Abstract
Pyroptosis, a type of programmed necrosis associated with inflammatory, is a host defense mechanism against microbial infections. Although Chlamydia has been shown to induce pyroptosis, whether pyroptosis directly impacts the growth of Chlamydia has not been demonstrated. In this study, we found that C. trachomatis L2 infection of the mouse macrophage RAW 264.7 cells induced pyroptosis by monitoring the ultrastructural changes under transmission electron microscopy and the release of LDH and IL-1β. More importantly, this C. trachomatis-triggered pyroptosis with activation of caspase-1 and caspase-11 was also accompanied by gasdermin D (GSDMD) activation. Suppression of these two inflammatory caspases inhibited GSDMD activation. Interestingly, the C. trachomatis-triggered pyroptosis significantly inhibited the intracellular growth of C. trachomatis since inactivation of either GSDMD or caspase-1/11 significantly rescued infectious C. trachomatis yields, which suggests pyroptosis response can be utilized as an intrinsic mechanism to restrict C. trachomatis intracellular infection in addition to the well- documented extrinsic mechanisms by recruiting and enhancing inflammatory responses. This study may reveal novel targets for attenuating C. trachomatis infectivity and/or pathogenicity.
1 Introduction
Chlamydia trachomatis (C. trachomatis), an obligate intracellular Gram-negative bacterium, is a major pathogen of human sexually transmitted disease increasing public health burden (Taylor-Robinson, 2017). C. trachomatis has a unique biphasic development cycle. Initially, the infectious, extracellular elementary body (EB) infects the epithelial host cell. Intracellularly, the EB transforms to the metabolically active reticulate body (RB) for replication. The progeny RBs condense into EBs, which will be released when the host cell breaks down. At this time, macrophages recruited to sites of tissue infection can internalize C. trachomatis by phagocytosis (Morrison and Morrison, 2000). However, the intracellular fate of C. trachomatis in macrophages is still controversial. Some studies have found that C. trachomatis can survive in monocytes and macrophages for more than 7 days, which facilitates persistent C. trachomatis infection (Zuck et al., 2017; Lausen et al., 2019; Sumiyoshi et al., 2019). It has also been found that reactive arthritis caused by C. trachomatis infection in the urogenital tract is likely to be caused by the spread of monocyte-macrophages carrying active C. trachomatis through the circulatory system (Sumiyoshi et al., 2019). However, a large body of evidence indicated that macrophages can rapidly clear C. trachomatis infection to limit C. trachomatis intracellular reproduction (Stagg et al., 1998; Qiu et al., 2008; Ziklo et al., 2016). Recently, Faris et al. found that although macrophages support the intracellular growth of C. trachomatis serotype L2, they also play a role in resisting C. trachomatis infection (Faris et al., 2019). Therefore, understanding the interaction between macrophages and C. trachomatis is critical to understand C. trachomatis infectivity and pathogenicity.
Pyroptosis, a type of pro-inflammatory programmed cell death, is characterized by cell swelling and cell membrane rupture, and the release of proinflammatory cytokines. Inflammatory caspases (caspase-1/–4/–5/–11) are activated during pyroptosis (Gram et al., 2019). These active caspases cleave gasdermin-D (GSDMD), the effector of pyroptosis, at a link region between the N- and C-terminus, releasing the N-terminus fragment from the inhibitory C-terminal domain. The N-terminus of GSDMD (GSDMD-NT) binds to phosphoinositides located in the inner side of the plasma membrane and forms pores on the membrane leading to cell lysis (Sborgi et al, 2016). Inflammatory cytokine, IL-1 and IL-18 processed by caspase-1, are released during cell lysis or from the pores formed by GSDMD-NT (Shi et al., 2015).
Pyroptosis is an important type of cell death for defending against intracellular pathogen infection. GSDMD plays a key role in mediating the inhibition of Salmonella, Legionella pneumophila and Francisella infections in macrophages (Zhu et al., 2018; Gonçalves et al., 2019; Xia et al., 2019). It has been reported that C. trachomatis induces pyroptosis indicated by the releases of LDH and IL-1β via activating caspase-1 and caspase-11 in macrophages (Finethy et al., 2015; Webster et al., 2017). However, pyroptosis has not previously been demonstrated to directly impact the growth or development of Chlamydia, although inferring that pyroptosis has negative effects on Chlamydia infection. More direct experimental evidence is needed to confirm the role of pyroptosis in Chlamydia-infected macrophages. This study directly investigate the effect of pyroptosis on chlamydial replication and development and also first investigate the role of GSDMD in Chlamydia infection. We demonstrated that C. trachomatis induced GSDMD-mediated pyroptosis via activating caspase-1/11 in RAW264.7 cells, which caused cell lysis and pro-inflammatory cytokines release, and subsequent chlamydial clearance.
2 Materials and methods
2.1 Cells, bacteria, and infections
RAW264.7 cells, HeLa229 cells and iBMDM cells were purchased from the American Type Culture Collection (ATCC) and maintained in DMEM supplemented with 10% FBS. Cells were incubated at 37°C in a humidified incubator of 5% CO2, and sub-cultured every 2~3 days. C. trachomatis L2/LGV-434/Bu was also obtained from ATCC and was inoculated and propagated in HeLa cells as described previously (Zhong et al., 2001). As for infections, RAW264.7 cells and HeLa cells either grown in tissue culture dishes or plates were inoculated with chlamydial organisms as described previously (Zhong et al., 2001). For inhibitor experiments, we pretreated the cells for 30 minutes with Ac-YVAD-cmk (20 or 50μM), or Necrosulfonamide (5, 10 or 20μM) inhibitors prior to C. trachomatis L2 infection, respectively. The same concentrations of the inhibitors were maintained throughout the rest of the infection.
2.2 Antibodies and reagents
Primary antibodies against caspase-1 (ab179515), caspase-11 (ab180673), GSDMD (ab209845), GSDME (ab215191) and Biotin Goat polyclonal to Chlamydia trachomatis (ab20387) were obtained from Abcam (Cambridge, UK), Antibody for Chlamydia HSP60 (sc57840) was bought from Santa Cruz Biotechnology (California, USA), Antibodies for caspase-8 (4790), caspase-8 p18 (8592), β-Tubulin (2128) and GAPDH (5174) were obtained from Cell Signaling Technology (Danvers, MA, USA), while secondary antibodies (SA00001-15, SA00001-1) used for immunoblotting and Fluorescein (FITC)-conjugated Affinipure Rabbit Anti-Goat IgG(H+L) (SA00003-4) used for immunofluorescence staining were bought from Proteintech (Chicago, USA). IL-1β (CSB-E08054m) and IL-18 (CSB-E04609m) ELISA kits were obtained from CUSABIO (Wuhan, China). Caspase-1 inhibitor Ac-YVAD-cmk (SML0429) was purchased from Sigma (California, USA), Necrosulfonamide (AG-CR1-3705-M005) was bought from Adipogen (Epalinges, Switzerland). Caspase-11 inhibitor Wedelolactone (T3384) was obtained from Target Mol (Boston, MA). All inhibitors were dissolved in dimethyl sulfoxide (DMSO).
2.3 Immunoblot analysis
Culture supernatant was harvested to collect dead/floating cells by centrifugation at 12,000 rpm for 10 minutes at 4°C and pooled with adherent cells washing with PBS buffer three times. All cells were lysed on ice to extract protein. Equal amounts of protein lysates (40ug) were separated on SDS-PAGE gels (CWBIO, China) under reducing conditions and subsequently transferred onto nitrocellulose membranes. The caspase-1 antibody (1:1000 dilution), caspase-11 antibody (1:1000 dilution), GSDMD antibody (1:1000 dilution), GSDME antibody (1:1000 dilution), cHSP60 antibody (1:200 dilution), caspase-8 antibody (1:1000 dilution), caspase-8 p18 antibody (1:1000 dilution), β-Tubulin antibody (1:2000 dilution) and GAPDH antibody (1:2000 dilution) were incubated with polyvinylidene difluoride membranes at 4°C overnight. Then we washed the blots with PBS and incubated them with the previous described secondary antibodies. Protein bands were visualized using ECL detection regents (GE Healthcare, USA). Western blot quantification was performed by measuring band intensity with ImageJ freeware (National Institutes of Health, Bethesda, MD, USA). The quantification of cleaved caspases band was normalized first to GAPDH then to the pro-caspase band intensity. The quantification of GSDMD-NT band was normalized first to GAPDH and then to the full-length GSDMD intensity.
2.4 Cytokine analysis
RAW264.7 cells were infected with C. trachomatis L2 at a multiplicity of infection (MOI) of 5 for 12 hours. Culture supernatant was harvested by low-speed centrifugation to remove cells from the supernatant. After centrifugation the supernatant was directly used for analysis. IL-1β and IL-18 ELISA kits were used to detect the concentrations of IL-1β and IL-18 cytokines in the cell supernatant according to the manufacturer′s instructions.
2.5 Cell morphology observation
RAW264.7 cells with 70% confluence in 24-well plates were infected with C. trachomatis L2, then cultured in DMEM supplemented with 10% FBS at indicated times. Cells were visualized and photographed at a 40 X magnification using a light microscope.
2.6 Transmission electron microscopy (TEM)
RAW264.7 cells were harvested after infecting with C. trachomatis L2 at a MOI of 5 for 12 hours and were fixed by Gluta mirror fixing fluid (Solarbio, China) dehydrated with acetone, soaked and buried with pure acetone and encapsulation liquid (1:1) for 12 hours then pure encapsulation liquid for 12 hours. Samples were placed in a 37°C oven overnight, then placed in a 60°C oven for 12-24 hours for curing. Ultrathin sections were performed using an ultra-microtome (Leica Ultracut UCT, Leica, Austria). Sections were using uranium acetate and lead nitrate double staining and photographed with a HT7700 electron microscope.
2.7 siRNA transfections
The double-stranded caspase-11 small interfering RNA (siRNA) (5′CCAUUGAUCGGGCAACCUUTT3′) and double-stranded negative control siRNA were purchased from GenePharma (Suzhou, China). RAW264.7 cells were plated to 60%-70% confluence in 60-mm dishes 24 hours before transfection. 200 pmol per dish caspase-11 siRNA, or negative control siRNA was transfected using Advanced DNA RNA Transfection Reagent™ (Zeta Life, USA) following the manufacturer’s instructions. At 48 hours after transfection, the efficiency of the corresponding gene knockdown was confirmed with western blot.
2.8 Immunofluorescence microscopy analysis
To detect C. trachomatis inclusion, we infected cells with C. trachomatis L2 at a MOI of 5, and cultured cells for different times. Then the cells were fixed by 4% paraformaldehyde for 15 minutes and permeabilized with 0.1% (v/v) Triton X-100 for 5 minutes. Then we blocked the cells for 1 hour and incubated the samples with anti-Chlamydia trachomatis antibody at 4°C overnight. Fluorescein (FITC)-conjugated Affinipure Rabbit Anti-Goat IgG (H+L) antibody was used as secondary antibody. The nuclei staining was revealed with the Hoechst 33342 (Solarbio, China) solution for 5 minutes. Cells were washed with PBS solution three times for 5 minutes per-time after the primary and secondary antibody incubations. The final treated cells were observed by Zeiss LSM880 microscope and the immunoflurescence signals were processed with ZEN software.
2.9 Infectious chlamydial yields quantitation
RAW264.7 cells were infected with C. trachomatis L2 at a MOI of 5 for 40 hours under different treatment conditions. RAW264.7 cells then were lysed to collect C. trachomatis infectious progenies to re-infect a new culture of HeLa cells that had been grown to equal confluency. Reinfected HeLa cells were fixed at 24 hours post infection, immunostained and immunofluorescence microscopy quantitative analysis of inclusion number relative to nuclei in HeLa cells was used to estimate C. trachomatis infectious yields within RAW264.7 cells.
2.10 Propidium iodide (PI) staining
RAW264.7 cells were infected with C. trachomatis L2 at a MOI of 5 for 12 hours. On each specimen, we removed the media and rinsed it once with PBS buffer. PI solution (Sigma, USA) diluted into full media with the final concentration of 2 μg/ml was prepared and used to incubate the cells at 37°C for 10 minutes. Then we washed the cells once with PBS and fixed them with 4% paraformaldehyde in PBS for 30 minutes. Fluorescent images of cells were obtained with the Zeiss LSM880 microscope, and fluorescent images were deconvolved using Zen software.
2.11 LDH cytotoxicity assay
RAW264.7 cells were infected with C. trachomatis L2 at a MOI of 5 for 12 hours. LDH release in the culture medium was measured using a fully Automatic Biochemical Analyzer (Hitachi, Japan).
2.12 Statistical analysis
All experiments were performed three times independently. Data were expressed as mean ± standard deviation (SD). Statistical analysis was performed using GraphPad Prism7.0 (GraphPad Software Inc., San Diego, CA, USA). For comparison between two groups, P values were determined using two-tailed Student’s t tests. For multiple-group comparisons, one-way ANOVAs were used to test whether differences among the group means were statistically significant. P-values < 0.05 were considered statistically significant.
3 Result
3.1 C. trachomatis-induced pyroptosis is dependent on the activation of GSDMD
To determine whether pyroptosis occurs in macrophages during C. trachomatis infection, the RAW264.7 macrophages were infected with C. trachomatis at a MOI of 5 or left uninfected and multiple pyroptosis indicators were detected at 12 hours post infection. TEM images showed that, compared with uninfected group, RAW264.7 cells infected with C. trachomatis had ultrastructural changes including decreased cytoplasmic density, damaged organelles (Mitochondrial swelling and Golgi fragmentation) and fractured cell membrane, but intact nucleus (Figure 1A). Light microscopy images displayed that the infected macrophages exhibited typical swelling and characteristic large blebs from the plasma membrane (Figure 1B). Moreover, PI staining and LDH release assays were used to estimate cell membrane integrity. We observed a significant increase in PI fluorescence intensity (Figure 1C) and LDH release (Figure 1D) in the C. trachomatis-infected RAW264.7 cells compared to the uninfected cells. Immunoblot analysis detected GSDMD-NT, known as pyroptosis executor, in the RAW264.7 cells at 12 hours post infection (Figure 1E). Notably, the N-terminal fragment of cleaved GSDME (GSDME-NT), another member of the gasdermin family which can induce pyroptosis (Wang et al., 2017), was not detected (Figure 1E). Taken together, these results strongly demonstrated that C. trachomatis infection induced GSDMD-mediated pyroptosis in the infected macrophages.
Figure 1
3.2 Caspase-1 and caspase-11 are required for the activation of GSDMD induced by C. trachomatis
Caspase-1, caspase-11 or/and caspase-8 activations could regulate GSDMD-dependent pyroptosis (Gram et al., 2019). Here, we tried to explore whether GSDMD-mediated pyroptosis induced by C. trachomatis infection in macrophages was also affected by these activations. RAW264.7 cells were infected with C. trachomatis at a MOI of 5 and then cultured for different time course. We found caspase-1 was activated in a time-dependent manner in C. trachomatis-infected RAW264.7 cells (Figure 2A; Figure S1A). Furthermore, we observed that C. trachomatis also negatively regulated caspase-11 activation in a time-dependent manner within 24 hours (Figure 2A; Figure S1B). GSDMD was progressively activated with the ascending infection time and the greatest activation was observed at 12 hours post infection (Figure 2A; Figure S1C). We also found decreased expression of chlamydial heat shock protein 60 (cHSP60), the chlamydial marker protein, by prolonging infection time (Figure 2A; Figure S1D), indicating that macrophages could gradually inhibit Chlamydia replication. In addition, at 12 hours post infection, cleavage fragments of caspase-8 (p18) was not detected in the infected group compared with the uninfected group, indicating that caspse-8 was not involved in the cleavage of GSDMD (Figure 2B).These results suggested that caspase-1 and caspase-11 may play an important role in C. trachomatis clearance mediated by GSDMD activation.
Figure 2
To further evaluate the contributions of caspase-1 in GSDMD-mediated pyroptosis, RAW264.7 cells were infected with C. trachomatis at a MOI of 5, then cultured for 12 hours. We blocked the activations of caspase-1 with the specific inhibitor Ac-YVAD-cmk. Ac-YVAD-cmk treatment significantly reduced GSDMD-NT levels (Figure 2C; Figure S2A), proinflammatory cytokines IL-1β (Figure 2D) and IL-18 (Figure 2E) secretions, and LDH release (Figure 2F). These results indicated that caspase-1 could mediate GSDMD activation. To ascertain the role of caspase-11, RAW264.7 cells were transfected with control siRNA or caspase-11 siRNA and then were infected with C. trachomatis at a MOI of 5 for 12 hours. siRNA knockdown of caspase-11 strongly prevented GSDMD cleavage (Figure 2G; Figure S3D), reduced IL-1β (Figure 2H) and IL-18 (Figure 2I) secretions and LDH release (Figure 2J), which indicated that caspase-11 also mediated GSDMD activation. To our surprise, caspase-1 activation was inhibited upon caspase-11 knockdown (Figure 2G; Figure S3E). Inhibition of caspase-11 expression with a caspsae-11 inhibitor wedelolactone showed the same results (Figure S4A). Collectively, these data suggested that GSDMD-mediated pyroptosis and proinflammatory cytokines IL-1β and IL-18 release in C. trachomatis-infected macrophages could be stimulated via activating caspase-1 and caspase-11.
3.3 Blockade of GSDMD-dependent pyroptosis increases intracellular growth of C. trachomatis in macrophages
We next sought to determine the effect of GSDMD-mediated pyroptosis on chlamydia survival in macrophages. Necrosulfonamide, a potent specific inhibitor of GSDMD, which could restrain the oligomerization of GSDMD-NT and pyroptotic pore formation (Rathkey et al., 2018), was used in this study. RAW264.7 cells were infected with C. trachomatis at a MOI of 5. After Necrosulfonamide treatment, proinflammatory cytokines IL-1β (Figure 3A) and IL-18 (Figure 3B) secretions and LDH release (Figure 3C) in C. trachomatis-infected RAW264.7 cells at 12 hours post infction were decreased in a dose-dependent manner. These results indicated that Necrosulfonamide could inhibit pyroptosis in macrophages via blocking the pores formation in the cell membrane. It is worth noting that the expression levels of cHSP60 positively correlated with increased concentrations of necrosulfonamide in the RAW264.7 cells (Figure 4A). This result suggested that pyroptosis could restrict chlamydial growth in macrophages. Immunofluorescence assays were conducted at 40 hours post infection for further verification. As expected, in the presence of Necrosulfonamide, the number and the size of C. trachomatis inclusions were significantly increased in RAW264.7 cells compared to untreated group (Figures 4B, C). Infectious C. trachomatis progenies in RAW264.7 cells went up in the re-infection assay in HeLa cells (Figure 4D). Therefore, GSDMD-mediated pyroptosis is critical for limiting C. trachomatis growth in macrophages.
Figure 3
Figure 4
In summary, we proposed that GSDMD-mediated pyroptosis could be a defensive mechanism against C. trachomatis infection in macrophages through cleaving executor GSDMD to GSDMD-NT with pore-forming activity. The latter formed pyroptotic pores in cell membrane, consequently led to cell lytic death and proinflammatory cytokines secretion.
3.4 Pyroptosis mediated by Caspase-1 and -11-activated GSDMD is able to inhibit the intracellular growth of C. trachomatis
Finally, we suppressed the activation of upstream molecules caspase-1 and caspase-11 to further study the role of pyroptosis. RAW264.7 cells were infected with C. trachomatis at a MOI of 5 for 12 and 40 hours. With Ac-YVAD-cmk treatment, RAW264.7 cells presented an increased C. trachomatis loads (Figure 5A) and inclusion numbers (Figures 5E, F). Similarly, there were rising C. trachomatis loads (Figure 5C) and the inclusion numbers (Figures 5E, G) upon caspase-11 knockdown. We also verified the requirements of caspase-1 and caspase-11 activations in RAW264.7 cells for restricting infectious C. trachomatis progeny production by reinfection assay. C. trachomatis infected-RAW264.7 cells were lysed at 40 hours post infection and then the infectious C. trachomatis progenies within cells were harvested and used to re-infect HeLa cells. With Ac-YVAD-cmk treatment or upon caspase-11 knockdown, there was an obvious increase of infectious C. trachomatis yields in RAW264.7 cells as supported by the increasing inclusion numbers in the HeLa cells (Figures 5H, I). Thus, these results indicated that both caspase-1 or caspase-11 contributed to restraining chlamydial growth in macrophages. Notably, GSDMD-NT levels decreased when RAW264.7 cells were treated with Ac-YVAD-cmk treatment or transfected by caspase-11 siRNA, while cHSP60 expression levels increased with the progressive inhibition of GSDMD (Figures 5A–D). Therefore, inactivation of caspase-1 or caspase-11 inhibited GSDMD-mediated pyroptosis, which promoted the survival of C. trachomatis. In conclusion, these data suggested that pyroptosis mediated by caspase-1 and -11-activated GSDMD is able to inhibit the intracellular growth of C. trachomatis.
Figure 5
4 Discussion
In this study, we characterized the role of GSDMD-mediated pyroptosis during C. trachomatis infection in macrophages. Firstly, we clearly demonstrated that the pyroptosis occurred in macrophages with C. trachomatis infection. Additionally, evidence was provided showing that caspase-1 and caspase-11 activation were required for GSDMD-mediated pyroptosis. Specifically, our study revealed that caspase-1/11-GSDMD-mediated pyroptosis may lead to cell lytic death and proinflammatory cytokines secretion, which restrained C. trachomatis growth in macrophages.
Our study found that inhibition of C. trachomatis growth was dependent on GSDMD-NT pore-forming activity. GSDMD-NT can form extensive pores on phosphoinositide- or cardiolipin-containing liposomes or on liposomes made of natural polar lipid mixtures (Shi et al., 2017), some essential constituents of chlamydial inclusion membrane (Yao et al., 2015). Thus, GSDMD-NT may exhibit strong membrane pore-forming activity on both the cell plasma membrane and chlamydial inclusion membrane. In fact, GSDMD-NT can form pores not only in the plasma membrane, but also in bacterial membranes (Jorgensen et al., 2016), mitochondrial membranes (Estfanous et al., 2021) and phagosomal membranes (Estfanous et al., 2021). Hence, apart from forming pores in the cell membrane, we speculate that GSDMD-NT may also form pores in inclusion membrane directly, resulting in destruction of chlamydial reproductive niche and contributing to C. trachomatis clearance although this hypothesis requires more experimental evidence to confirm.
GSDMD-mediated infection clearance was demonstrated in several intracellular bacteria. Pyroptotic cell death deprives intracellular pathogens from their replicative niches as a cell-intrinsic mechanism to control infection (Jorgensen and Miao, 2015). Chlamydiae are obligately intracellular pathogens, it has been extensively documented the premature death of C. trachomatis-infected cells disrupts the ability of the bacteria to form infectious EBs. Hence, we focus on whether pyroptosis can lead to cell-intrinsic inhibition of C. trachomatis. We observed C. trachomatis infection induced-pyroptosis occurred most strongly at early infection as the greatest activation of GSDMD-NT was observed at 12 hours post infection (Figure 2A). In this period, EB differentiates into RB and the rupture of pyroptotic cells deprives the replicative niche required for RBs. As a result, RB replication is diminished, disallowing the RBs to differentiate back into the infectious EBs. The combined outcome of these effects is cell-intrinsic inhibition of C. trachomatis. This is consistent with previous studies showing that C. trachomatis-infected mouse macrophages undergo pyroptosis early in infection (Finethy et al., 2015; Webster et al., 2017).
Caspase-11 directly acts as a receptor of cytosolic bacterial lipopolysaccharide (LPS) and is activated by binding to LPS (Shi et al., 2014). Our results showed that C. trachomatis organisms activated caspase-11 in macrophages. Paradoxically, a recent study has shown that C. trachomatis LPS could not activate caspase-11, as shown by the lack of GSDMD activation in murine bone marrow-derived macrophages (BMDMs) transfected with Chlamydia LPS (Yang et al., 2019). But several studies found that Chlamydia infection did induce caspase-11 activation (Finethy et al., 2015; Webster et al., 2017). This may be caused by differences in the ability of Chlamydia LPS and C. trachomatis organism activating caspase-11. Webster et al. have reported that caspase-11 expression was markedly reduced in BMDMs stimulated with irradiated C. trachomatis, suggesting that caspase-11 expression requires additional, essential signals provided by C. trachomatis replication and/or metabolism intracellularly. NF-κB activation is essential for caspase-11 expression in response to LPS (Schauvliege et al., 2002).Whereas transfection of Chlamydia LPS into macrophages did not activate NF-κB (Yang et al., 2019). Our experiments indicated that C. trachomatis organisms can activate NF-κB (data not shown). Thus, the fact that C. trachomatis organisms are capable of activating caspase-11 in macrophages is not contradictory. However, the exact mechanisms of caspase-11 activation remain to be elucidated.
C. trachomatis infection results in caspase-1 activation via activation of NLRP3 and AIM2 inflammasome. NLRC4 and NLRP1, which activate caspase-1 without ASC, were not activated based on evidence in the literature using BMDMs (Finethy et al., 2015). We found that C. trachomatis infection activated caspase-1 using immortalized mouse bone marrow-derived macrophages (iBMDMs) expressing ASC protein (Figure S5A), which was consist with previous study (Finethy et al., 2015). Surprisingly, caspase-1 was activated in RAW264.7 cells deficient in ASC acquired for NLRP3 and AIM2 in this study. This observation appeared to be inconsistent with previous research. A possible explanation for this apparent contradiction is that there may be a caspase-1 activation pathway independent of NLRP3, AIM2, NLRC4, and NLRP1 activation in RAW264.7 cells infected with C. trachomatis, which is supported by the two studies. One study reported that caspase-1 was activated treated with nigerin, a NLRP3 classic activator, in RAW26.7 cells, suggesting the existence of a NLRP3 inflammasome-independent caspase-1 activation pathway (Armstrong et al., 2019). Another study also demonstrated that caspase-1 was activated through an inflammasome-independent pathway in RAW264.7 cell model (Chuang et al., 2020). Therefore, C. trachomatis is likely to activate caspase-1 through an inflammasome- independent pathway in RAW264.7 cells. The underlying mechanism for regulating caspase-1 activation will be a challenging but interesting future research direction.
We have noticed that caspase-11 knockdown had a strong protection from cell death (Figures 2H–J) and promoted Chlamydia survival (Figures 5C, E, G) since caspase-11 knockdown significantly inhibited pyroptosis. Caspase-11 knockdown not only inhibited GSDMD activation, but also inhibited caspase-1 activation unexpectedly (Figure 2G). It is well-established in the literature that caspase-11 activation leads to non-canonical NLRP3 inflammasome assembly and caspase-1 activation (Kayagaki et al., 2011). By surprise, caspase-11 knockdown inhibited caspase-1 activation significantly in NLRP3 inflammasome-deficient Raw264.7 cells (Figure 2G). How caspase-11 regulates a NLRP3 inflammasome-independent caspase-1 activation pathway needs further exploration. Moreover, caspase-11 inhibitor wedelolacetone treatment produced the same effect as caspase-11 siRNA transfection shown in Figure 2G. Despite being widely available, wedelolacetone inhibits caspase-11 expression indirectly. Wedelolactone has been reported to inhibit caspase-11 expression by inhibiting the NF-κB pathway since caspase-11 gene expression in response to LPS requires NF-κB activation (Schauvliege et al., 2002; Kobori et al., 2004). Although the possibilities of NF-κB signaling inhibition suppressing pyroptosis cannot be ruled out, wedelolacetone treatment inhibited caspase-11 expression and blocked its activation (Figure S4A) and these results are consistent with results from caspase-11 knockdown (Figure 2G), which indicated that these observed phenotypes may be at least partially attributable to the inhibitory effect of wedelolacetone on caspase-11 expression. In addition, our result showed that necrosulfonamide treatment largely prevented GSDMD-NT pore formation (Figure 3). The off-target effects of necrosulfonamide in this study were less likely. Because necrosulfonamide, a known inhibitor of MLKL, has no effect on necrosis in murine cells (Sun et al., 2012).
Some researchers believed that macrophages are permissive for C. trachomatis growth. However, the growth in macrophages is severely limited compared to that observed in epithelial cells (Beagley et al., 2009). Macrophages could restrict intracellular growth of C. trachomatis through distinct mechanisms including lysosomal degradation (Kuo et al., 2002; Kinchen and Ravichandran, 2008; Yasir et al., 2011), autophagy (Al-Zeer et al., 2009; Al-Zeer et al., 2013) and nutrient starvation (Heuer et al., 2009; Soliman et al., 2010; Luo et al., 2019). Previous research has inferred that pyroptosis is detrimental to Chlamydia infection. By inhibiting GSDMD-mediated pyroptosis, we found that the infectious yield of C. trachomatis are increased in RAW264.7 cells (Figure 4D). Thus, our study further supported the idea that pyroptosis is indeed a host defense mechanism against Chlamydia infection and may help explain why the macrophage environment is hostile to chlamydial growth.
In summary, we presented here a model of intracellular chlamydial growth inhibition in macrophages (Figure 6). Caspase-1 and caspase-11 are activated in C. trachomatis-infected macrophages to cleave GSDMD into GSDMD-NT, causing pyroptotic cell lysis and IL-1β and IL-18 secretions, which limited C. trachomatis growth. The C. trachomatis-mouse macrophage interaction model may be used to further investigate how C. trachomatis triggers caspase-1/11 activation and how C. trachomatis is inhibited in the pyroptotic cells. This study is helpful to understand the pathophysiological process of Chlamydia infection and reveals novel targets for treating C. trachomatis infection.
Figure 6
Statements
Data availability statement
The raw data supporting the conclusions of this article will be made available by the authors, without undue reservation.
Author contributions
PJ, HC, NZ, JC, and LT designed the experiments. PJ, HC, XF, MJ, DX, HT, and LZ performed the experiments. PJ, XF, and HX analyzed data and wrote the manuscript. HX, NZ and LT revised the manuscript. All authors contributed to the article and approved the submitted version.
Funding
This study was supported by Natural Science Foundation of Changsha City (grant number kq2202415) and Natural Science Foundation of Hunan Province (grant number 2018JJ2559).
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Supplementary material
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fcimb.2023.1116335/full#supplementary-material
References
1
Al-ZeerM. A.Al-YounesH. M.BraunP. R.ZerrahnJ.MeyerT. F. (2009). IFN-gamma-inducible Irga6 mediates host resistance against chlamydia trachomatis via autophagy. PloS One4, e4588. doi: 10.1371/journal.pone.0004588
2
Al-ZeerM. A.Al-YounesH. M.LausterD.Abu LubadM.MeyerT. F. (2013). Autophagy restricts chlamydia trachomatis growth in human macrophages via IFNG-inducible guanylate binding proteins. Autophagy9, 50–62. doi: 10.4161/auto.22482
3
ArmstrongH.Bording-JorgensenM.ChanR.WineE. (2019). Nigericin promotes NLRP3-independent bacterial killing in macrophages. Front. Immunol.10. doi: 10.3389/fimmu.2019.02296
4
BeagleyK. W.HustonW. M.HansbroP. M.TimmsP. (2009). Chlamydial infection of immune cells: Altered function and implications for disease. Crit. Rev. Immunol.29, 275–305. doi: 10.1615/critrevimmunol.v29.i4.10
5
ChuangJ. P.KaoC. Y.LeeJ. C.LingP.MaaM. C.LeuT. H. (2020). EPS8 regulates an NLRP3 inflammasome-independent caspase-1 activation pathway in monosodium urate crystal-treated RAW264.7 macrophages. Biochem. Biophys. Res. Commun.530, 487–493. doi: 10.1016/j.bbrc.2020.05.084
6
EstfanousS.KrauseK.AnneM. N. K.EltobgyM.CautionK.Abu KhweekA.et al. (2021). Gasdermin d restricts burkholderia cenocepacia infection in vitro and in vivo. Sci. Rep.11, 855. doi: 10.1038/s41598-020-79201-5
7
FarisR.AndersenS. E.McCulloughA.GourroncF.KlingelhutzA. J.WeberM. M. (2019). Chlamydia trachomatis serovars drive differential production of proinflammatory cytokines and chemokines depending on the type of cell infected. Front. Cell Infect. Microbiol.9. doi: 10.3389/fcimb.2019.00399
8
FinethyR.JorgensenI.HaldarA. K.de ZoeteM. R.StrowigT.FlavellR. A.et al. (2015). Guanylate binding proteins enable rapid activation of canonical and noncanonical inflammasomes in chlamydia-infected macrophages. Infect. Immun.83, 4740–4749. doi: 10.1128/IAI.00856-15
9
GonçalvesA. V.MargolisS. R.QuirinoG. F. S.MascarenhasD. P. A.RauchI.NicholsR. D.et al. (2019). Gasdermin-d and caspase-7 are the key caspase-1/8 substrates downstream of the NAIP5/NLRC4 inflammasome required for restriction of legionella pneumophila. PloS Pathog.15, e1007886. doi: 10.1371/journal.ppat.1007886
10
GramA. M.BootyL. M.BryantC. E. (2019). Chopping GSDMD: caspase-8 has joined the team of pyroptosis-mediating caspases. EMBO J.38, e102065. doi: 10.15252/embj.2019102065
11
HeuerD.Rejman LipinskiA.MachuyN.KarlasA.WehrensA.SiedlerF.et al. (2009). Chlamydia causes fragmentation of the golgi compartment to ensure reproduction. Nature457, 731–735. doi: 10.1038/nature07578
12
JorgensenI.MiaoE. A. (2015). Pyroptotic cell death defends against intracellular pathogens. Immunol. Rev.265, 130–142. doi: 10.1111/imr.12287
13
JorgensenI.ZhangY.KrantzB. A.MiaoE. A. (2016). Pyroptosis triggers pore-induced intracellular traps (PITs) that capture bacteria and lead to their clearance by efferocytosis. J. Exp. Med.213, 2113–2128. doi: 10.1084/jem.20151613
14
KayagakiN.WarmingS.LamkanfiM.Vande WalleL.LouieS.DongJ.et al. (2011). Non-canonical inflammasome activation targets caspase-11. Nature479, 117–121. doi: 10.1038/nature10558
15
KinchenJ. M.RavichandranK. S. (2008). Phagosome maturation: going through the acid test. Nat. Rev. Mol. Cell Biol.9, 781–795. doi: 10.1038/nrm2515
16
KoboriM.YangZ.GongD.HeissmeyerV.ZhuH.JungY. K.et al. (2004). Wedelolactone suppresses LPS-induced caspase-11 expression by directly inhibiting the IKK complex. Cell Death Differ.11, 123–130. doi: 10.1038/sj.cdd.4401325
17
KuoC. C.PuolakkainenM.LinT. M.WitteM.CampbellL. A. (2002). Mannose-receptor positive and negative mouse macrophages differ in their susceptibility to infection by chlamydia species. Microb. Pathog.32, 43–48. doi: 10.1006/mpat.2001.0479
18
LausenM.ChristiansenG.Bouet Guldbæk PoulsenT.BirkelundS. (2019). Immunobiology of monocytes and macrophages during chlamydia trachomatis infection. Microbes Infect.21, 73–84. doi: 10.1016/j.micinf.2018.10.007
19
LuoZ.NevilleS. L.CampbellR.MoreyJ. R.MenonS.ThomasM.et al. (2019). Structure and metal binding properties of Chlamydia trachomatis YtgA. J. Bacteriol.202, e00580-19. doi: 10.1128/JB.00580-19
20
MorrisonS. G.MorrisonR. P. (2000). In situ analysis of the evolution of the primary immune response in murine chlamydia trachomatis genital tract infection. Infect. Immun.68, 2870–2879. doi: 10.1128/IAI.68.5.2870-2879.2000
21
QiuH.FanY.JoyeeA. G.WangS.HanX.BaiH. (2008). Type I IFNs enhance susceptibility to chlamydia muridarum lung infection by enhancing apoptosis of local macrophages. J. Immunol.181, 2092–2102. doi: 10.4049/jimmunol.181.3.2092
22
RathkeyJ. K.ZhaoJ.LiuZ.ChenY.YangJ.KondolfH. C.et al. (2018). Chemical disruption of the pyroptotic pore-forming protein gasdermin d inhibits inflammatory cell death and sepsis. Sci. Immunol.3, eaat2738. doi: 10.1126/sciimmunol.aat2738
23
SborgiL.RühlS.MulvihillE.PipercevicJ.HeiligR.StahlbergH.et al. (2016). GSDMD membrane pore formation constitutes the mechanism of pyroptotic cell death. EMBO J.35, 1766–1778. doi: 10.15252/embj.201694696
24
SchauvliegeR.VanrobaeysJ.SchotteP.BeyaertR. (2002). Caspase-11 gene expression in response to lipopolysaccharide and interferon-gamma requires nuclear factor-kappa b and signal transducer and activator of transcription (STAT) 1. J. Biol. Chem.277, 41624–41630. doi: 10.1074/jbc.M207852200
25
ShiJ.GaoW.ShaoF. (2017). Pyroptosis: Gasdermin-mediated programmed necrotic cell death. Trends Biochem. Sci.42, 245–254. doi: 10.1016/j.tibs.2016.10.004
26
ShiJ.ZhaoY.WangY.GaoW.DingJ.LiP.et al. (2014). Inflammatory caspases are innate immune receptors for intracellular LPS. Nature514, 187–192. doi: 10.1038/nature13683
27
ShiJ.ZhaoY.WangK.ShiX.WangY.HuangH.et al. (2015). Cleavage of GSDMD by inflammatory caspases determines pyroptotic cell death. Nature526, 660–665. doi: 10.1038/nature15514
28
SolimanH.Mediavilla-VarelaM.AntoniaS. (2010). Indoleamine 2,3-dioxygenase: is it an immune suppressor? Cancer J.16, 354–359. doi: 10.1097/PPO.0b013e3181eb3343
29
StaggA. J.TuffreyM.WoodsC.WunderinkE.KnightS. C. (1998). Protection against ascending infection of the genital tract by chlamydia trachomatis is associated with recruitment of major histocompatibility complex class II antigen-presenting cells into uterine tissue. Infect. Immun.66, 3535–3544. doi: 10.1128/IAI.66.8.3535-3544.1998
30
SumiyoshiR.KogaT.TsujiS.EndoY.TakataniA.ShimizuT.et al. (2019). Chlamydia-induced reactive arthritis diagnosed during gout flares: A case report and cumulative effect of inflammatory cytokines on chronic arthritis. Med. (Baltimore).98, e17233. doi: 10.1097/MD.0000000000017233
31
SunL.WangH.WangZ.HeS.ChenS.LiaoD.et al. (2012). Mixed lineage kinase domain-like protein mediates necrosis signaling downstream of RIP3 kinase. Cell148, 213–227. doi: 10.1016/j.cell.2011.11.031
32
Taylor-RobinsonD. (2017). The discovery of chlamydia trachomatis. Sex Transm Infect.93, 10. doi: 10.1136/sextrans-2016-053011
33
WangY.GaoW.ShiX.DingJ.LiuW.HeH.et al. (2017). Chemotherapy drugs induce pyroptosis through caspase-3 cleavage of a gasdermin. Nature547, 99–103. doi: 10.1038/nature22393
34
WebsterS. J.BrodeS.EllisL.FitzmauriceT. J.ElderM. J.GekaraN. O.et al. (2017). Detection of a microbial metabolite by STING regulates inflammasome activation in response to chlamydia trachomatis infection. PloS Pathog.13, e1006383. doi: 10.1371/journal.ppat.1006383
35
XiaX.WangX.ZhengY.JiangJ.HuJ. (2019). What role does pyroptosis play in microbial infection? J. Cell Physiol.234, 7885–7892. doi: 10.1002/jcp.27909
36
YangC.BrionesM.ChiouJ.LeiL.PattonM. J.MaL.et al. (2019). Chlamydia trachomatis lipopolysaccharide evades the canonical and noncanonical inflammatory pathways to subvert innate immunity. mBio10, e00595–e00519. doi: 10.1128/mBio.00595-19
37
YaoJ.DodsonV. J.FrankM. W.RockC. O. (2015). Chlamydia trachomatis scavenges host fatty acids for phospholipid synthesis via an acyl-acyl carrier protein synthetase. J. Biol. Chem.290, 22163–22173. doi: 10.1074/jbc.M115.671008
38
YasirM.PachikaraN. D.BaoX.PanZ.FanH. (2011). Regulation of chlamydial infection by host autophagy and vacuolar ATPase-bearing organelles. Infect. Immun.79, 4019–4028. doi: 10.1128/IAI.05308-11
39
ZhongG.FanP.JiH.DongF.HuangY. (2001). Identification of a chlamydial protease-like activity factor responsible for the degradation of host transcription factors. J. Exp. Med.193, 935–942. doi: 10.1084/jem.193.8.935
40
ZhuQ.ZhengM.BalakrishnanA.KarkiR.KannegantiT. D. (2018). Gasdermin d promotes AIM2 inflammasome activation and is required for host protection against Francisella novicida. J. Immunol.201, 3662–3668. doi: 10.4049/jimmunol.1800788
41
ZikloN.HustonW. M.HockingJ. S.TimmsP. (2016). Chlamydia trachomatis genital tract infections: When host immune response and the microbiome collide. Trends Microbiol.24, 750–765. doi: 10.1016/j.tim.2016.05.007
42
ZuckM.EllisT.VenidaA.HybiskeK. (2017). Extrusions are phagocytosed and promote chlamydia survival within macrophages. Cell Microbiol.19, e12683. doi: 10.1111/cmi.12683
Summary
Keywords
Chlamydia trachomatis, GSDMD, pyroptosis, macrophage, caspase-1, caspase-11
Citation
Jiang P, Chen H, Feng X, Xie H, Jiang M, Xu D, Tang H, Zhang N, Chen J, Zhang L and Tang L (2023) GSDMD-mediated pyroptosis restrains intracellular Chlamydia trachomatis growth in macrophages. Front. Cell. Infect. Microbiol. 13:1116335. doi: 10.3389/fcimb.2023.1116335
Received
05 December 2022
Accepted
03 March 2023
Published
16 March 2023
Volume
13 - 2023
Edited by
Andres Vazquez-Torres, University of Colorado Denver, United States
Reviewed by
Jon Audia, University of South Alabama, United States; Heping Zheng, Southern Medical University, China; Chunxue Lu, University of South China, China
Updates
Copyright
© 2023 Jiang, Chen, Feng, Xie, Jiang, Xu, Tang, Zhang, Chen, Zhang and Tang.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Lingli Tang, linglitang@csu.edu.cn
This article was submitted to Bacteria and Host, a section of the journal Frontiers in Cellular and Infection Microbiology
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