key: cord-0942894-ezoyfsse
authors: Ferreira, André C.; Soares, Vinicius Cardoso; de Azevedo-Quintanilha, Isaclaudia G.; Dias, Suelen da Silva Gomes; Fintelman-Rodrigues, Natalia; Sacramento, Carolina Q.; Mattos, Mayara; de Freitas, Caroline S.; Temerozo, Jairo R.; Teixeira, Lívia; Damaceno Hottz, Eugenio; Barreto, Ester A.; Pão, Camila R. R.; Palhinha, Lohanna; Miranda, Milene; Bou-Habib, Dumith Chequer; Bozza, Fernando A.; Bozza, Patrícia T.; Souza, Thiago Moreno L.
title: SARS-CoV-2 engages inflammasome and pyroptosis in human primary monocytes
date: 2021-03-01
journal: Cell Death Discov
DOI: 10.1038/s41420-021-00428-w
sha: 40062544816c2356b822518c5cc0f2ce7b9b0791
doc_id: 942894
cord_uid: ezoyfsse

Infection by the severe acute respiratory syndrome coronavirus 2 (SARS-CoV-2) has been associated with leukopenia and uncontrolled inflammatory response in critically ill patients. A better comprehension of SARS-CoV-2-induced monocyte death is essential for the identification of therapies capable to control the hyper-inflammation and reduce viral replication in patients with 2019 coronavirus disease (COVID-19). Here, we show that SARS-CoV-2 engages inflammasome and triggers pyroptosis in human monocytes, experimentally infected, and from patients under intensive care. Pyroptosis associated with caspase-1 activation, IL-1ß production, gasdermin D cleavage, and enhanced pro-inflammatory cytokine levels in human primary monocytes. At least in part, our results originally describe mechanisms by which monocytes, a central cellular component recruited from peripheral blood to respiratory tract, succumb to control severe COVID-19.

Severe acute respiratory coronavirus 2 (SARS-CoV-2), the etiological agent of the 2019 coronavirus disease , emerged in China, causing a major public health burden in decades. Although patients with severe COVID-19 may present an asymptomatic/mild disease, others experience acute respiratory distress syndrome (ARDS) characterized by elevated serum levels of proinflammatory mediators-the cytokine storm 1-3 . Patients with severe COVID-19, monocytes/macrophages may be the main source of uncontrolled levels of the pro-inflammatory mediators TNF-α and IL-6 in the respiratory tract in peripheral blood 4 . Plasmatic levels of IL-6 have been associated with mortality, intensive care admission and hospitalization, representing a poor prognostic factor for COVID-19 5 . The uncontrolled inflammation triggered by SARS-CoV-2 occurs 7 to 10 days after onset of illness and associates with decreased viral loads 6, 7 .

In severe COVID-19, the cytokine storm associates with high levels of tissue insult, judged by increased levels lactate dehydrogenase (LDH) and D-dimer in the plasma [6] [7] [8] . Moreover, high LDH levels and leukopenia in severe COVID-19 points out that white cells loses the integrity of plasma membrane [8] [9] [10] [11] . Among these cells, monocytes should orchestrate the equilibrium between innate and adaptative immune responses, which may be presumably affected during cytokine storm. The leukopenia of patients with severe COVID-19 seem to precede the cytokine storm 11, 12 . Moreover, in other virus-induced cytokine storm episodes in the respiratory tract, such as induced by influenza A virus, monocytes and macrophages are severely affected 13-16 . There are various mechanisms involved in lytic cell death, which are differently engaged from development to responses to infection 17 . For certain diseases, such as COVID-19, in which the immunopathogenesis mechanisms associate with poor clinical outcomes, controlling the way cells collapse to infection is vital for the host 17 . Lytic cell death may be triggered by pyroptosis or necroptosis, in monocytes/macrophages this phenomenon exacerbates inflammation, because of release of intracellular damage-associated molecular patterns 18, 19 . Pyroptosis is a caspase-1-dependent event that leads to gasdermin D (GSDMD) pore formation 20 . Necroptosis depends on intracellular signaling of receptor-interacting protein kinases (RIPK) and mixed lineage kinase domainlike phosphorylation to form membrane pores 20 . Thus, we hypothesized that the monocyte cell death induced by SARS-COV-2 exacerbates the production of inflammatory cytokines, as well as impairs the immune balance in the hosts. In fact, we found that SARS-CoV-2 engages inflammasomes and pyroptosis in human monocytes, by experimental or natural infection. These events were associated with caspase-1 activation, IL-1ß production, GSDMD cleavage and dysregulation of cytokine release. Finally, we show that inhibition of early steps of SARS-CoV-2 life cycle by atazanavir (ATV) could block pyroptosis in SARS-CoV-2-infected human primary monocytes.

For initial assessments of SARS-CoV-2-induced monocyte death, we quantified the LDH activity in the culture supernatant and annexinV/propidium iodide (PI) labeling through flow cytometry and fluorescence microscopy. SARS-CoV-2 increased LDH levels similarly to the positive control, LPS + ATP (Fig. 1A) . SARS-CoV-2 was as potent as LPS + ATP to increase PI + cells by 300fold and PI + /annexinV + cells by 200-fold (Fig. 1B) . Flow cytometry and fluorescence microscopy also reconfirm plasma membrane disruption triggered by SARS-CoV-2 in a similar magnitude to the positive control ( Fig. 1B-E) . These data suggest that SARS-CoV-2 infection can induce lytic cell death in human primary monocytes.

Severe COVID-19 was associated with inflammasome activation 21 . Indeed, we observed that glyburide, which prevents NLR family pyrin domain containing 3 (NLRP3) activation 22 , abolished SARS-CoV-2-dependent monocyte lytic death ( Fig. 2A) . Next, we measured caspase-1 activation, a downstream event to inflammasome engagement 20 . SARS-CoV-2 induced pro-caspase-1 cleavage, similarly to LPS + ATP, by western blotting and flow cytometry analysis (Fig. 2B, C) . Apoptotic caspases-3/-7 were not upregulated in SARS-CoV-2-infected monocytes (Fig. 2F, G) .

Caspase-1 activation is known to trigger IL-1β production and GSDMD cleavage [20] [21] [22] [23] [24] . Indeed, SARS-CoV-2 infection increased IL-1β production, which was prevented by selective inhibition of capase-1 (AC-YVAD-CMK) or by treatment with pan-caspase inhibitor (Z-VAD-FMK) (Fig. 2H) . Impairment of NLPR3, by glyburide, also prevented SARS-CoV-2-induced IL-1β production (Fig. 2H) . RIPK inhibition by necrostatin could not prevent significantly IL-1β production (Fig. 2H) .

Based on the pharmacological characterization, SARS-CoV-2 depends on cellular components associated with pyroposis to promote lytic monocyte death. We thus measured the cleaved GSDMD as a proxy of the pore forming structure. In fact, SARS-CoV-2, similarly to LPS + ATP, enhanced cleaved GSDMD levels (Fig. 2I) . Importantly, inhibition of IL-1R engagement reduced SARS-CoV-2-mediated caspase-1 activation and cell lysis (Fig. S1A, B) , suggesting that inflammasome-dependent IL-1β secretion amplify caspase-1 activation and pyroptosis in SARS-CoV-2 infection.

We subsequently quantified the levels of IL-6 and TNFα, in SARS-CoV-2-infected monocytes upon pharmacological treatment to block inflammasome and pyroptosis. Inhibition of caspase-1, NLP3, and IL-1 receptor prevented SARS-CoV-2-induced enhancement of IL-6 and TNF-α levels ( Fig. 3A, B ). In addition, inhibition of IL-1 receptor engagement also reduced SARS-CoV-2dependent production of IL-1 β (Fig. S1C ). Moreover, IL-8 production, which is independent of inflammasome engagement and pyroptosis, was only modulated by pancaspase inhibition in SARS-CoV-2-infeced monocytes (Fig. S2 ).

Since lytic cell death in monocytes may depend on SARS-CoV-2 replication, we tested whether orally available generic antivirals could prevent these events. Flow cytometry analysis of SARS-CoV-2-infected monocytes treated with ATV demonstrated a significant reduction in caspase-1 activity (Fig. 4A, B) . Other orally available repurposed anti-SARS-CoV-2 drugs, such as lopinavir (LPV) and ribavirin (RBV), did not affect SARS-CoV-2induced caspase-1 activation (Fig. 4C) . Moreover, treatments with ATV did not alter the activity of caspase-1, -3 and -7 in monocytes exposed to LPS + ATP (Fig. S3) , indicating a specific antiviral activity of this drug. Consistently, treatment with ATV also reduced the levels of IL-1β, IL-6, and TNF-α in SARS-CoV-2-infected monocytes, when compared to the untreated cells ( Fig. 4D -F). ATV did not interfere with the production of IL-8, which is independent of virus-induced inflammasome engagement (Fig. 4G ). Consistently, lower levels of LDH were detected in the supernatants of SARS-CoV-2-infected monocytes treated with ATV, when compared to infected and untreated cells (Fig. 4H ). Since ATV inhibits the early proteolytic processing of viral antigens, an early event during SARS-CoV-2 replication, this drug represented the most upstream process pharmacologically inhibited in this investigation to prevent lytic monocyte death.

Caspase 1-activation, lytic monocyte death, and Il-1β associate with severe COVID-19

To clinically validate our findings, we evaluated if monocytes obtained from critically ill patients with COVID-19 would also display signals of pyroptosis-like caspase-1-dependent cell death. We observed that monocytes from COVID-19 patients had increased caspase-1 activation (Fig. 5A , B) and significantly higher lytic death, by PI+ staining, when compared to monocytes from healthy donors (HD) (Fig. 5C, D) . Corroborating with our in vitro data, we also detected higher levels of IL-1β in the plasma of critically ill patients, compared to HD (Fig. 5E) . Therefore, the in vitro results from the previous sections stand on the shoulders of the clinical relevance of monocytes in patients with severe COVID-19.

COVID-19 has caused in over 100,000 deaths/month worldwide 21 and represent the major public health crisis of the beginning of 21st century, leading to an unpredictable impact in global economics 25, 26 . SARS-CoV-2 infection triggers an uncontrolled inflammatory response and marked leukopenia with consequent lung/respiratory dysfunction 27, 28 . Similarly, to other respiratory viruses 29-31 , SARS-CoV-2 induces a cytokine storm, characterized by an uncontrolled inflammatory response mediated by monocytes/macrophages, when they should orchestrate the antiviral immune response 32 . In this work, we demonstrate that SARS-CoV-2 engages inflammasome, with subsequent caspase-1 activation, increase IL-1ß levels and GSDMD pore formation in human primary monocytes, pointing toward a pyroptotic cell death. This deleterious immune dysregulation loop triggered by SARS-CoV-2 may be impaired by ATV, glyburide and the blockage of the IL-1 receptor.

Our results demonstrate that SARS-CoV-2 leads to an intense cell death in human primary monocytes, observed by the increase in LDH release in infected cultures, as well as by the higher number of PI + cells when compared to uninfected controls, both in experimental infection and in patients with severe COVID-19. Pyroptosis is an inflammatory and lytic programmed cell death triggered after inflammasome engagement [18] [19] [20] , it has been demonstrated that NLRP3 inflammasome activation in peripheral blood mononuclear cells (PBMCs) associated with severe COVID-19 21 . We confirmed that SARS-CoV-2 infection triggers NLRP3 inflammasome engagement in monocytes, because glyburide, a drug for treatment of type 2 diabetes which modulates ATP-dependent K + channel 22 , could prevent virus-induced cell lysis. Next, we further demonstrated that downstream events could be prevented by early inhibition of virus replication, at protein translation levels, by ATV. Conversely, inhibition of viral RNA synthesis, by RBV did not affect cell death. Based on analogy with SARS-CoV from 2002, late viral proteins E, Orf3, and Orf8, which are synthetized after RNA synthesis, have been implicated in inflammasome activation 33 . Thus, it likely that other nonstructural proteins (nsp) from SARS-CoV-2 can affect intracellular K + imbalance to trigger NLRP3. Among the possible SARS-CoV-2 proteins, nsp6 may affect K + channels 34 .

Moreover, activation of caspase-1, increased production of IL-1ß and GSDMD pore was documented here in SARS-CoV-2-infected monocytes, points towards pyroptotic cell death These in vitro results are in accordance with the literature and with our finding described here that indicate the formation of inflammasomes in patients with severe COVID-19 35 . We also showed that the release of IL-1ß could be promoted by the activation of inflammasomes during the SARS-CoV-2 infection, because blockage of IL-1ß receptors reduced caspase-1 activation and cell death. These results corroborate with studies showing that the increase in IL-1ß production is associated with severe COVID-19 [36] [37] [38] [39] [40] [41] [42] [43] . Under our experimental conditions, the increase in IL-1ß precedes the unbalanced IL-6 release. These information should not be neglected when considering biopharmaceuticals to tackle cytokine storm in severe COVID-19.

To establish the clinical relevance of SARS-CoV-2induced pyroptosis in monocytes 44,45 , we analyzed peripheral monocytes isolated from patients with severe COVID-19. We found that the cells from the patients displayed higher caspase-1 activation, when compared with monocytes isolated from HD. Recent clinical data reveal high levels of LDH and consistent leukopenia in critically ill COVID-19 patients 6, 7, 35, [42] [43] [44] [45] [46] . Our data also demonstrate intense monocyte death in COVID-19 patients, as detected through flow cytometry analyzes. Altogether, these data suggest that the severity of COVID-19 may be associated with inflammasome activation in monocytes that results in large amounts of IL-1ß and generates an excessive inflammatory response, further characterized by high levels of IL-6 and TNF-α. Consistently, treatment inhibition of IL-1 receptor has been associated with clinical and inflammatory improvements in critically ill COVID-19 patients 42 . These results are in line with clinical case reports that demonstrate that monocytes/macrophages are key cells in the deleterious pro-inflammatory events that characterize the most serious cases of COVID-19 [47] [48] [49] .

In this work, we originally describe that infection by SARS-CoV-2 can engage inflammasome activation and pyroptotic cell death, which may be related to the intense leukopenia and exacerbated inflammation seen in severe cases of the COVID-19. Since there is no specific therapy for this disease, our results point out that ATV has a promising therapeutic potential against SARS-CoV-2induced cell death.

Reagents ATV and RBV were received as donations from Instituto de Tecnologia de Faŕmacos (Farmanguinhos, Fiocruz). The antiviral LPV/ritonavir (4:1 proportion) was pruchased from AbbVie (Ludwingshafen, Germany). ELISA assays were purchased from R&D Bioscience. Lipopolysacchadides-LPS, adenosine triphosphate (ATP), the specific inhibitor of caspase-1 (AC-YVAD-CMK), pan-caspase inhibitor (ZVAD-FMK), RIPK1 (Necrostatin-1-Nec-1), IL-1 receptor (IL-1RA) and glyburide were all purchased from Sigma-Aldrich (St. Louis, MO, USA). All small molecule inhibitors were dissolved in 100 % dimethylsulfoxide (DMSO) and subsequently diluted at least 10 4 -fold in culture or reaction medium before each assay. The final DMSO concentrations showed no cytotoxicity. The materials for cell culture were purchased from Thermo Scientific Life Sciences (Grand Island, NY), unless otherwise mentioned.

African green monkey kidney (Vero, subtype E6) cells were cultured in DMEM high glucose supplemented with 10% fetal bovine serum (FBS; HyClone, Logan, Utah) and 100 U/mL penicillin, and 100 μg/mL streptomycin (P/S). Vero cells were incubated at 37°C in 5% CO 2 atmosphere.

Human primary monocytes were obtained through plastic adherence of PBMCs, which were obtained from buffy coat preparations of HDs by density gradient centrifugation (Ficoll-Paque, GE Healthcare). In brief, PBMCs (2.0 × 10 6 cells) were plated onto 48-well plates (NalgeNunc) in RPMI-1640 without serum for 2-4 h; then, non-adherent cells were removed by washing and the remaining monocytes were maintained in DMEM with 5% human serum (HS; Millipore) and penicillin/ streptomycin. SARS-CoV-2 was isolated and expanded on Vero E6 cells from a nasopharyngeal swab of a confirmed case from Rio de Janeiro, Brazil. Experiments were performed after one passage in cell culture, when Vero E6 cells with DMEM plus 2% FBS in 150 cm 2 flasks were incubated at 37°C in 5% CO 2 atmosphere. Cytopathic effect was observed daily and peaked 4-5 days after infection. All procedures related to virus culture were handled at biosafety level 3 (BSL3) multiuser facility, according to WHO guidelines. Virus titers were determined as the tissue culture infectious dose at 50% (TCID50/mL). Virus stocks were kept in −80°C ultralow freezers. The virus strain was sequenced to confirm the virus identity and its complete genome is publicly deposited (GenBank accession No. MT710714).

Human primary monocytes were infected with multiplicity of infection (MOI) of 0.01 at density of 2-8 × 10 5 cells/well in 48-well culture plates, depending on the total cell number from each donor. After 1 h at 37°C, cells were washed, and various concentrations of compounds were added in DMEM with 2% FBS. After 48 h, the supernatants were harvested and virus replication was quantified by real time RT-PCR and infectious titers by TCID50/mL.

Monolayers of Vero cells (2 × 10 4 cell/well) in 96-well culture plates were infected with log-based dilutions of the supernatants containing SARS-CoV-2 for 1 h at 37°C. The cells were washed and fresh medium with 2% FBS was added. After 3-5 days, the cytopathic effects were scored in at least ten replicates per dilution by independent readers, who were blind with respect to source of the supernatant. Reed and Muench scoring method was employed to determine TCID50/mL.

For flow cytometry analysis, monocytes were diluted in labeling buffer (10 6 cells/mL). Then, 100 µL of cell samples were marked with 5 µL of AnnexinV and PI for 15 min for cell death evaluation. Around 10,000 gated events were acquired using FACSCalibur and the analysis was performed using the CellQuest software. Monocytes were gated through cell size (foward light scatter) and granularity (side light scatter) analysis.

Human monocytes were stained for caspase-1 activity with FAM-YVAD-FMK (fluorescent-labeled inhibitor of caspase-1 [FLICA] and FAM-FLICA Caspase-3/7 activity or HLA-DR APC.H7 or IgG APC.H7. Caspase-1 and caspase-3/7 activity was determined via flow cytometry (FACSCalibur) by detecting FLICA fluorescence and expression of HLA-DR as mean fluorescence intensity (MFI) value for each sample. Acquisition of data was set to count a total of 10,000 events, and the FLOWJO software package was used to analyze the data.

Human primary monocytes were plated on glass coverslips at density of 2-8 × 10 5 cells/well in 48-well plates.

Infection was performed for 2 h at 37°C and then fresh medium with 2% FBS was added. After 24 h, the cells were washed with Binding buffer and stained with PI (0.5 µg/mL) for 5 min. Next, the cells were fixed with 3.7% formaldehyde for 30 min at room temperature. The nuclei were stained with DAPI (1 µg/mL) for 5 min and the coverslips were mounted using an antifade mounting medium (VECTA-SHIELD). Fluorescence was analyzed by fluorescence microscopy with an ×100 objective lens (Olympus, Tokyo, Japan).

The levels of IL-1ß, TNF-α, IL-6, IL-8, and LDH were quantified in the culture supernatants from infected and uninfected monocytes using ELISA kits, according to the manufacturer's intructions (R&D System).

Extracellular LDH was quantified using Doles ® kit according to manufacturer's instructions. In brief, cell culture supernatants were centrifuged at 5000 rpm for 1 min, to remove cellular debris, and then 25 μL were placed into 96-well plates and incubated with 5 μL of ferric alum and 100 μL of LDH substrate for 3 min at 37°C. Nicotinamide adenine dinucleotide (oxidized form) was added followed by the addition of a stabilizing solution. After 10 min, the reaction was read in a spectrophotometer at 492 nm.

Cellular extracts of 1 × 10 6 cells were homogenized in the RIPA lysis buffer in the presence of proteinase inhibitor cocktail (Roche), and the protein levels were measured by bicinchoninic acid assay protein assay kit. A total of 20 μg of protein was loaded onto a 10% sodium dodecyl sulfate polyacrylamide gel for separation by electrophoresis and the protein bands were then transferred to a polyvinylidene difluoride membranes (ImmobilonP-SQ, Millipore). The membranes were blocked with 5% albumin diluted in Tris-buffered saline containing 0.05% of Tween 20 for 2 h at room temperature and incubated with the specific primary antibodies (Cell Signaling Technology), to detect pro-caspase-1 and cleaved-caspase-1, after overnight incubation at 4°C. After washing, membranes were incubated with secondary antibodies (IRDye ® 800CW Goat-anti-Mouse and IRDye ® 680LT Goat anti-Rabbit IgG Antibody, LI-COR, Lincoln) for 30 min at RT. The protein bands were visualized by digital fluorescence (Odyssey ® CLx Imaging System), and protein density was analyzed by the ImageJ software. All the data were normalized by β-actin expression quantification.

We prospectively enrolled severe COVID19 RT-PCRconfirmed cases, as well as SARS-CoV-2-negative healthy controls. Blood samples were obtained from 12 patients with severe COVID-19 within 72 h from intensive care unit admission in two reference centers (Instituto Estadual do Cérebro Paulo Niemeyer and Hospital Copa Star, Rio de Janeiro, Brazil). Severe COVID-19 was defined as critically ill patients presenting viral pneumonia on computed tomography scan and in mechanical ventilation. All patients had SARSCoV-2 confirmed diagnostic through RT-PCR of nasal swab or tracheal aspirates. Peripheral vein blood was also collected from eight SARS-CoV-2-negative healthy control participants as tested by RT-PCR on the day of blood sampling. The characteristics of severe (n = 12), and control (n = 8) participants are presented in Table 1 . Severe COVID-19 patients usually present older age and higher prevalence of comorbidities as obesity, cardiovascular diseases and diabetes as in previously reported patient cohorts. In the present study, the SARS-CoV-2-negative control group was designed to include subjects of older age and chronic noncommunicable diseases, so it is matched with critically ill COVID-19 patients (Table 1) . Patients with ARDS were managed with neuromuscular blockade and a protective ventilation strategy that included low tidal volume (6 mL/ kg of predicted body weight) and limited driving pressure (less than 16 cm H 2 O) as well as optimal PEEP calculated based on the best lung compliance and PaO 2 /FiO 2 ratio. In those with severe ARDS and PaO 2 /FiO 2 ratio below 150 despite optimal ventilatory settings, prone position was initiated. Our management protocol included antithrombotic prophylaxis with enoxaparin 40-60 mg per day. Patients did not receive routine steroids, antivirals, or other anti-inflammatory or anti-platelet drugs. The SARS-CoV-2-negative control participants were not under antiinflammatory or anti-platelet drugs for at least 2 weeks. All clinical information were prospectively collected using a standardized form-ISARIC/WHO Clinical Characterization Protocol for Severe Emerging Infections (CCPBR).

Experimental procedures involving human cells from HDs were performed with samples obtained after written informed consent and were approved by the Institutional Review Board (IRB) of the Oswaldo Cruz Foundation/Fiocruz (Rio de Janeiro, RJ, Brazil) under the number 397-07. The National Review Board approved the study protocol (CONEP 30650420.4.1001.0008), and informed consent was obtained from all participants or patients' representatives.

The assays were performed in blinded way. They were performed by one professional, codified and read by another fellow. All experiments were carried out at least six independent times, including a minimum of two technical replicates in each assay. The equations to fit the best curve were generated based on R 2 values ≥ 0.9. Student's t test was used to access statistically significant P values < 0.05. 

Funding was also provided by CNPq, CAPES, and FAPERJ through the National Institutes of Science and Technology Program (INCT) to Carlos Morel (INCT-IDPN) and to Wilson Savino (INCT-NIM). Thanks are due to Oswaldo Cruz Foundation/ Fiocruz under the auspicious of Inova program. The funding sponsors had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the paper, and in the decision to publish the results.

Author details

RJ, Brazil. 3 National Institute for Science and Technology on Innovation in Diseases of Neglected Populations (INCT/IDPN), Center for Technological Development in Health (CDTS), Fiocruz, Rio de Janeiro, RJ, Brazil. 4 Program of Immunology and Inflammation

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We thank the Hemotherapy Service from Hospital Clementino Fraga Filho (Federal University of Rio de Janeiro, Brazil) for providing buffy-coats. This work was supported by grants from Fundação de Amparo a Pesquisa do Estado do Rio de Janeiro (FAPERJ), Inova Fiocruz, Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) and Coordenação de Aperfeiçoamento de

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