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Introduction

Myocardial infarction (MI) is a key manifestation of cardiovascular disease (1). According to the Centers for Medicare & Medicaid Services Hospital Inpatient Quality Reporting Program data on 2,363 hospitals in 2018, the average mortality of acute MI was 13.6% (2). MI is the injury and necrosis of myocardial cells caused by a sudden decrease in coronary blood flow, continuous myocardial ischemia and hypoxia (3,4). In clinical practice, the primary application of percutaneous coronary intervention is to promptly restore coronary blood transport and save the dying myocardium (5,6). Left ventricular remodeling following MI can have serious consequences, such as heart failure and rupture, and is the primary cause of death in patients with MI (1). Therefore, delaying or preventing left ventricular remodeling is an important step in preventing heart failure following MI. However, the detailed mechanisms underlying MI remain unclear. Therefore, it is important to investigate the mechanisms of MI injury, which may help to develop novel therapies for myocardial injury.

Programmed cell death includes necroptosis, parthanatos, oxytosis, ferroptosis, extracellular trap (ET)osis, neutrophil ETosis and pyroptosis (7). Pyroptosis leads to myocardial perforation and rupture of the cell membrane and releases pro-inflammatory factors such as interleukin-1β (IL-1β) and IL-18, initiated by caspase-1, causing a local inflammatory response (8). Previous studies have found that pyroptosis serves an important role in cardiovascular disease progression (including atherosclerosis, MI, ischemia-reperfusion, diabetic cardiomyopathy and heart failure) (9–11).

A previous study indicated that the inflammatory body-caspase axis serves an important role in inflammation-induced cell death following ischemia-reperfusion (10). The inflammasome is a complex that can transform pro-caspase-1 into activated caspase-1. Activated caspase-1 can convert pro-IL-1β and pro-IL-18 into mature IL-1β and IL-18, cleave gasdermin D (GSDMD) into the GSDMD-N terminal with a pore-forming effect and induce pyroptosis (12). GSDMD, a member of the GSDM family, is a common substrate for caspase-1,-4, −5 and −11 and mediates pyroptosis by producing an N-terminal fragment (13,14). Active caspase-1, −4 −11 cleave GSDMD in response to canonical and non-canonical inflammasome activation (15). Moreover, GSDMD inhibition improves cardiac function and decreases infarct size by attenuating cardiomyocyte pyroptosis (16,17). The role of pyroptosis and the mechanism of its occurrence and development in the MI process remain to be elucidated, which may provide novel directions and strategies for the clinical treatment of cardiovascular disease.

Interferon regulators (IRFs) are multifunctional transcription factors that serve an important regulatory role in the interferon signaling pathway, which is involved in host immune response, cell differentiation and immune regulation (18). IRF2 is a member of the IRF family of transcription factors (19), which can transcriptionally induce direct target genes, including toll-like receptor 3, Bcl-11a and GSDMD (20–22). Kayagaki et al (22) found that IRF2 transcriptionally induces GSDMD expression in pyroptosis and directly drives GSDMD mRNA expression. GSDMD expression is significantly decreased in IRF2-deficient macrophages, endothelial cells and multiple types of tissue, corresponding to decreased IL-1 secretion and inhibition of pyroptosis (22). However, its functional contribution to MI remains unclear and requires further clarification.

The present study investigated the effect of IRF2 in MI injury and clarified the potential mechanism of IRF2 involvement in MI via GSDMD-induced pyroptosis.

Materials and methods

Bioinformatics analysis

GeneMANIA (23), a web tool that can identify other proteins associated with a set of input genes, was used to generate protein-protein interaction (PPI) network images. The associations between co-expression, colocalization, predicted related genes, shared protein domains, genetic interactions and physical interactions were determined using GeneMANIA.

Animals and MI model in vivo

A total of 25 male C57BL/6 mice (aged 6–8 weeks; weight, 20–26 g) were provided by Ai Ling Fei (Nanjing, China). Mice were maintained at 23–25°C with 60–70% humidity, 12-h light/dark cycles and access to normal chow diet and water. The mice were divided into the following five groups (n=5 per group): i) Control (Con); ii) sham; iii) MI; iv) MI + sh-NC; and v) MI + sh-IRF2. Untreated mice were set as the con group. For shRNAs transfection in vivo, mice were injected with lentivirus-IRF2-short hairpin (sh)RNA (sh-IRF2 forward, GGTCCTGACTTCAACTATA; reverse, TATAGTTGAAGTCAGGACC) or lentivirus-scramble (forward, UUCUCCGAACGUGUCACGUTT; reverse, ACGUGACACGUUCGGAGAATT) (both 1×109 viral particles/mouse, Shanghai GenePharma Co., Ltd.) via the tail vein. After 7 days, a mouse model of MI was generated by ligation of the left anterior descending coronary artery, as previously described (24). Briefly, mice were anesthetized with 45 mg/kg 1% pentobarbital sodium intraperitoneal injection and then underwent open-heart surgery. The MI model was established by threading a 7/0 surgical thread 2 mm under the left auricle and ligating the anterior descending branch of the left coronary artery for 24 h. In the sham group, a parallel operation was performed, however, the thread was threaded without ligation. After operation, 40,000 units of penicillin (Thermo Fisher Scientific, Inc.) were injected intraperitoneally daily for 3 consecutive days.

Cell culture and MI model in vitro

H9c2 cells were purchased from EK Biosciences GmbH (Shanghai, China) and cultured in Dulbecco's Modified Eagle Medium containing 10% foetal bovine serum (both Thermo Fisher Scientific, Inc.) at 37°C with 5% CO2. To establish an MI injury model in vitro, H9c2 cells were exposed to a hypoxia incubator (1% oxygen, 5% CO2 and 94% N2) for 6, 12, 24 and 48 h. Untreated cells were set as Con group.

Histopathological examination and immunohistochemical (IHC) staining

At 24 h after the surgery, the were mice were euthanized by intraperitoneal injection of 50 mg/kg, followed by dislocation of the cervical spine. The heart tissue samples were fixed in 4% paraformaldehyde at room temperature for 24 h, embedded in paraffin and sectioned into 5 µm slices. The slices were stained with hematoxylin-eosin (H&E) for 7 min at room temperature and photographed using a light microscope (×400 magnification; Nikon Eclipse TE2000-U; Nikon Corporation). For IHC staining of IRF2, the tissue slices were deparaffinized in xylene, dehydrated with graded ethanol solutions and rehydrated in PBS. The slices then were incubated with 3% H2O2 at 37°C for 10 min to block endogenous peroxidase activity. For antigen retrieval, the slices were treated with PBS (pH 9) for 15 min at 95°C in a microwave oven and then cooled in running water. Subsequently, slices were incubated with normal goat serum sealant (Shanghai Haoran Biotechnology Co., Ltd.) for 20 min at room temperature. Slices were then incubated with anti-IRF2 antibody (cat. no. PA5-83159; 1:200; Sigma-Aldrich; Merck KGaA) in a humidified chamber at 4°C overnight and were visualized with DAB at room temperature for 2 min and counterstained with hematoxylin at room temperature for 5 min.

Echocardiographic measurement

Transthoracic echocardiography was performed 24 h after surgery in mice post-MI using an echocardiography system equipped with a 12-MHz phased-array transducer. The left ventricular ejection fraction (EF) and fractional shortening (FS) were measured using M-mode tracing. All experiments were performed by professional technicians who were blinded to the experimental groups.

Western blotting

Total protein samples from H9c2 cells and heart tissue were extracted by using RIPA lysis buffer containing 1 mM phenylmethylsulfonyl fluoride (Beyotime Institute of Biotechnology). The total protein concentrations were determined using a bicinchoninic acid Protein Assay kit (Beyotime Institute of Biotechnology). Proteins (30 µg per lane) were separated using 10% SDS-PAGE (Beyotime Institute of Biotechnology) and then transferred to PVDF membranes. The membranes were blocked in 5% skimmed milk for 1 h and then incubated overnight at 4°C with primary antibodies. The blot was probed using the following primary antibodies: IRF2 (cat. no. A303-380A-T; 1:1,000; Thermo Fisher Scientific, Inc.), cleaved caspase-1 (c-caspase-1; cat. no. PA5-77886; 1:1,000; Thermo Fisher Scientific, Inc.), GSDMD (cat. no. PA5-30823; 1:1,000; Thermo Fisher Scientific, Inc.), GSDMD-N (cat. no. ab215203; 1:1,000; Abcam), IL-1β (cat. no. P420B; 1:1,000; Thermo Fisher Scientific, Inc.), IL-18 (cat. no. PA5-79477; 1:1,000; Thermo Fisher Scientific, Inc.), and GAPDH (cat. no. ab8245; 1:5,000; Abcam), followed by incubation with goat anti-rabbit IgG secondary antibody (cat. no. G-21234; 1:10,000; Thermo Fisher Scientific, Inc.) at room temperature for 1 h. Protein bands were visualized by enhanced chemiluminescence Pierce™ ECL Western Blotting Substrate (cat. no. 32209; Thermo Fisher Scientific, Inc.). The densitometry analysis was performed using ImageJ software (version 1.8.0; National Institutes of Health).

TUNEL staining

Myocardial tissue apoptosis was measured using a In Situ Cell Death Detection Kit (Sigma Aldrich; Merck KGaA) according to the manufacturer's instructions. For the TUNEL staining, the heart tissue samples were fixed in 4% paraformaldehyde at room temperature for 24 h, embedded in paraffin and sectioned into 5-µm slices. The slices were deparaffinized in xylene, dehydrated with graded ethanol solutions and rehydrated in PBS, and then treated with 25 µg/ml proteinase K for 8 min at room temperature. Then, the slices were stained with the TUNEL reaction mixture containing TdT and TMR-dUTP for 1 h at 37°C in the dark. After applying stop solution for 10 min at room temperature, streptavidin-HRP working solution (50 µl) was added at room temperature for 30 min, followed by incubation with DAB (50 µl) solution at room temperature for 10 min. The color was then developed using 3,3-diaminobenzidine (Sigma-Aldrich; Merck KGaA). A total of five fields of view were randomly selected to count the TUNEL-positive cells under a light microscope (×400 magnification) and the proportion of TUNEL-positive cells was calculated.

Determination of cellular apoptosis

H9c2 cells were cultured at room temperature in 6-well plates at a density of 1×105 cells/well to evaluate pyroptosis. After hypoxia treatment, the treated H9c2 cells were harvested and incubated with Annexin V-fluorescein isothiocyanate and propidium iodide for 15 min at 4°C. The samples were analyzed using a flow cytometer (BD Accuri C6 Plus; BD Biosciences) with FlowJo software (v10.6.2; FlowJo, LLC) according to the manufacturer's instructions.

Chromatin immunoprecipitation (ChIP) assay

The ChIP assay was performed with the ChIP Assay kit (cat. no. P2078; Beyotime Institute of Biotechnology) according to the manufacturer's protocol. Briefly, H9c2 cells (1×105) were incubated with 1% formaldehyde for 10 min at 25°C to crosslink the protein and DNA. Glycine (Beijing Solarbio Technology Co., Ltd.) was then used to terminate the crosslinking. H9c2 cells were centrifugated at 1,000 × g for 2 min at 4°C, resuspended in the lysis buffer (0.2 ml) at at 4°C for 10 min. The Ch fragments were obtained by shearing crosslinked complex DNA with ultrasound, followed by IP with the antibody directed against anti-IRF2 (cat. no. ab245658; 1:100; Abcam) overnight at 4°C, taking IgG as a negative control. Ch fragments were detected by PCR.

RNA extraction and reverse transcription-quantitative PCR (RT-qPCR)

Total RNA was isolated from H9c2 cells using RNAsimple Total RNA Kit (cat. no. DP419; Tiangen Biotech Co., Ltd.) and RNA was reverse transcribed into cDNA using a PrimeScript® RT reagent kit (Takara Bio, Inc.) according to the manufacturer's protocol. Subsequently, qPCR was performed using the SYBR Premix Ex Taq™ II kit (Thermo Fisher Scientific, Inc.) and an ABI Prism 7700 sequence detector (Applied Biosystems; Thermo Fisher Scientific, Inc.). The sequences of the PCR primers used were as follows: GSDMD forward, 5′-TCTGCCCTCAACACTTCTGG-3′ and reverse, 5′-TGCAGCCACAAATAACTCAGC-3′; and GAPDH forward, 5′-GAAGGTCGGAGTCAACGGATT-3′ and reverse, 5′-TTCCCGTTCTCAGCCATGT-3′. The following thermocycling conditions were used: 90°C for 5 min; then 90°C for 15 sec and 60°C for 30 sec for 45 cycles. Expression levels were quantified using the 2−∆∆Cq method (25) and normalized to the internal reference gene GAPDH.

Dual-luciferase reporter assay

The recombinant luciferase reporter plasmids containing the GSDMD promoter (pEZX-PG04-GSDMD), pcDNA3.1 vector (pc-NC, 100 nM), IRF2 overexpression vector (IRF2, 100 nM), IRF2 short hairpin (sh)RNA (sh-IRF2 forward, GGTCCTGACTTCAACTATA; reverse, TATAGTTGAAGTCAGGACC; 100 nM) or negative control (sh-NC forward, UUCUCCGAACGUGUCACGUTT; reverse, ACGUGACACGUUCGGAGAATT; 100 nM) were co-transfected into H9c2 cells by Lipofectamine™ 3000 transfection reagent (cat. no. L3000001; Thermo Fisher Scientific, Inc.) for 48 h at 37°C. Following 48 h transfection, the luciferase activity was detected using a Dual-Luciferase Reporter Gene Assay Kit (cat. no. 11402ES60; Shanghai Qcbio Science & Technologies Co., Ltd.) according to the manufacturer's instructions. The firefly luciferase activity was normalized to Renilla luciferase activity for each sample.

Statistical analysis

All data were analyzed using GraphPad Prism 9 (GraphPad Software, Inc.) and are expressed as the mean ± SD. All experiments were repeated three times. One-way ANOVA followed by Tukey's multiple comparisons test was used for comparisons between groups. P<0.05 was considered to indicate a statistically significant difference.

Results

IRF2 expression is associated with MI in mice

H&E and IHC staining for IRF2 showed severe MI in MI model mice. IHC analysis revealed a positive association between increased IRF2 expression and MI progression (Fig. 1A and B). Western blotting indicated that IRF2 expression was increased in MI samples compared with that in the con (Fig. 1C). Taken together, these results indicated that IRF2 expression was positively associated with MI progression.

Figure 1. IRF2 expression is associated with MI in mice. (A) Representative hematoxylin and eosin staining in the left ventricle of mice. (B) IRF2 expression in heart tissue of MI mice. Scale bar, 20 µm. (C) Western blotting was used to detect the expression of IRF2 in heart tissue of MI mice. All data are expressed as the mean ± SD (n=3). *P<0.05 vs. Sham. IRF2, interferon regulatory factor 2; MI, myocardial infarction; Con, control.

IRF2 silencing attenuates MI in mice

The effect of IRF2 on MI was investigated. IRF2 shRNA was transmitted to mice using a lentivirus. IRF2 silencing alleviated histological heart damage in the MI + sh-IRF2 group compared with the MI group (Fig. 2A). To understand the effects of IRF2 silencing on MI mice, in vivo cardiac function was measured using transthoracic echocardiography (Fig. 2B). Compared with the sham group, MI significantly decreased EF and FS; this was improved in the MI + sh-IRF2 group (Fig. 2C and D). These data suggested that IRF2 silencing alleviated systolic dysfunction in MI mice.

Figure 2. IRF2 silencing attenuates MI in mice. (A) Representative hematoxylin and eosin staining in the left ventricle of mice following IRF2 silencing. Scale bar, 20 µm. Arrows indicate alleviation of histological heart damage. (B) After silencing IRF2, cardiac function of mice was measured by transthoracic echocardiography to assess (C) EF and (D) FS. All data are expressed as the mean ± SD (n=3). *P<0.05 vs. Sham; #P<0.05 vs. MI + sh-NC. IRF2, interferon regulatory factor 2; MI, myocardial infarction; EF, ejection fraction; FS, fractional shortening; sh, short hairpin; NC, negative control.

IRF2 silencing attenuates GSDMD-induced pyroptosis in vivo

Pyroptosis, a new form of inflammatory programmed cell death, has been shown to aggravate MI following cardiomyocyte loss (16). To investigate the protective effect of IRF2 silencing on MI by decreasing pyroptosis, TUNEL staining was used to evaluate pyroptotic cell death in the MI model. Cardiac pyroptosis and the number of TUNEL-positive cells increased in the MI group and IRF2 silencing significantly inhibited cardiac pyroptosis (Fig. 3A). Western blot analysis revealed that MI resulted in the upregulation of c-caspase-1, IL-1β, IL-18, GSDMD-N and GSDMD 24 h after MI; IRF2 silencing significantly inhibited expression of c-caspase-1, IL-1β, IL-18, GSDMD-N and GSDMD protein levels induced by MI (Fig. 3B and C).

Figure 3. IRF2 silencing attenuates GSDMD-induced pyroptosis in vivo. (A) Myocardial apoptosis of mice was detected by TUNEL staining. Scale bar, 20 µm. (B) Effect of silencing IRF2 on expression of (B) c-caspase-1, GSDMD-N and GSDMD and (C) IL-1β and IL-18 in heart tissue of MI model mice. All data are expressed as the mean ± SD (n=3). *P<0.05 vs. Sham; #P<0.05 vs. MI + sh-NC. IRF2, interferon regulatory factor 2; GSDMD, gasdermin D; c-, cleaved; MI, myocardial infarction; sh, short hairpin; NC, negative control.

IRF2 silencing attenuates GSDMD-induced pyroptosis in vitro

One of the key events in MI is hypoxia, which also promotes pyroptosis (26,27). To determine whether IRF2 silencing prevented pyroptosis in cardiomyocytes, H9c2 cells were cultured under hypoxic conditions for 6, 12, 24 and 48 h. Exposure of H9c2 cells to hypoxia (6–48 h) induced a time-dependent increase in IRF2 expression (Fig. 4A). Compared with the NC group, IRF2 expression was significantly decreased in the sh-IRF2 group and significantly increased in the IRF2 overexpression group (Fig. 4B). Hypoxia markedly elevated the rate of programmed cell death, and IRF2 silencing significantly decreases the rate of programmed cell death, and IRF2 overexpression aggravated the rate of programmed cell death compared with the hypoxia group (Fig. 4C). Western blot analysis showed that hypoxia resulted in the upregulation of c-caspase-1, IL-1β, IL-18, GSDMD-N and GSDMD (Fig. 4D and E). Moreover, IRF2 silencing significantly inhibited the protein expression of c-caspase-1, IL-1β, IL-18, GSDMD-N and GSDMD induced by hypoxia. These results suggested that IRF2 silencing attenuated GSDMD-induced pyroptosis in vitro.

Figure 4. IRF2 silencing attenuates GSDMD-induced pyroptosis in vitro. (A) IRF-2 expression in H9c2 cells stimulated by hypoxia (6, 12, 24 and 48 h) was detected by reverse transcription-quantitative PCR. *P<0.05 vs. Con. (B) IRF2 expression was detected by western blotting. *P<0.05 vs. sh-NC; #P<0.05 vs. pc-NC. (C) Following transfection of sh-IRF2 and IRF2, apoptosis of H9c2 cells was detected by flow cytometry under hypoxic conditions. &P<0.05 vs. Hypoxia + pc-NC, *P<0.05 vs. Con; #P<0.05 vs. Hypoxia+sh-NC. Following transfection of sh-IRF2 and IRF2, the expression of (D) c-caspase-1, GSDMD-N, GSDMD, (E) IL-1β, and IL-18 was detected by western blotting under hypoxic conditions. *P<0.05 vs. Con; #P<0.05 vs. Hypoxia + sh-NC. All data are expressed as the mean ± SD (n=3). IRF2, interferon regulatory factor 2; GSDMD, gasdermin D; c-, cleaved; MI, myocardial infarction; sh, short hairpin; NC, negative control; Con, control.

IRF2 is key for the transcriptional activation of GSDMD

Co-expression of IRF2 and upstream genes recorded in GeneMANIA (28) (genemania.org/) showed that IRF2 may interact with HIF-1, indicating an association between HIF-1 and IRF2 (Fig. 5A). Exposure of H9c2 cells to hypoxia (6–48 h) induced a time-dependent increase in the expressions of IRF2 and HIF-1 (Fig. 5B). These data suggested that IRF2 expression may be regulated by the HIF-1 pathway in hypoxia-stimulated H9c2 cells. To verify whether IRF2 directly drives GSDMD in hypoxia-induced H9c2 cells, ChIP-PCR and dual-luciferase reporter assay were used to evaluate effect of IRF2 on GSDMD transcriptional activity. ChIP-PCR analysis of H9c2 cells using specific antibodies against IRF2 showed IRF2 was bound to the GSDMD promoter (Fig. 5C). Furthermore, dual-luciferase reporter assay showed that IRF2 overexpression increased GSDMD promoter activity and IRF2 silencing decreased GSDMD promoter activity (Fig. 5D). These findings demonstrated that IRF2 bound directly to the GSDMD promoter. Western blot analysis showed that treatment of cells with hypoxia and sh-IRF2 inhibited c-caspase-1, GSDMD-N, and GSDMD protein expression in H9c2 cells (Fig. 5E). Moreover, GSDMD overexpression increased the expression levels of c-caspase-1, GSDMD-N and GSDMD. These data suggested that IRF2 silencing alleviated MI and hypoxia-induced cardiomyocyte pyroptosis via transcriptional activation of GSDMD.

Figure 5. IRF2 is key for the transcriptional activation of GSDMD. (A) Co-expression of IRF2 and upstream genes was detected in GeneMANIA database. (B) HIF-1 and IRF-2 expression in H9c2 cells were stimulated following hypoxia (6, 12, 24 and 48 h). *P<0.05 vs. Con. (C) Chromatin immunoprecipitation-PCR was used to evaluate the transcriptional activity of IRF2 on GSDMD. *P<0.05 vs. IgG. (D) Dual-luciferase reporter assay was used to evaluate the effect of IRF2 on GSDMD transcriptional activity. *P<0.05 vs. pc-NC; #P<0.05 vs. sh-NC. (E) Following transfection of sh-IRF2 and GSDMD, the expression of c-caspase-1, GSDMD-N and GSDMD was detected by western blotting under hypoxic conditions. *P<0.05 vs. Normoxia; #P<0.05 vs. Hypoxia; &P<0.05 vs. Hypoxia + GSDMD. All data are expressed as the mean ± SD (n=3). IRF2, interferon regulatory factor 2; GSDMD, gasdermin D; HIF-1, hypoxia inducible factor-1; Con, control; sh, short hairpin; NC, negative control; c-, cleaved.

Discussion

The present study addressed the key role of IRF2 in MI. First, IRF2 expression was significantly increased in an MI mouse model and hypoxia-treated H9c2 cells, and the level of IRF2 expression was positively associated with duration of hypoxia in H9c2 cells. Second, IRF2 silencing alleviated MI and hypoxia-induced cardiomyocyte pyroptosis in vivo and in vitro. Third, IRF2 was key for the transcriptional activation of GSDMD in cardiomyocytes. Therefore, IRF2 is a novel therapeutic target for treating MI.

Despite the use of advanced therapeutic interventions (29,30), MI remains the leading cause of death from cardiovascular disease (31). Pyroptosis is a newly identified form of programmed cell death that is mediated by inflammatory caspase-1, accompanied by release of a large number of pro-inflammatory factors and induces a cascade of amplified inflammatory responses (32); it is associated with numerous diseases, including MI and myocardial cell loss following ischemia-reperfusion (33,34). IRF2 is a member of the IRF family and combines with interferon gene promoters to serve a key role in immune response and promote cell proliferation (35). Previous studies found that IRF2 is involved in various cancer mechanisms, including liver, lung and gastric cancer (36–38). To the best of our knowledge, however, there are few reports of its involvement in cardiovascular disease, particularly in MI. Recently, Kayagaki et al (22) found that IRF2 transcription induces GSDMD expression to cause pyroptosis. Therefore, it was hypothesized that IRF2 may erve a role in MI by regulating GSDMD-induced pyroptosis. In the present study, IRF2 expression was positively associated with MI progression and IRF2 silencing attenuated MI in mice.

Studies have found that the GSDM family induces cell death and inflammation; in particular, GSDMD is associated with pyroptosis (39–41). Activated caspase-1, −4, −5 and −11 cleave GSDMD protein into the GSDMD-N terminal with pore-forming activity (42). GSDMD-N combines with the cell inner membrane to form a pore, which causes cell swelling and osmotic lysis and induces pyroptosis (42). The present study showed that IRF2 silencing significantly suppressed pyroptosis-associated proteins, including GSDMD, GSDMD-N and c-caspase-1. The inflammatory response caused by MI is key to healing of heart trauma, however, it can also aggravate heart damage and dysfunction (12). MI activates the NLRP3 inflammasome, leading to the conversion of IL-1β and IL-18 into active mature forms in a caspase-1-dependent manner (43). Pro-inflammatory cytokines IL-1 and IL-18 expand infarct size and promote cardiac dysfunction (44). The present results showed that the expression levels of pro-inflammatory cytokines IL-1β and IL-18 increased in the MI group, and IRF2 silencing notably inhibited the expression levels of IL-1β and IL-18. Collectively, these data suggested that IRF2 silencing decreased myocardial injury by attenuating the pro-inflammatory response and decreasing pyroptosis.

Hypoxia stimulates myocardial cell damage and secretion of inflammatory factors, which can partially mimic heart damage in MI (26). Numerous studies have found that hypoxic stimulation activates the NLRP3 inflammasome and pyroptosis to induce cardiomyocyte death (26,27). The present results showed that IRF2 silencing decreased the expression levels of IL-1β, IL-18 and pyroptosis-associated proteins. H9c2 cells exposed to hypoxia were positively associated with IRF2 expression. The association between HIF1 and IRF2 was verified and it was shown that IRF2 expression may be regulated by the HIF-1 pathway. The present ChIP-PCR and luciferase reporter assays further demonstrated that IRF2 directly bound to the GSDMD promoter to drive GSDMD transcription for the execution of pyroptosis in hypoxia-stimulated H9c2 cells.

In conclusion, the present study demonstrated that IRF2 was key for MI and acts via increasing inflammasomes and pyroptosis. These findings confirmed that IRF2 was a key regulator of MI and provided novel insights into the mechanism of MI progression.

Acknowledgements

Not applicable.

Funding

Funding: No funding was received.

Availability of data and materials

The datasets used and analyzed during the current study are available from the corresponding author on reasonable request.

Authors' contributions

YL conceptualized and designed the study and wrote the manuscript. YL, YW and YH performed the experiments. HG and QW analyzed and interpreted the data. YL and YW confirm the authenticity of all the raw data. All authors read and approved the final version of the manuscript.

Ethics approval and consent to participate

The experimental protocol of the present study was performed in accordance with the Guide for the Care and Use of Laboratory Animals. All institutional and national guidelines for the care and use of laboratory animals were followed and the study was approved by the Ethics Committee of Cangzhou Central Hospital (approval no. CZSZ20200113).

Patient consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Glossary

Abbreviations

Abbreviations:

References