 medium supplemented with FBS (10%) and antibiotics[12]. At least 90% of primary colonic epithelial cells were viable for 2 wk in culture as determined by trypan blue exclusion. This procedure was supported by Dr. Sang Hoon Lee of the University of California, Los Angeles, CA[12,23].

Quantitative reverse transcriptase-PCR

Total RNA was extracted from BFT-treated cells using Trizol. Reverse transcription and PCR amplification were performed as described previously[12]. The primers and expected PCR product sizes were as follows: mouse HO-1, 5'-AAG AGG CTA AGA CCG CCT TC-3' (sense), 5'-GTC GTG GTC AGT CAA CAT GG-3' (antisense), 591 bp [NM_010442.2 Mus musculus heme oxygenase (decycling) 1 (Hmox1), mRNA][24]; mouse β-actin, 5'-GTG GGC CGC TCT AGG CAC CAA-3' (sense) and 5'-CTC TTT GAT GTC ACG CAC GAT TTC-3' (antisense), 540 bp [NM_007393.4 Mus musculus actin, beta (Actb), mRNA][25]. For quantifying mRNA molecules, reverse transcription and PCR amplification were performed as described previously[12]. The sizes of PCR products generated from standard RNAs for mouse HO-1 and β-actin are 478 bp and 746 bp, respectively[12].

Electrophoretic mobility shift assays

Cells were harvested and nuclear extracts were prepared as described previously[9,26]. The concentration of protein in extracts was determined using a Bradford assay (Bio-Rad, Hercules, CA, United States). Electrophoretic mobility shift assays were performed according to the manufacturer’s instructions (Promega, Madison, WI, United States)[9]. In brief, 5 μg of nuclear extract was incubated for 30 min at room temperature with γ32P-labeled oligonucleotide probes (5'-AGT TGA GGG GAC TTT CCC AGG C-3' for the NF-κB binding site; 5'-CGC TTG ATG ACT CAG CCG GAA-3' for the AP-1 binding site; 5'- TGG GGA ACC TGT GCT GAG TCA CTG GAG-3' for the Nrf2 binding site). Oligonucleotide probes for the NF-κB- and AP-1-binding assays were purchased from Promega. Santa Cruz Biotechnology supplied Nrf2 oligonucleotides. Nrf2 supershift and competition assay were performed as previously described[9,12].

Transfection assay

were used to For suppression of NF-κB, AP-1, Nrf2, or MAPK signals, lentiviral systems containing mammalian expression vectors were used as previously described[9,12]. Transfection assays using lentiviral systems were performed according to the manufacturer’s instructions, as described previously[9,12]. Small interfering RNA (siRNA) against the NF-κB p65 subunit and c-jun, and negative (non-silencing) siRNA control (NS-RNA) were obtained (Qiagen, Valencia, CA, United States) as described previously[9,12]. Briefly, cells were cultured in 6-well plates to 50%-80% confluence and then transfected with siRNA using Fugene 6 (Roche, Mannheim, Germany) as a transfection reagent, as described previously[9,12]. Transfected cells were incubated for 48 h before the assay.

Immunoblots, ELISA, and cellular ROS assay

For immunoblot, cells were washed with ice-cold PBS and lysed in 0.5 mL/well lysis buffer (150 mmol/L NaCl, 20 mmol/L Tris pH 7.5, 0.1% Triton X-100, 1 mmol/L PMSF, and 10 μg/mL aprotinin). Fifteen to 50 µg of protein per lane was size-fractionated on a polyacrylamide minigel (Mini-PROTEIN II, Bio-Rad) and electrophoretically transferred to a nitrocellulose membrane (0.1-μm pore size). Immunoreactive proteins to which primary Abs bound were visualized using goat anti-rabbit or anti-mouse secondary Abs conjugated to horseradish peroxidase, followed by enhanced chemiluminescence (ECL system; Amersham Life Science, Buckinghamshire, United Kingdom) and exposure to X-ray film[9,12].

The level of HO-1 proteins was measured using a commercially available kit (R&D Systems, Inc., Minneapolis, MN, United States). An ELISA kit of the TransAM Nrf2 (Active Motif, Carlsbad, CA, United States) was also used[9,25]. For detecting expression of phospho-Elk1, a p44/42 MAP kinase assay kit (Cell Signaling Technology) was used[12]. Briefly, immobilized phospho-p44/42 MAPK (Thr202/Tyr204) mAb was used to immunoprecipitate active p44/42 MAPK from cell extracts, after which an in vitro kinase assay was performed using Elk-1 protein as a substrate. Elk-1 phosphorylation was then detected by Western blotting using phospho-Elk-1 (Ser383) Ab. Each assay was performed according to each manufacturer’s instructions.

The level of intracellular ROS was determined using a commercially available kit (Thermo Fisher Scientific). Briefly, BFT-exposed cells were washed with PBS and were then incubated with 5 μmol/L CellROX® Reagent (Thermo Fisher Scientific) at 37 °C for 30 min. Fluorescence was measured using a Varioskan Flash spectral scanning multimode reader (Thermo Fisher Scientific). The assay was performed according to the manufacturer’s protocol.

Immunofluorescence assay for detecting intracellular HO-1 and Nrf2

Immunofluorescence assay was performed, as described previously[9,12,19]. Briefly, cells were cultured (5 × 104 cells in 0.2 mL of RPMI 1640/well) in microslides coated with poly-D-lysine (Santa Cruz). After stimulation with BFT for the indicated period, cells were treated with goat anti-HO-1 and rabbit anti-phospho-Nrf2 Abs as primary Abs for 2 h. Cells were then treated with Alexa fluor 488-conjugated secondary Ab (green color) against goat IgG and DyLight 549-conjugated secondary Ab (red color) against rabbit IgG for 1 h. Images were captured using a fluorescence microscope (DMI4000B, Leica Microsystems GmbH, Wetzlar, Germany)[9,12,19].

Statistical analysis

Data from quantitative RT-PCR assays are presented as mean ± SD and data from ELISA and ROS assay are presented as mean ± SE. Mann-Whitney t-test was used for statistical analysis. P values < 0.05 were considered statistically significant.

RESULTS

BFT induces HO-1 upregulation in DCs

BFT enhanced HO-1 mRNA expression in murine BMDCs (Figure 1A). Significant increases in HO-1 mRNA expression in DC were first noted 9 h after stimulation with BFT, the expression continued to increase for 24 h before decreasing thereafter. Since BFT was known to upregulate HO-1 expression in intestinal epithelial cells[12], we observed differenced in the kinetics of HO-1 mRNA expression between DCs and intestinal epithelial cells. As shown in Figure 1B, compared with DCs, primary murine intestinal epithelial cells showed early expression of HO-1 mRNA, with peak expression approximately 6 h post-stimulation that decreased to baseline level at 24 h post-stimulation. These results suggest that the kinetics of HO-1 mRNA expression in DCs differs from that of intestinal epithelial cells. To determine whether increased levels of mRNA transcripts were parallel with protein expression, we performed immunoblot analyses. As shown in Figure 1C, BFT increased the expression of HO-1 proteins in BMDCs (top panel). Similar results were obtained in the murine DC cell line DC2.4 when stimulated with BFT (Figure 1C, middle panel). In contrast to DCs, primary murine intestinal epithelial cells first noted upregulated expression HO-1 proteins 3 h after stimulation with BFT (Figure 1C, bottom panel). In the present study, we used 100 ng/mL of BFT after previously establishing that the EC50 of BFT was 99.8 ng/mL for expression of HO-1[12].

Figure 1

Heme oxygenase-1 expression in dendritic cells stimulated with Bacteroides fragilis enterotoxin. A and B: Bone marrow-derived dendritic cells (DCs) (A, BMDCs) or primary murine intestinal epithelial cells (B, Murine intestinal epithelial cells, IECs) were stimulated with Bacteroides fragilis toxin (BFT) (100 ng/mL) for the indicated periods. Levels of heme oxygenase-1 (HO-1) and β-actin mRNAs were analyzed by quantitative RT-PCR using each standard RNA. The values are expressed as mean ± SD (n = 5). aP < 0.05 vs unstimulated controls. C: BMDCs, DC2.4 cells and murine IECs were treated with BFT (100 ng/mL) for the indicated periods. Expression of HO-1 and actin was analyzed by immunoblot. Results are representative of more than three independent experiments. IECs: Intestinal epithelial cells; HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

Activation of NF-κB and AP-1 is not involved in the induction of HO-1 in BFT-exposed DCs

Since there is no evidence for BFT-induced activation of NF-κB and AP-1 signaling in DCs, we first examined whether BFT stimulation could activate NF-κB and AP-1 signaling in DCs. As shown in Figure 2A, treatment of BM-derived DCs with BFT increased NF-κB DNA binding, as assessed by EMSA. In addition, enhanced expression of phosphorylated IκBα was observed in BFT-treated DCs. Similar results were also observed in DC 2.4 cells exposed to BFT (Figure 2B). Based on these results, we determined whether BFT-induced activation of NF-κB signal was related to HO-1 expression in DCs. For these experiments, we used DC2.4 cells transfected with lentivirus-IκBα-AA. As shown in Figure 2C, transfection with lentivirus-IκBα-AA suppressed NF-κB activity to the control level under BFT-treated condition (Figure 2C, top panel). In this experimental system, HO-1 expression induced by stimulation with BFT did not differ between untransfected and transfected cells (Figure 2C, bottom panel). Consistent with these results, transfection with lentivirus-IκBα-AA did not significantly alter HO-1 mRNA expression in DC2.4 cells under BFT exposure (Figure 2D). To confirm these results, another experiment using p65 siRNA was performed to inhibit NF-κB activity. As shown in Figure 2E, BFT-induced nuclear phospho-p65 protein expression was reduced in p65 siRNA-transfected cells compared with untransfected cells (Figure 2E, top panel). In contrast, no difference of BFT-induced HO-1 expression was observed between cells with p65 siRNA transfection and cells without transfection (Figure 2E, bottom panel).

Figure 2

Effects of NF-κB suppression on heme oxygenase-1 expression in dendritic cells treated with Bacteroides fragilis enterotoxin. A and B: Bone marrow-derived dendritic cells (DCs) (A) and DC2.4 cells (B) were treated with BFT (100 ng/mL) for the indicated times. NF-κB DNA binding activity was assessed by EMSA. Immunoblot results for concurrent phospho-IκBα and lamin B in nuclear extracts under the same conditions are provided beneath the EMSA. C: DC2.4 cells were transfected with either lentivirus containing IκBα-superrepressor (IκBα-AA) or control virus (GFP). Transfected cells were stimulated with BFT (100 ng/ml) for 1 h. NF-κB binding activity was assayed by EMSA (top panel). Transfected or untransfected cells were treated with BFT (100 μg/ml) for 12 h. Expression of heme oxygenase-1 (HO-1) and actin was analyzed by immunoblot (bottom panel). Results are representative of more than three independent experiments. D: Transfected DC2.4 cells were treated with BFT (100 ng/ml) for the indicated periods. The levels of HO-1 mRNA were analyzed by quantitative RT-PCR using a standard RNA. The values are expressed as mean ± SD (n = 5). The β-actin mRNA levels in each group remained relatively constant throughout the same periods (approximately 106 transcripts/μg total RNA). aP < 0.05 vs untransfected cells treated with BFT. E: DC2.4 cells were transfected with NF-κB p65-specific silencing siRNA or NS-RNA as a control for 48 h, after which cells were combined with BFT (100 ng/mL) for 1 h. Nuclear extracts were analyzed by immunoblotting with the indicated Abs (top panel). Transfected cells were stimulated with BFT (100 ng/mL) for 24 h. Expression of HO-1 and actin was analyzed by immunoblot (bottom panel). Results shown are representative of more than three independent experiments. HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

BFT can activate AP-1 signaling in DCs. As shown in Figure 3, stimulation of DCs with BFT increased AP-1-DNA binding activity in murine BMDCs (Figure 3A) and DC2.4 cells (Figure 3B), as shown by EMSA. Concurrently, increased expression of phosphorylated c-jun was observed in BFT-treated murine BMDCs and DC2.4 cells. The effects of transfection with lentivirus-dn-c-jun on HO-1 expression in BFT-stimulated DC2.4 cells were assessed next. As shown in Figure 3C, transfection with lentivirus-dn-c-jun suppressed AP-1 activity to control levels in DC2.4 cells stimulated with BFT (top panel). Consistent with this, expression of nuclear phospho-c-jun was reduced in lentivirus-dn-c-jun-transfected cells compared with untransfected cells (Figure 3C, middle panel), while transfection with lentivirus-dn-c-jun did not change the BFT-induced HO-1 expression (Figure 3C, bottom panel). In addition, lentivirus-dn-c-jun-transfected cells did not significantly alter HO-1 mRNA expression compared with untransfected cells under BTT-exposed condition (Figure 3D). In another experiment, we used c-jun siRNA to suppress AP-1 activity. As shown in Figure 3E, c-jun siRNA almost completely suppressed the expression of nuclear phospho-c-jun in DC2.4 cells (top panel). However, no change was observed in BFT-induced HO-1 protein expression between AP-1-suppressed and unsuppressed cells (Figure 3E, bottom panel).

Figure 3

Effects of AP-1 suppression on heme oxygenase-1 expression in dendritic cells stimulated with Bacteroides fragilis enterotoxin. A and B: Bone marrow-derived dendritic cells (DCs) (A) and DC2.4 cells (B) were treated with Bacteroides fragilis toxin (BFT) (100 ng/mL) for the indicated periods. AP-1 DNA binding activity was assessed by EMSA and expression of phospho-c-jun in nuclear extracts was detected using immunoblot. Results are representative of more than three independent experiments. C: DC2.4 cells were transfected with lentivirus containing dominant-negative c-jun plasmid (dn-c-jun) or control virus (GFP). Transfected cells were stimulated with BFT (100 ng/mL) for 1 h. AP-1 binding activity was assayed by EMSA (top panel). Immunoblot results for concurrent phospho-c-jun and lamin B in nuclear extracts under the same conditions are provided beneath the EMSA (middle panel). Expression of heme oxygenase-1 (HO-1) and actin proteins was analyzed by immunoblot (bottom panel). Results are representative of more than three independent experiments. D: Transfected DC2.4 cells were treated with BFT (100 ng/mL) for the indicated periods. Levels of HO-1 mRNA were analyzed by quantitative RT-PCR using a standard RNA. The values are expressed as mean ± SD (n = 5). The β-actin mRNA levels in each group remained relatively constant throughout the same periods (approximately 106 transcripts/μg total RNA). E: DC2.4 cells were transfected with AP-1 c-jun-specific silencing siRNA or NS-RNA as a control for 48 h, after which cells were combined with BFT (100 ng/mL) for 1 h. Nuclear extracts were analyzed by immunoblotting with the indicated Abs (top panel). Transfected cells were stimulated with BFT (100 ng/mL) for 24 h. Expression of HO-1 and actin was detected by immunoblot (bottom panel). Results shown are representative of more than three independent experiments. HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

To confirm these results, BM-derived DCs were preincubated with NF-κB inhibitor Bay 11-7082 or AP-1 inhibitor SR11302 for 30 min, and BFT was then added to the culture system. As shown in Figure 4A, there was no significant difference between the group treated with Bay 11-7082 + BFT and the group treated with BFT alone. A similar result was observed between the group treated with SR11302 + BFT and the group treated with BFT alone. Consistent with these findings, no significant changes in BFT-induced HO-1 expression in BM-derived DCs were observed between the three groups consisting of combined treatment with Bay 11-7082 and BFT, combined treatment with SR11302 and BFT, and BFT treatment alone (Figure 3B).

Figure 4

Relationship between the suppression of NF-κB or AP-1 activity and heme oxygenase-1 expression in bone marrow-derived dendritic cells stimulated with Bacteroides fragilis enterotoxin. A: Bone marrow (BM)-derived dendritic cells (DCs) were treated with Bacteroides fragilis toxin (BFT) (100 ng/mL) for 24 h, respectively. The expression of heme oxygenase-1 (HO-1) and actin was analyzed by immunoblot. Results are representative of more than three independent experiments. B: BM-derived DCs were preincubated with the NF-κB inhibitor Bay 11-7082 (50 μmol/L) or the AP-1 inhibitor SR11302 (10 μmol/L) for 30 min, followed by stimulation with BFT (100 ng/mL) for an additional 24 h. Expression levels of HO-1 protein were measured by ELISA (mean ± SE, n = 5). NS: Statistically non-significant; HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

Activation of Nrf2 is required to upregulate HO-1 expression in BFT-exposed DCs

Since there was no evidence for BFT-induced activation of Nrf2 signaling in DCs, we first examined whether BFT stimulation could activate Nrf2 signals in DCs. As shown in Figure 5A, BFT enhanced DNA-binding activity of Nrf2 in murine BM-derived DCs. Similar results were found in BFT-exposed DC2.4 cells (Figure 5B). To confirm the specificity of Nrf2-DNA binding, two assays, including a competition assay using cold Nrf2 and an inhibition assay using anti-Nrf2 Ab, were performed. In the first experiment, the addition of excess Nrf2 oligomer (cold Nrf2) markedly decreased Nrf2-DNA binding in comparison to no addition of Nrf2 oligomer (hot Nrf2) under BFT-exposed condition (Figure 5C). In the second experiment, treatment with anti-Nrf2 Ab definitely inhibited Nrf2-DNA binding in nuclear extracts from BM-derived DCs, as assessed by supershift assay (Figure 5D).

Figure 5

Activation of Nrf2 in dendritic cells stimulated with Bacteroides fragilis enterotoxin. A and B: Bone marrow (BM)-derived dendritic cells (DCs) (A) and DC2.4 cells (B) were treated with BFT (100 ng/mL) for the indicated periods. Nrf2 DNA binding activity was assessed by EMSA. Immunoblot results for concurrent phospho-Nrf2 and lamin B in nuclear extracts are provided beneath the EMSA. C and D: Competition and supershift assays for Nrf2 signals. C: BM-derived DCs were treated with BFT (100 ng/mL) for 6 h and nuclear extracts were then prepared. The competition assay for Nrf2 signals was performed by adding a 100-fold excess of the unlabeled probe (“cold” probe) before the addition of the radiolabeled probe (“hot” probe) or a mutant probe to the reaction (top panel). D: Supershift assays using nuclear extracts were performed using anti-Nrf2 Ab and IgG isotype control Ab (bottom panel). Results are representative of more than three independent experiments. E: DC2.4 cells were transfected with Nrf2-specific shRNA or control RNA. Transfected cells were combined with BFT (100 ng/mL) for 12 h. Nrf2 binding activity was assayed by EMSA (top panel). Transfected cells were treated with BFT (100 ng/mL) for 24 h and the expression of heme oxygenase-1 (HO-1) and actin was analyzed by immunoblot (bottom panel). F: DC2.4 cells were treated with BFT (100 ng/mL) for the indicated periods. The levels of HO-1 mRNA were analyzed by quantitative RT-PCR using a standard RNA. The values are expressed as mean ± SD (n = 5). β-actin mRNA levels in each group remained relatively constant throughout the same periods (approximately 106 transcripts/μg total RNA). aP < 0.05 vs untransfected cells treated with BFT. HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

Based on these results, we next evaluated whether BFT-induced HO-1 expression was related to Nrf2 activation. For these experiments, DC2.4 cells transfected with lentivirus containing Nrf2 shRNA were used. Transfection with Nrf2 shRNA decreased BFT-induced activity of Nrf2-DNA binding in DC2.4 cells (Figure 5E, top panel). In this experimental system, enhanced expression of HO-1 protein in BFT-treated DC2.4 cells were reduced with transfection of Nrf2 shRNA compared with no transfection (Figure 5E, bottom panel). Consistent with this, transfection with Nrf2 shRNA significantly inhibited HO-1 mRNA expression in BFT-stimulated DC2.4 cells compared with no transfection (Figure 5F). An additional experiment using immunofluorescent microscopy showed that phospho-Nrf2 and HO-1 signals increased in BFT-exposed DC2.4 cells, while Nrf2 shRNA reduced the extent of phospho-Nrf2 and HO-1 signals (Figure 6A). To confirm these results, BM-derived DCs obtained from Nrf2−/− knockout mice were used. As shown in Figure 6B, there was a significant difference in HO-1 expression between DCs from wild-type mice and those derived from Nrf2−/− knockout mice.

Figure 6

Effects of Nrf2 suppression on heme oxygenase-1 expression in dendritic cells stimulated with Bacteroides fragilis s enterotoxin. A: Nrf2 translocation and heme oxygenase-1 (HO-1) expression in B. fragilis enterotoxin (BFT)-stimulated dendritic cells (DCs). DC2.4 cells were transfected with Nrf2-specific shRNA or control RNA. Cells were treated with BFT (100 ng/mL) for 24 h and immunofluorescent microscopy was performed. Each group of cells was stained with the active form-specific anti-Nrf2-Cys Ab (red), anti-HO-1 Ab (green), and DAPI (blue, nucleus). The data are representative of at least five experiments. B: HO-1 expression in cells derived from wild-type and Nrf2−/− knockout mice. BMDCs derived from wild-type or Nrf2−/− knockout mice were exposed to BFT (100 ng/mL) for the indicated periods. Expression of HO-1 protein in each panel was measured by ELISA (mean ± SE, n=5). aP < 0.05 vs each group of cells derived from wild-type mice. HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin; WT: Wild-type; KO: Knockout.

MAPKs are associated with HO-1 induction in BFT-exposed DCs

We further evaluated whether MAPK signaling could be associated with Nrf2 and HO-1 expression in DCs. As shown in Figure 7A, BFT increased phosphorylated signals of MAPKs, including phospho-ERK1/2, phospho-p38, and phospho-JNK, in BM-derived DCs. Similar results were observed in DC2.4 cells (Figure 7B). We next examined whether inhibition of MAPK activity could influence expression of HO-1 in BFT-exposed DCs. As shown in Figure 7C, pretreatment of BM-derived DCs with PD98059 (≥ 10 μmol/L), SB203580 (≥ 10 μmol/L), or SP600125 (≥ 50 μmol/L) significantly inhibited BFT-induced expression of HO-1.

Figure 7

Mitogen-activated protein kinases signals associated with heme oxygenase-1 expression in Bacteroides fragilis enterotoxin-stimulated dendritic cells. A and B: Bone marrow (BM)-derived dendritic cells (DCs) (A) and DC2.4 cells (B) were stimulated with Bacteroides fragilis toxin (BFT) (100 ng/mL) for the indicated periods. ERK1/2, p38, and JNK activities were measured by immunoblot analysis. Results are representative of three independent experiments. C: BM-derived DCs were preincubated with SB203580 (open circle), PD98059 (open triangle), or SP600125 (open square) for 30 min, and then stimulated with BFT (100 ng/mL) for another 24 h. Expression levels of heme oxygenase-1 (HO-1) protein were determined by ELISA. Data are expressed as the mean % increase relative to unstimulated controls ± SE (n = 5). aP < 0.05 vs BFT alone. HO-1: Heme oxygenase-1.

To confirm these results, lentiviral systems containing dominant-negative plasmids were used. Phosphorylation of each MAPK protein was markedly suppressed in DC2.4 cells transfected with lentiviruses containing each dominant-negative plasmid (Figure 8A). Transfection with lentivirus-dn-Erk2 and lentivirus-dn-p38 significantly decreased BFT-induced Nrf2 activation, as assessed by EMSA (Figure 8B). In these experimental systems, cells transfected with lentivirus-dn-Erk2 and lenti-dn-p38 reduced the expression of HO-1 compared with untransfected cells under BFT-treated conditions (Figure 8C). Moreover, lentivirus-dn-Erk2 and lentivirus-dn-p38 significantly inhibited the activities of both phosphorylated Nrf2 and HO-1 in BFT-stimulated cells (Figure 8D and 8E). These results suggest that exposure of DCs to BFT activates a signaling cascade involving ERK and p38 MAPKs, leading to Nrf2 activation and finally to HO-1 induction.

Figure 8

Effects of mitogen-activated protein kinases suppression on heme oxygenase-1 expression in dendritic cells stimulated with Bacteroides fragilis enterotoxin. A: DC2.4 cells were infected with lentiviruses containing either a dominant-negative or control plasmid (GFP). Transfected cells were stimulated with BFT (100 ng/mL) for 30 min and immunoblots were then performed. Results are representative of three independent experiments. B and C: Transfected cells were stimulated with BFT (100 ng/mL) for 3 h (Nrf2) or 24 h (heme oxygenase-1, HO-1). B: DNA binding activities of Nrf2 were evaluated by EMSA. C: Expression of HO-1 and actin was analyzed by immunoblot. Results are representative of more than three independent experiments. D: Transfected cells were stimulated with BFT (100 ng/mL) for 3 h. Phospho-Nrf2 activities were measured using an ELISA kit. Data are expressed as mean fold induction ± SE of Nrf2 relative to untreated controls (n = 5). E: Transfected cells were stimulated with BFT (100 ng/mL) for 24 h. Transfected cells were either left untreated or stimulated with BFT (100 ng/mL) for another 6 h (Nrf2) or 24 h (HO-1). Each ELISA kit measured activities of phospho-IκBα and Nrf2, as well as HO-1 expression. Data are expressed as mean fold induction ± SE (%) relative to untreated controls (n = 5). aP < 0.05. HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

HO-1 induction is dependent on ROS generation in BFT-exposed DCs

Although BFT is reported to induce the generation of ROS in T84 intestinal epithelial cells[27], there are no reports regarding BFT-induced ROS generation in DCs. In the present study, we demonstrated that BFT markedly increased intracellular ROS generation in DC2.4 cells, while antioxidant NAC significantly inhibited it (Figure 9A). In this experimental system, treatment with NAC attenuated the increased levels of phospho-ERK and phospho-p38 in DC2.4 cells exposed to BFT (Figure 9B). Upregulated expression of both phospho-Nrf2 and HO-1 were also reduced in the presence of NAC under BFT-stimulated conditions, indicating that ROS seems to regulate the overall signaling process of inducing HO-1 expression in BFT-exposed DCs.

Figure 9

Reactive oxygen species mediated Bacteroides fragilis enterotoxin-induced heme oxygenase-1 expression in dendritic cells. A: DC2.4 cells were stimulated with BFT (100 ng/mL) in the absence or presence of the antioxidant N-acetyl-L-cysteine (NAC, 0.5 mmol/L) for 6 h. Production of reactive oxygen species (ROS) was measured by a commercially available ROS detection kit. Data are expressed as mean fold induction ± SE (%) relative to untreated controls (n = 5). aP < 0.05. B: DC2.4 cells were stimulated with BFT (100 ng/mL) in the absence or presence of NAC (0.5 mmol/L) for 30 min (phospho-ERK and phospho-p38), 3 h (phospho-Nrf2), or 24 h (heme oxygenase-1, HO-1). The effects of NAC on each protein level were determined using immunoblot. Results are representative of three independent experiments. NAC: N-acetyl-L-cysteine; HO-1: Heme oxygenase-1; BFT: Bacteroides fragilis toxin.

DISCUSSION

ETBF is a noninvasive bacterium associated with pathogenic effects in the intestine[2]. Since invasion of ETBF into the surface epithelium from the intestine has not been reported and no bacteremia has been observed in infected rabbit models[2,28], the produced BFT seems to be primarily present in the lumen. Organized and diffuse lymphoid tissues are found in the intestinal mucosa layer and DCs are abundant in the lamina propria. DCs can extend dendritic processes between intestinal epithelial cells into the lumen to sample antigens. In addition, BFT can destroy the tight junctions in the intestinal epithelium by cleaving E-cadherin[3-5] and the secreted BFT may come into direct contact with DCs. Therefore, BFT may be exposed to DCs at the site of ETBF infection. In experiments reported here, we demonstrated that the exposure of DCs to BFT could upregulate expression of HO-1 at the mRNA and protein levels.

Transcription factors such as NF-κB, AP-1, and Nrf2 regulate a variety of inflammatory responses and their promoter regions of HO-1 contain binding sites for these transcription factors[9,12,29]. We previously demonstrated that stimulation of intestinal epithelial cells with BFT activate NF-κB and AP-1 signaling[12]. However, there have been no reports on whether BFT may activate these transcription factors in DCs. The present study showed that signals of NF-κB, AP-1, and Nrf2 were activated by exposure of DCs to BFT. However, whether HO-1 induction of DCs may be regulated by NF-κB, AP-1 or Nrf2 remains controversial. In the present study, suppression of NF-κB activity either by transfection with lentivirus-IκBα-AA and p65 siRNA, or pretreatment with chemical inhibitor Bay 11-7082 did not significantly reduce BFT-induced HO-1 expression in DCs. In addition, the suppression of AP-1 signals did not result in a significant change in HO-1 expression. In contrast, the suppression of BFT-induced activation of Nrf2 led to the downregulation of HO-1 in DCs assessed by transfection with Nrf2 shRNA. These results were confirmed by experiments using DCs isolated from Nrf2−/− knockout mice. Our results differ from previous findings that LPS-induced HO-1 expression is mediated by an NF-κB-dependent pathway in DCs[30]. In addition, the present results are different from our previous study, in which H. pylori outer membrane vesicles induced HO-1 expression through both NF-κB- and Nrf2-dependent pathway in DCs[9]. Therefore, this Nrf2-dependent and both NF-κB- and AP-1-independent expression of HO-1 may be a distinctive signature of DCs exposure to BFT.

Kinetics of both NF-κB and AP-1 signaling in DCs resemble those in intestinal epithelial cells stimulated with BFT when comparing the present and previous results[12]. However, the kinetics of Nrf2 signals induced by BFT are different in DCs and intestinal epithelial cells. The present study showed that Nrf2 signals in DCs continued to increase over the ensuing 24 h following stimulation. In contrast, our previous study showed that the activation of Nrf2 in intestinal epithelial cells treated with BFT peaked between 1 h and 6 h after stimulation and then decreased[12]. Compared with previous results, the activation of Nrf2 in DCs was delayed compared to the response of intestinal epithelial cells to BFT stimulation. The delayed activation of Nrf2 seems to be associated with the delayed upregulation of HO-1 expression in BFT-exposed DCs.

MAPK signaling is known to be an important event underlying HO-1 expression[11,31,32]. In the present study, suppression of ERK or p38 MAPK signals in BFT-treated DCs resulted in significant inhibitions of both Nrf2 activation and HO-1 expression. Considering that suppression of p38 MAPK results in significant attenuation of BFT-induced NF-κB and HO-1 activities in intestinal epithelial cells[12], two differential pathways may be involved in BFT-induced HO-1 expression. That is, the exposure of DCs to BFT can activate a signaling cascade involving ERK and p38 MAPKs, leading to Nrf2 activation and HO-1 induction. In contrast, BFT-exposed intestinal epithelial cells can activate a signaling cascade involving p38 MAPKs, leading to NF-κB activation and finally to HO-1 induction.

Since ROS production is known to be related to the activation of MAPK signaling[33] and BFT increase ROS production in intestinal epithelial cells[27], we investigated the role of ROS in the regulation of MAPK and Nrf2 signaling. In the present study, exposure of DCs to BFT enhanced ROS production and treatment of BFT-exposed DCs with the antioxidant NAC significantly inhibited the activation of ERK and p38 MAPK signals. In addition, both Nrf2 activation and HO-1 expression were attenuated in the presence of NAC under BFT-stimulated conditions. Based on these results, increased intracellular ROS is proposed as the mechanism allowing BFT to contribute to ERK/p38 MAPK pathway-mediated Nrf2 activation and HO-1 expression in DCs.

BFT has been shown to not directly induce DC maturation[8]. Nevertheless, many papers have demonstrated that HO-1 expression is associated with inhibition of DC maturation[31,34,35]. Therefore, BFT-induced HO-1 upregulation seems to affect the maturation process of DCs and consequently inhibit maturation. Further studies are needed to clarify the role HO-1 plays in DC maturation in ETBF infection.

Upregulated HO-1 is likely to attenuate acute inflammation in ETBF infection. The rationale for this supposition is that HO-1 controls a variety of infections in mice, including Mycobacterium avium[36], Listeria monocytogenes[37], and Salmonella Typhimurium[38]. Further, HO-1 expression induces anti-inflammatory cytokine IL-10 production[34,39] and HO-1 mediates the anti-inflammatory effect of IL-10[40]. Based on these results, upregulated HO-1 may be an important mediator of the anti-inflammatory effects of DCs in acute ETBF infection. However, further studies are required to clarify the anti-inflammatory effects in BFT-stimulated DCs.

In summary, we demonstrated that exposure of DCs to BFT resulted in ROS-mediated activation of MAPK signaling, which then led to the induction of HO-1 molecules via Nrf2 signaling pathway in DCs.

ARTICLE HIGHLIGHTS

Research background

Enterotoxigenic Bacteroides fragilis (ETBF) causes colitis and diarrhea, and is considered a candidate pathogen in inflammatory bowel diseases as well as colorectal cancers. These diseases are dependent on ETBF-secreted toxin (BFT). Dendritic cells (DCs) play an important role in directing the nature of adaptive immune responses to bacterial infection and heme oxygenase-1 (HO-1) is involved in the regulation of DC function.

Research motivation

Although BFT can activate such transcription factor signaling in intestinal epithelial cells, there is no evidence that signals associated with BFT-induced transcription factors are related to HO-1 induction in DCs. These led us to this study.

Research objectives

The present study aimed to investigate the role of BFT in HO-1 expression in DCs.

Research methods

Murine DCs were generated from specific pathogen-free C57BL/6 and Nrf2−/− knockout mice. DCs were exposed to BFT, after which HO-1 expression and the related signaling factor activation were measured by quantitative RT-PCR, EMSA, fluorescent microscopy, immunoblot, and ELISA.

Research results

HO-1 expression was upregulated in DCs stimulated with BFT. Although BFT activated transcription factors such as NF-κB, AP-1, and Nrf2, activation of NF-κB and AP-1 was not involved in the induction of HO-1 expression in BFT-exposed DCs. Instead, upregulation of HO-1 expression was dependent on Nrf2 activation in DCs. Moreover, HO-1 expression via Nrf2 in DCs was regulated by mitogen-activated protein kinases (MAPKs) such as ERK and p38. Furthermore, BFT enhanced the production of reactive oxygen species (ROS) and inhibition of ROS production resulted in a significant decrease of phospho-ERK, phospho-p38, Nrf2, and HO-1 expression.

Research conclusions

These results suggest that signaling pathways involving ROS-mediated ERK and p38 MAPK-Nrf2 activation in DCs are required for HO-1 induction during exposure to ETBF-produced BFT.

Research perspectives

Upregulated HO-1 expression in DCs will help explain the pathogenesis of the ETBF infection. In addition, upregulated HO-1 may be an important mediator of the anti-inflammatory effects of DCs in acute ETBF infection. However, further studies are required to clarify the anti-inflammatory effects in BFT-stimulated DCs.