In response to infection, polymorphonuclear neutrophils (PMN) are recruited in the infectious sites, and employ three major strategies to fight against the microbes including phagocytosis, degranulation, and neutrophil extracellular traps (NETs). NETs are a meshwork of chromatin fibers mixed with granule-derived antimicrobial peptides and enzymes, which trap and kill the bacteria extracellularly. In this study, by using a mouse sepsis model, we identified a novel mechanism by which NETs induce macrophage (Mϕ) pyroptosis, a caspase-1-dependent regulated cell death. We show that NET-derived HMGB1, acting through RAGE and dynamin-dependent signaling, triggers an intra-Mϕ cascade of molecular events including cathepsin B (CatB) release from the ruptured lysosomes, followed by pyroptosome formation and caspase-1 activation, and subsequent Mϕ pyroptosis. The study further demonstrates that Mϕ pyroptosis augments inflammatory responses following sepsis. These findings shed light on the proinflammatory role of NETs in mediating PMN–Mϕ interaction, which therefore influences the progress of inflammation following infection.
Sepsis, a leading cause of human death worldwide, is characterized by excessive inflammation in response to infection1. During septic peritonitis, polymorphonuclear neutrophils (PMN) and monocytes are recruited in the peritoneal cavity, and the latter differentiate into inflammatory macrophages (Mϕ)2. The interaction between PMN and Mϕ has been suggested as an important factor that regulates inflammation following trauma, hemorrhagic shock, and endotoxemia, as well as other pathological conditions3,4,5,6,7. For instance, we have reported that exosomes released from the hemorrhagic shock-activated alveolar Mϕ promote PMN necroptosis in the lungs5. Others have demonstrated that neutrophil extracellular traps (NETs) acting through inducing cytokine production from Mϕ promote inflammation and the development of atherosclerosis7. However, in sepsis, the role of the interaction between PMN and Mϕ in the development of inflammation and the underlying mechanism remains unclear.
In response to microbial infection, one of the defensing mechanisms of the host is to release nuclear contents of the PMN into the extracellular space to trap and kill the microbes, known as NETs. Since first discovered in 20048, NETs have been recognized as an important strategy of the host immune system to respond against infections9. NETs are composed of decondensed chromatin decorated with granular and cytoplasmic proteins, which may serve as danger-associated molecular patterns (DAMPs) playing critical role in the progression of host inflammation10,11.
High-mobility group box 1 (HMGB1), a highly conserved nuclear protein widely present in the nucleus and cytoplasm of nearly all cell types, is the prototypic DAMP molecule when released into the extracellular space12. Our previous studies reported that HMGB1 plays a critical role in inducing pyroptosis of Mϕ and vascular endothelial cell (EC)13,14. Pyroptosis is a caspase-1-dependent form of regulated cell death, which is usually triggered by various pathological stimuli, i.e., intracellular pathogens and extracytoplasmic stimuli15. The characteristics of pyroptosis include cell swelling, rapid plasma membrane rupture, and release of proinflammatory contents16. Pyroptotic cell-released danger signals or DAMP molecules enhance inflammatory responses17.
In this study, we identified a novel mechanism of PMN–Mϕ interaction in sepsis. We demonstrate in the mouse cecal ligation and puncture (CLP) sepsis model that PMN through ejecting NETs induce peritoneal Mϕ pyroptosis. We further confirm that HMGB1 released from NETs acting through the receptor for advanced glycation end products (RAGE) initiates dynamin-dependent signaling pathway that includes cathepsin B (CatB) activation, pyroptosome formation, and caspase-1 activation, which in turn leads to Mϕ pyroptosis. These findings suggest a previously unidentified pathway of PMN–Mϕ cross-talk, which causes enhanced Mϕ death and subsequent exaggerated post-sepsis inflammation.
Sepsis induces peritoneal Mϕ pyroptosis
In CLP-induced sepsis, we found that a considerable part of the peritoneal Mϕ (PMϕ) underwent cell death. As shown in Fig. 1, mice subjected to CLP exhibited a gradual increase in PMϕ death. The PMϕ death, as defined as double staining of Annexing V and 7-AAD, reached a peak (~36%) at 18 h after CLP. In order to determine the type of PMϕ death, PMϕ collected from the peritoneal lavage fluid (PLF) were further detected for nuclear fragmentation, caspase-1 activation, and the characteristics of pyroptosis, by staining the cells with TMR-Cell Death Reagent and Alexa Flour 488-labeled caspase-1 FLICA, and measured by flow cytometry. We observed ~14% pyroptotic PMϕ at 18 h after CLP (Fig. 1b). These results suggest that pyroptosis is responsible for ~39% of the PMϕ death following sepsis.
Interestingly, we further observed NET formation in PLF, associated with the exhibition of PMϕ pyroptosis following CLP. PLF samples were collected from mice that were subjected to either CLP or sham operation for 0 to 24 h, and each of the PLF samples was divided into two aliquots for florescence microscopy of NETs and PMϕ pyroptosis, respectively. Using SYTOX green staining of DNA and florescence microscopy, we detected in PLF a progressive increase in NET formation, which started at as early as 3 h and reached a peak at 6 h after CLP, and remained at a high level for at least 24 h (Fig. 1c, e). Associated with the formation of NETs, PMϕ pyroptosis occurrence starts at 12 h after CLP (Fig. 1d). Intraperitoneal injection (i.p.) of Cl-Amidine (Cl-Ad, 50 mg/kg B.W.), an inhibitor of NET formation by suppressing peptidylarginine deiminase 4 (PAD4)18,19, at 30 min prior to CLP prevented NET formation following sepsis (Fig. 1e). Notably, the suppression of NET formation was associated with the decrease in PMϕ pyroptosis at 18 h after CLP (Fig. 1f). These results led us to determine the causal role of NETs in PMϕ pyroptosis.
NETs induce PMϕ pyroptosis
To investigate a direct role of NETs in regulating Mϕ death, we collected peritoneal PMN, which were recruited into the peritoneal cavity in response to i.p. injection of 9% casein, and stimulated the PMN in vitro with PMA (50 nM) for 2 h to induce NETs20. The NET formation was confirmed by SYTOX green and histone double staining, and florescence microscopy, as shown in Fig. 2a. The induced NETs in the culture medium supernatant were then co-cultured with normal bone marrow-derived macrophages (BMDM) for up to 24 h, followed by the detection of BMDM pyroptosis. As shown in Fig. 2b, NETs induced BMDM pyroptosis, which reached a peak at 12 h after the co-culture; however, the medium supernatant from unstimulated PMN did not cause BMDM pyroptosis.
These results suggest that NET formation in the peritoneal cavity following sepsis is responsible for PMϕ pyroptosis.
NET-derived HMGB1 induces PMϕ pyroptosis
Our previous studies showed that HMGB1 can induce cell pyroptosis13,14, which led us to hypothesize that HMGB1 released from the NETs might serve as a critical mediator to induce PMϕ pyroptosis, as considering that NETs consist of decondensed chromatin, and HMGB1 is one of the chromatin proteins. We first determined whether the NET component includes HMGB1. Peritoneal PMN were isolated and stimulated with PMA (50 nM) for up to 4 h to induce NET formation in the presence and absence of NET inhibitor Cl-Ad (200 μM)21, and then HMGB1 in the PMN medium supernatant was measured by western blotting. As shown in Fig. 3a, b, at 2 h after PMA stimulation, with NET formation, HMGB1 started to increase in the supernatant; however, the NET inhibitor Cl-Ad prevented HMGB1 increase in the supernatant. These in vitro observations were recapitulated in vivo. HMGB1 level in PLF was significantly elevated at 6 h after CLP, and maintained at a high level for at least 24 h (Fig. 3c). This elevation in the HMGB1 level was suppressed by a pre-treatment with i.p. injection of NET inhibitor Cl-Ad (Fig. 3d). These results suggest that NET formation associates with HMGB1 release.
To determine whether the NET-derived HMGB1 induces PMϕ pyroptosis, we subjected wild-type (WT) and HMGB1−/− mice to CLP for 18 h, and then measured PMϕ pyroptosis. HMGB1 deficiency significantly decreased the PMϕ pyroptosis, as compared to that in the WT mice (Fig. 3e), although NET formation in the CLP groups was not affected by HMGB1 deficiency (Fig. 3f). To specifically define the role of the NET-derived HMGB1 in inducing Mϕ pyroptosis, we induced NETs in WT and HMGB1−/− PMN in vitro and co-cultured the NETs with WT normal BMDM for 12 h. As shown in Fig. 3g, HMGB1 deficiency significantly attenuates the NET-induced BMDM pyroptosis, as compared to the group treated with WT NETs. These results demonstrate an important role of NET-released HMGB1 in inducing Mϕ pyroptosis.
RAGE–dynamin signaling mediates NET-induced PMϕ pyroptosis
To determine whether NET-induced Mϕ pyroptosis following sepsis is a specific receptor-dependent event, we isolated BMDM from WT, RAGE−/−, TLR4−/−, and TLR9−/− mice, and then treated the cells with NETs (or the medium supernatant of the unstimulated PMN as a control) for 12 h. The results showed that RAGE deficiency effectively prevented Mϕ pyroptosis induced by NETs, whereas the genetic deletion of TLR4 or TLR9 failed to block Mϕ pyroptosis (Fig. 4a). We further subjected RAGE−/− mice to CLP and observed that RAGE deficiency significantly prevented PMϕ pyroptosis at 18 h after CLP, as compared to that in the WT mice (Fig. 4b), although there was no significant change in NET formation between these two groups (Fig. 4c).
Our previous in vitro study has shown that RAGE–dynamin signaling mediates HMGB1-induced Mϕ pyroptosis13. However, this mechanism has yet to be determined in an in vivo sepsis model. To elucidate the role of RAGE–dynamin signaling in NET-induced PMϕ pyroptosis, we applied dynamin inhibitor dynasore (30 µg/ml) in the NET-BMDM co-culture system, and found that dynasore exhibited a suppressive effect on the NET-induced BMDM pyroptosis (Fig. 4d). Collectively, these results show that NET-derived HMGB1 mediates Mϕ pyroptosis via a RAGE–dynamin pathway.
Lysosome destabilization and cathepsin B activation are required for pyroptosome formation and PMϕ pyroptosis
It has been reported that pyroptosome, a complex including adaptor protein apoptosis-associated speck-like protein containing a CARD (ASC), also known as ASC focus, recruits pro-caspase-1, resulting in its activation and proteolysis of the mature form via neighboring activated caspase-1 proteins22. Our previous study showed that pyroptosome, rather than inflammasome, mediates HMGB1-induced Mϕ pyroptosis via lysosome enzyme cathepsin B (CatB)-dependent pathway13. To determine whether CatB pathway contributes to NET-induced Mϕ pyroptosis, we treated WT BMDM with NETs that were induced from WT or HMGB1−/− PMN in the presence or absence of dynasore (30 µg/ml) for 9 h, followed by measuring the lysosome integrity and CatB activation in the BMDM using fluorescence-tagged DQ ovalbumin and Magic Red CatB detection reagent, respectively. The WT NETs induced lysosome rupture and CatB activation in WT Mϕ, while dynasore effectively blocked these effects (Fig. 5a, b). HMGB1−/− NETs did not induce the lysosome destabilization, and CatB activation, as shown in Fig. 5a, b. In addition, WT NETs failed to induce lysosome rupture and CatB activation in RAGE deficiency Mϕ (Fig. 5a, b). Furthermore, we subjected the WT, HMGB1−/−, and RAGE−/− mice to CLP for 12 h, and detected lysosome destabilization and CatB activation in PMϕ. As shown in Fig. 5c, d, CLP caused the lysosome rupture and CatB activation in the PMϕ from WT mice, but not in the PMϕ from the HMGB1−/− and RAGE−/− mice.
To determine whether pyroptosome formation is implicated in the Mϕ pyroptosis induced by NET-derived HMGB1, we stimulated WT BMDM with WT NETs or HMGB1−/− NETs in the presence or absence of CatB inhibitor CA-074-me (10 μM)13, followed by visualizing the ASC focus using florescence-tagged ASC antibody and confocal microscopy, and detecting caspase-1 activation by western blotting. Figure. 5e, f shows that WT NETs induced ASC foci formation and caspase-1 activation, whereas CatB inhibitor prevented these effects of WT NETs; HMGB1−/− NETs failed to induce ASC foci formation and caspase-1 activation. Taken together, these results suggest that NET-derived HMGB1 mediates Mϕ pyroptosis through RAGE–CatB–ASC–Caspase1 signaling pathway.
NET-induced Mϕ pyroptosis enhances inflammatory responses
We have previously reported that pyroptotic EC increased the inflammatory cytokine expression in non-pyroptotic cells, suggesting a proinflammatory effect of the pyroptotic cells14. To determine the role of Mϕ pyroptosis in acute inflammatory response, WT, RAGE−/−, and caspase1−/− mice were subjected to CLP for 18 h with or without i.p of NET inhibitor Cl-Ad (50 mg/kg B.W.), and then tumor necrosis factor-α (TNF-α) and the interleukin-1β (IL-1β) concentrations in PLF were measured by enzyme-linked immunosorbent assay (ELISA). As shown in Fig. 6a, b, TNF-α and IL-1β levels significantly increased in the PLF collected from WT mice following CLP, whereas the genetic deletion of either RAGE or caspase-1 markedly decreased the cytokines release in response to CLP. Furthermore, NET inhibitor Cl-Ad suppressed the release of TNF-α and IL-1β in PLF after sepsis. In order to determine that the observed influences are specifically derived from Mϕ pyroptosis, we first treated WT BMDM and RAGE−/− BMDM (as a negative control) with NETs for 12 h to induce pyroptosis, and then co-cultured the pyroptotic BMDM with normal WT BMDM in the Transwell for 6 h to assess the effect of pyroptotic Mϕ on normal neighboring Mϕ. As shown in Fig. 6c, d, WT normal Mϕ co-cultured with pyroptotic BMDM (NET-treated WT BMDM) exhibited a significant increase in TNF-α and IL-1β mRNA expression; however, WT normal Mϕ co-cultured with NET-treated RAGE−/− BMDM, which were not induced to pyroptosis, presented a much lower level of TNF-α and IL-1β mRNA expression.
Ungoverned inflammation is responsible for high morbidity and mortality during sepsis23. The interaction between innate immune cell populations, especially the interaction between PMN and Mϕ, plays a critical role in the development of inflammation24. In this study, we demonstrate a previously unidentified role for PMN–Mϕ interaction in promoting inflammation in sepsis. We showed that while NETs function as an anti-bacteria mechanism, they can also induce Mϕ death, particularly pyroptosis, which in turn enhances inflammation.
In response to infection, PMN are recruited into the infectious sites and employ three major strategies to fight against the microbes including phagocytosis, degranulation, and NETs. NETs are a meshwork of chromatin fibers mixed with granule-derived antimicrobial peptides and enzymes, such as elastase, cathepsin G, and myeloperoxidase8. Accompanied with NET ejection, a range of molecules are released into the extracellular space. Some endogenous molecules serve as DAMPs and exert the role of proinflammatory cytokine in the development of inflammatory diseases including acute organ injury7,25,26,27,28. However, the mechanism by which NET-derived DAMPs promote inflammation, remains poorly addressed. In this study, we revealed that HMGB1 released with NETs mediates Mϕ death, particularly pyroptosis, thereby amplifying the inflammation. We demonstrate that NET formation was associated with increased extracellular level of HMGB1 and inhibition of NET formation by Cl-Ad decreased the extracellular HMGB1 in vivo and in vitro. Although an elevated basal level of HMGB1 in PLF was detected after CLP, NET-caused further increase in the HMGB1 level in PLF seems required for PMϕ pyroptosis, since inhibition of NET formation significantly decreased Mϕ pyroptosis. The role of NET-released HMGB1 in inducing Mϕ pyroptosis was further evidenced by the observation that NETs formed from HMGB1−/− PMN failed to induce Mϕ pyroptosis.
As a DAMP molecule, HMGB1 implicates as an endogenous proinflammatory mediator to induce nuclear factor-kB activation and augments the secretion of TNF-α, IL-1β, IL-6, and IL-1229,30,31. Our previous studies demonstrated a novel function of HMGB1 in inducing Mϕ and vascular EC pyroptosis in non-infectious settings13,14. We demonstrated that HMGB1 acting through RAGE and dynamin-dependent signaling initiated HMGB1 endocytosis, which in turn induced cell pyroptosis. The endocytosis of HMGB1 triggered a cascade of molecular events including CatB release from the ruptured lysosomes, followed by pyroptosome formation and caspase-1 activation. However, it was not clear whether this pathway was also valid in sepsis. The current study not only explored the source of HMGB1 that induces Mϕ pyroptosis, but also validated the pathway in sepsis model. We demonstrate in this study that suppression of HMGB1–RAGE binding or its downstream events including RAGE deletion, inhibition of dynamin, CatB, and caspase-1 activation prevent Mϕ pyroptosis. These findings support a causal role for HMGB1–RAGE–dynamin signaling in the induction of cell pyroptosis, which is valid in both infectious and non-infectious conditions.
Pyroptosis was primarily defined as caspase-1-dependent death form32. Activated caspase-1 cleaves Gasdermin-D (GSDMD) to generate a mature GSDMD that induces pore formation on the membrane, resulting in cell swelling, plasma membrane rupture, and release of proinflammatory intracellular contents33. Release of intracellular molecules from the pyroptotic cells into the extracellular space is thought to be a proinflammatory event, which would result in exaggerated inflammation. In the current study, we determined the influence of Mϕ pyroptosis in the host inflammatory response. We found that the levels of TNF-α and IL-1β in PLF are significantly elevated in response to CLP; however, suppressing Mϕ pyroptosis by inhibiting NET formation or deletion of RAGE or caspase-1 markedly decreased the levels of TNF-α and IL-1β in PLF following CLP. In vitro study further showed that pyroptotic Mϕ was able to induce TNF-α and IL-1β expression in normal Mϕ, and the induction is mediated by soluble molecules from pyroptotic cells (Fig. 6c, d), since there is no physical attachment between the pyroptotic Mϕ and the normal Mϕ in the co-culture system
In summary, this study demonstrates a novel mechanism by which NETs through the release of HMGB1 induce Mϕ pyroptosis, which in turn plays an important role in directing the progress of inflammation following infection. These findings shed light on the proinflammatory role of NETs in augmenting inflammation in sepsis, and provide us with new information for generating therapeutic strategy against infectious diseases.
Materials and methods
All the mice used in the experiments were 8–10-weeks-old and on a C57BL/6 background. C57BL/6 wild-type (WT) mice were purchased from the Jackson Laboratory (Bar Harbor, ME, USA). TLR4 knockout (TLR4−/−) mice, TLR9 knockout (TLR9−/−) mice, RAGE knockout (RAGE−/−) mice, and HMGB1 knockout (HMGB1−/−) mice were obtained from Dr. Timothy Billiar’s laboratory at the University of Pittsburgh. All the animal experimental protocols were reviewed and approved by the Institutional Animal Care and Use Committees of University of Pittsburgh and VA Pittsburgh Healthcare System.
Primary antibodies for cell staining and western blotting: ASC Ab (Santa Cruz Biotechnologies), rabbit polyclonal anti-mouse HMGB1 antibody (Abcam, Cambridge, MA, USA), rabbit polyclonal anti-mouse caspase-1 p10 (Santa Cruz Biotechnologies), and GAPDH (D16H11) XP Rabbit mAb (Cell Signaling Technology). Secondary antibodies including Alexa Fluor 488-conjugated anti-mouse IgG, Cy5-conjugated anti-mouse IgG, Alexa Fluor 488-conjugated anti-rabbit IgG, and Cy3-conjugated anti-rabbit IgG were provided by the Center for Biologic Imaging, University of Pittsburgh Medicine Center. In Situ Cell Death Detection Kit, TMR red (TUNEL) was purchased from Roche (Indianapolis, IN, USA). Annexin-V detection kit was purchased from BD Biosciences. iScript™ Reverse Transcription Supermix and iTaq™ Universal SYBR® Green Supermix were purchased from Bio-Rad. Phorbol 12-myristate 13-acetate(PMA) was from Sigma-Aldrich.
Mouse model of CLP
The mouse CLP model was carried out, as previously described20. Mice were anesthetized with ketamine (50 mg/kg) and xylazine (5 mg/kg) via i.p. injection. After disinfection, a 1 cm midline laparotomy was made in the abdomen. The cecum was then exteriorized, and the distal end was ligated with a 6.0 silk suture and punctured once with a needle (21-gauge) to achieve a sublethal sepsis model. Mice were resuscitated with (5 ml/100 g) saline, and killed at different time points after surgery to retrieve the peritoneal lavage.
BMDM isolation and culture
The femurs and tibias were harvested from the WT or gene knockout mice, followed by the bone marrow being flushed with prechilled Dulbecco’s modified Eagle's medium (DMEM).34 Briefly, the cell pellets were collected by centrifugation at 4 °C, and the erythrocytes were lysed with RBC lysis buffer (Thermo Fisher Scientific). The resultant cells were then washed two times with phosphate-buffered saline (PBS) and suspended in the cell culture medium (DMEM containing 10% fetal bovine serum (FBS) complemented with 50 μg/ml penicillin/streptomycin and 10 ng/ml recombinant macrophage-colony stimulating factor (Sigma-Aldrich, St. Louis, MO, USA)) at a concentration of 1 × 106 cells/ml and seeded into 6-cm ultra-low attachment surface plates (Corning Costar, Corning, NY, USA). The BMDM culture medium was changed on day 3 and day 5. BMDM were entirely differentiated and ready for use at day 7.
PMNs isolation and NETs induction
PMNs were induced in the peritoneal cavity of the mice, as previously described.20 Briefly, mice were injected intraperitoneally with 1 ml 9% casein solution twice overnight. The mice were killed 3 h after the second injection to harvest PLF. PLF was subsequently centrifuged, and the cell pellets were washed. The PMNs were isolated by discontinuous density gradient centrifugation with two commercially available solutions (Histopaque-1077 and Histopaque-1119) of differential density purchased from Sigma (St. Louis, MO), according to the manufacturer’s instructions. PMNs (106 cells/ml) were incubated with 50 nM PMA to induce NET formation.
NET quantification assay
The PMNs were cultured in 96-well plates at a concentration of 106 cells/ml. At the indicated time points after treatment, 1 U/ml micrococcal nuclease (New England Biolabs, Ipswich, MA) was added. PMNs were incubated at 37 °C for 15 min to allow the extruded DNA to detach from the cell debris. Cells were then centrifuged at 1800 g for 10 min. Cell-impermeable DNA-binding dye SYTOX Green (Thermo Fisher Scientific, Waltham, MA) was added to the extracted supernatants and incubated in the dark for 15 min. Extracellular DNA content is represented by the mean fluorescence intensity (MFI) detected with SpectraMax M2 (excitation wavelength 485 nM and emission wavelength 530 nM).
The supernatant of PLF or cell culture medium was concentrated 20 times by Ultracel-3 membrane 3 kDa, and the BMDM lysates were separated by 8% and 15% sodium dodecyl sulfate polyacrylamide gel electrophoresis, and then transferred onto the PVDF membranes. After blocking for 1 h at room temperature with blocking buffer (LI-COR Biosciences, Lincoln, NE, USA), the blots were incubated with the primary antibody at 4 °C overnight, followed by incubation with appropriate secondary antibodies (LI-COR Biosciences) for 1 h. Protein bands were detected using the Odyssey System from LI-COR Biosciences, and the intensity of each band was quantified using ImageJ version 1.50i. The intensity of the target protein band was normalized with a reference protein band and calculated for the fold changing.
Detection of lysosome rupture and CatB activation
PMϕ/BMDM (5 × 105 cells) cultured in 35 mm Petri dishes were stimulated with NETs (200 μl) for 9 h, followed by co-culturing with DQ Ovalbumin (10 mg/ml; Molecular Probes) or Magic Red CatB assay reagent (10 mg/ml; Immunochemistry Technologies, Bloomington, MN, USA) at 37 °C for 1 h for the detection of lysosome rupture and CatB activation. After fixation with 4% paraformaldehyde, the cells were visualized by confocal microscopy. Cells were randomly selected for the measurement of intracellular fluorescence intensity by using Olympus FV10-ASW software (Olympus).
Flow cytometry analysis of programmed cell death and pyroptosis
Programmed cell death was analyzed by flow cytometry with apoptosis detection kit (BD Biosciences, Franklin Lakes, NJ). The peritoneal macrophages (PMs)/BMDM were centrifuged, washed twice with prechilled PBS, and resuspended in the binding buffer. PMs/BMDM were incubated with Annexin-V and 7-AAD for 15 min at room temperature in the dark, and then were analyzed by flow cytometry. The cells double-stained positive for Annexin-V and 7-AAD were considered to be programmed cell death. Cell pyroptosis was detected by two-color flow cytometry. PMs or BMDM were incubated with Alexa Fluor 488- labeled caspase-1 FLICA at 37 °C for 1 h. After being fixed with 4% paraformaldehyde, the PMs/BMDM were stained with TMR red-labeled In-Situ Cell Death Detection reagent (Roche Applied Science, Indianapolis, IN, USA), following the manufacturer’s instructions. The cells were then analyzed by flow cytometry. The double-stained cells were identified as pyroptotic cells. Background and auto-fluorescence were determined by a control antibody with the same isotype staining. Acquisition was performed on 10,000 events using a FACScalibur cytometer (BD Biosciences, San Jose, CA, USA), BD LSR II (BD Biosciences) and FlowJo-V10 software (Tree Star, Ashland, OR, USA). The rate of cell death was calculated as (dead cells/total cells) × 100%.
Mϕ–Mϕ co-incubation was performed using Transwell plates (Corning Incorporated Life Sciences, Acton, MA, USA). BMDM (5 × 105 cells per well) were plated and cultured in the top well of the Transwell, then treated with NETs for 18 h to induce pyroptosis, followed by transferring from the top well into a new Transwell where untreated BMDM were cultured in the bottom well. The co-cultures were then incubated for 6 h in DMEM containing 10% FBS.
RNA extraction and quantitative real-time PCR
The BMDM from the co-culture bottom wells were harvested, and total RNA was isolated by using TRIzol RNA Isolation Reagent (Thermo Fisher Scientific), following the manufacturer’s instruction. Quantitative real-time PCR was done using iTaq Universal SYBR Green Supermix (1725121, Bio-Rad) in a Bio-Rad iQ5 real-time PCR machine (Bio-Rad). The specific primers for mouse TNF-α and IL-1β were also purchased from Bio-Rad: TNF-α forward, 5′-GACGTGGAACTGGCAGAAGAG-3′ and reverse, 5′-TTGGTGGTTTGTGAGTGTGAG-3′; IL-1β forward, 5′-GAAATGCCACCTTTTGACATG-3′ and reverse, 5′-TGGATGCTCTCATCAGGACAG-3′. After the amplification protocol was over, PCR product was subjected to melt curve analysis using Bio-Rad iQ5 software. The fold change was calculated using the ΔΔCT threshold cycle method35 and the value for the GAPDH gene, which was normalized to untreated groups.
Data presentation and statistical analysis
The data are presented as mean ± S.E.M. of the indicated number of experiments. SPSS 19.0 was used for statistical analysis. Significances between groups were determined by using one-way ANOVA or two-tailed Student’s t-test. P < .05 was considered as statistically significant.
Serafini, N. et al. The TRPM4 channel controls monocyte and macrophage, but not neutrophil, function for survival in sepsis. J. Immunol. 189, 3689–3699 (2012).
Serbina, N. V., Jia, T., Hohl, T. M. & Pamer, E. G. Monocyte-mediated defense against microbial pathogens. Annu. Rev. Immunol. 26, 421–452 (2008).
Fan, J., Li, Y., Vodovotz, Y., Billiar, T. R. & Wilson, M. A. Neutrophil NAD(P)H oxidase is required for hemorrhagic shock-enhanced TLR2 up-regulation in alveolar macrophages in response to LPS. Shock 28, 213–218 (2007).
Fan, J. & Malik, A. B. Toll-like receptor-4 (TLR4) signaling augments chemokine-induced neutrophil migration by modulating cell surface expression of chemokine receptors. Nat. Med. 9, 315–321 (2003).
Jiao, Y. et al. Frontline science: macrophage-derived exosomes promote neutrophil necroptosis following hemorrhagic shock. J. Leukoc. Biol. 103, 175–183 (2017).
Fan, J., Li, Y., Vodovotz, Y., Billiar, T. R. & Wilson, M. A. Hemorrhagic shock-activated neutrophils augment TLR4 signaling-induced TLR2 upregulation in alveolar macrophages: role in hemorrhage-primed lung inflammation. Am. J. Physiol. Lung Cell Mol. Physiol. 290, L738–L746 (2006).
Warnatsch, A., Ioannou, M., Wang, Q. & Papayannopoulos, V. Neutrophil extracellular traps license macrophages for cytokine production in atherosclerosis. Science 349, 316–320 (2015).
Brinkmann, V. et al. Neutrophil extracellular traps kill bacteria. Science 303, 1532–1535 (2004).
Kaplan, M. J. & Radic, M. Neutrophil extracellular traps: double-edged swords of innate immunity. J. Immunol. 189, 2689–2695 (2012).
Papayannopoulos, V. & Zychlinsky, A. NETs: a new strategy for using old weapons. Trends Immunol. 30, 513–521 (2009).
Sorensen, O. E. & Borregaard, N. Neutrophil extracellular traps—the dark side of neutrophils. J. Clin. Invest. 126, 1612–1620 (2016).
Lotze, M. T. & Tracey, K. J. High-mobility group box 1 protein (HMGB1): nuclear weapon in the immune arsenal. Nat. Rev. Immunol. 5, 331–342 (2005).
Xu, J. et al. Macrophage endocytosis of high-mobility group box 1 triggers pyroptosis. Cell Death Differ. 21, 1229–1239 (2014).
Yang, J. et al. Hemorrhagic shock primes for lung vascular endothelial cell pyroptosis: role in pulmonary inflammation following LPS. Cell Death Dis. 7, e2363 (2016).
Wallach, D., Kang, T. B., Dillon, C. P. & Green, D. R. Programmed necrosis in inflammation: toward identification of the effector molecules. Science 352, aaf2154 (2016).
Geng, Y. et al. Heatstroke induces liver injury via IL-1beta and HMGB1-induced pyroptosis. J. Hepatol. 63, 622–633 (2015).
Chan, F. K., Luz, N. F. & Moriwaki, K. Programmed necrosis in the cross talk of cell death and inflammation. Annu. Rev. Immunol. 33, 79–106 (2015).
Yost, C. C. et al. Neonatal NET-inhibitory factor and related peptides inhibit neutrophil extracellular trap formation. J. Clin. Invest. 126, 3783–3798 (2016).
Rohrbach, A. S., Slade, D. J., Thompson, P. R. & Mowen, K. A. Activation of PAD4 in NET formation. Front. Immunol. 3, 360 (2012).
Xu, F. et al. Aging-related Atg5 defect impairs neutrophil extracellular traps formation. Immunology 151, 417–432 (2017).
Knight, J. S. et al. Peptidylarginine deiminase inhibition is immunomodulatory and vasculoprotective in murine lupus. J. Clin. Invest. 123, 2981–2993 (2013).
Stehlik, C. et al. Apoptosis-associated Speck-like protein containing a caspase recruitment domain is a regulator of procaspase-1 activation. J. Immunol. 171, 6154–6163 (2003).
Luo, L. et al. Proinflammatory role of neutrophil extracellular traps in abdominal sepsis. Am. J. Physiol. Lung Cell Mol. Physiol. 307, L586–596 (2014).
Soehnlein, O. & Lindbom, L. Phagocyte partnership during the onset and resolution of inflammation. Nat. Rev. Immunol. 10, 427–439 (2010).
Saffarzadeh, M. et al. Neutrophil extracellular traps directly induce epithelial and endothelial cell death: a predominant role of histones. PloS ONE 7, e32366 (2012).
Nakazawa, D. et al. Histones and neutrophil extracellular traps enhance tubular necrosis and remote organ injury in ischemic AKI. J. Am. Soc. Nephrol. 28, 1753–1768 (2017).
Hu, Z. et al. Neutrophil extracellular traps induce IL-1β production by macrophages in combination with lipopolysaccharide. Int. J. Mol. Med. 39, 549–558 (2017).
Kumar, S. V. et al. Neutrophil extracellular trap-related extracellular histones cause vascular necrosis in severe GN. J. Am. Soc. Nephrol. 26, 2399–2413 (2015).
Park, J. S. et al. Involvement of toll-like receptors 2 and 4 in cellular activation by high mobility group box 1 protein. J. Biol. Chem. 279, 7370–7377 (2004).
Ivanov, S. et al. A novel role for HMGB1 in TLR9-mediated inflammatory responses to CpG-DNA. Blood 110, 1970–1981 (2007).
Huebener, P. et al. The HMGB1/RAGE axis triggers neutrophil-mediated injury amplification following necrosis. J. Clin. Invest. 125, 539–550 (2015).
Bergsbaken, T., Fink, S. L. & Cookson, B. T. Pyroptosis: host cell death and inflammation. Nat. Rev. Microbiol. 7, 99–109 (2009).
Shi, J. et al. Cleavage of GSDMD by inflammatory caspases determines pyroptotic cell death. Nature 526, 660–665 (2015).
Weischenfeldt, J., Porse, B. Bone marrow-derived macrophages (BMM): isolation and applications. CSH Protocols 2008, 1–6 (2008).
Livak, K. J. & Schmittgen, T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25, 402–408 (2001).
This work was supported by the National Institutes of Health Grant HL-079669 (to J.F.), National Institutes of Health Grant HL-123882 (to J.F.), National Institutes of Health Grant HL076179 (to J.F.), VA Merit Award 1I01BX002729 (to J.F.), National Natural Science Foundation of China 81470262 (to J.F.), National Natural Science Foundation of China 81400056 (to Y.Z.), Shanghai Municipal Commission of Health and Family Planning 201540161 (to Y.Z.), Shanghai Rising-Star Program 14QA1403200 (to P.Z.), and Shanghai Medical New Excellent Youth XYQ2013115 (to P.Z.).
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The authors declare that they have no conflict of interest.
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Edited by H.-U. Simon.
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Chen, L., Zhao, Y., Lai, D. et al. Neutrophil extracellular traps promote macrophage pyroptosis in sepsis. Cell Death Dis 9, 597 (2018). https://doi.org/10.1038/s41419-018-0538-5
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