FLIP (Flice-like inhibitory protein) suppresses cytoplasmic double-stranded-RNA-induced apoptosis and NF-κB and IRF3-mediated signaling
© Handa et al; licensee BioMed Central Ltd. 2011
Received: 30 October 2010
Accepted: 2 June 2011
Published: 2 June 2011
Cytoplasmic viral double-stranded RNA (dsRNA) is detected by a class of ubiquitous cytoplasmic RNA helicases, retinoic acid inducible gene-I (RIG-I) and melanoma differentiation antigen-5 (MDA5), which initiate a signaling cascade via their common adaptor called interferon-β (IFN-β) promoter stimulator-1 (IPS-1). This leads to the production of proinflammatory and antiviral cytokines, the type I Interferons, via mainly nuclear factor kappa B (NF-κB) and interferon response factor-3 (IRF3) transcription factors. Fas-associated death domain (FADD) protein, receptor-interacting protein (RIP1), caspase-8 and tumor necrosis factor receptor (TNFR)-associated death domain (TRADD) protein, all traditionally associated with death receptor signaling, are also involved in RIG-I/MDA5 signaling pathway. We previously showed that FLIP (Flice-like inhibitory protein), also designated as cflar (CASP8 and FADD-like apoptosis regulator), negatively regulates lipopolysaccharide (LPS)-induced toll-like receptor 4 (TLR4) signaling in endothelial cells and mouse embryonic fibroblasts (MEFs) and protected against TLR4-mediated apoptosis.
In this study, we investigated the role of FLIP in cellular response to cytoplasmic polyinosinic:polycytidylic acid, poly(I:C), a synthetic analog of dsRNA. C onsistent with the previously described role of FADD in RIG-I/MDA5-mediated apoptosis, we found that FLIP-/- MEFs were more susceptible to killing by cytoplasmic poly(I:C). However, FLIP-/- MEFs also exhibited markedly increased expression of NF-κB-and IRF3- dependent genes in response to cytoplasmic poly(I:C). Importantly, reconstitution of FLIP in FLIP-/-MEFs reversed the hyper-activation of IRF3- and NF-κB-mediated gene expression. Further, we found that caspase-8 catalytic activity was not required for cytoplasmic poly(I:C)-mediated NF-κB and IRF3 signaling.
These results provide evidence for a crucial dual role for FLIP in antiviral responses to cytoplasmic dsRNA: it protects from cytoplasmic dsRNA-mediated cell death while down-regulating IRF3-and NF-κB-mediated gene expression. Since the pathogenesis of several viral infections involves a heightened and dysregulated cytokine response, a possible therapy could involve modulating FLIP levels.
Cells respond to a viral challenge by rapidly producing type I Interferons (IFNs). The type I IFNs, IFN-α and IFN-β, are key cytokines, which induce an antiviral state and facilitate innate and adaptive immune responses . The induction of IFN-β is regulated by several transcription factors such as nuclear factor kappa (NF-κB) and interferon regulatory factor-3 (IRF3). IRF3 activation requires phosphorylation by two kinases, TANK-binding kinase 1 (TBK1) and IκB kinase (IKK)ε . Activated NF-κB and IRF3 translocate to the nucleus and trigger the expression of Type I IFNs, which are then secreted and bind to their cognate receptors on host cells. The mammalian Toll-like receptors (TLRs) that recognize the viral nucleic acids are TLR3, TLR7/8, and TLR9 for double-stranded RNA (dsRNA), single-stranded RNA, and DNA, respectively . In addition, dsRNA is sensed by a ubiquitous family of cytoplasmic RNA helicases, retinoic acid-inducible gene-I (RIG-I) and Melanoma differentiation-associated gene (MDA-5) , jointly referred to as RIG-like helicases (RLHs). While both serve as cytoplasmic sensors of RNA and function through a common adaptor protein called IPS-1 (IFN-β promoter stimulator-1, also known as MAVS, VISA, or Cardiff), a more precise picture of the substrates that they recognize has emerged. While RIG-I binds short double-stranded RNA with triphosphate or monophosphate at the 5' end, short lengths of poly(I:C) and predominantly negative sense single stranded viral RNAs [4, 5]; MDA-5 binds long lengths of poly(I:C) and mostly positive sense-single stranded viral RNA [5, 6]. The RLHs trigger the production of IFN-β in response to cytoplasmic dsRNA. The RLHs contain two caspase recruitment domains (CARDs), which mediate the activation of transcription factors like NF-κB, IRF3, and IRF7. Further, IPS-1 is also a CARD-containing downstream adaptor of the RLHs. Interestingly, several cytoplasmic adaptors of death receptor signaling have been shown to be involved in RLH signaling. IPS-1 has been demonstrated to interact with Fas-associated death domain (FADD), an adaptor in Fas signaling, and receptor-interacting protein-1 (RIP1) . Also, caspase-8, the apical caspase activated by tumor necrosis factor receptor (TNFR) and Fas, is cleaved in response to dsRNA, and, when over-expressed, its death effector domain (DED) can activate NF-κB in response to dsRNA . Further, Michallet and coworkers reported that TNFR-associated death domain (TRADD), the proximal adaptor in TNFR signaling pathway, plays a crucial role in antiviral signaling by interacting with IPS-1 and activating NF-κB and IRF3 in response to RNA virus .
In view of the involvement of several death receptor proteins in RLH signaling, we investigated the role of FLIP, a key regulator of TNFR and Fas signaling in viral responses. FLIP is homologous in structure to caspase-8, but is catalytically inactive due to critical mutations in the catalytic domain . By binding to TRADD or FADD and preventing caspase-8 recruitment, FLIP functions as a potent inhibitor of TNFR and Fas apoptotic signaling . FLIP has also been shown to regulate NF-κB activation induced by Fas engagement . Previous work from our laboratory also delineated a dual role of FLIP in response to LPS signaling through TLR4. FLIP protected against LPS-induced apoptosis and down-regulated LPS-induced NF-κB activation . In this study we find that FLIP not only protected from apoptosis induced by cytoplasmic poly(I:C), a synthetic analog of dsRNA, but also down-regulated poly(I:C)-induced NF-κB and IRF3-mediated type I IFN production. Further, we find that while the caspase-8 catalytic activity is important for poly(I:C)-induced death, it was not required for IRF3-mediated gene expression.
Cells and reagents
Wild type MEFs, FLIP-/+ heterozygous MEFs, and FLIP-/- MEFs were generous gifts of Wen-Chen Yeh, Amgen Institute, Toronto, Canada. The MEFs were cultured as described in DMEM (Hyclone) enriched with 10% fetal bovine serum, glutamine (2 mmol/L), sodium pyruvate (1 mmol/L), and non essential amino acids, in the presence of penicillin (100 U/ml) and streptomycin (100 μg/ml) . In our studies, wild type MEFs responded indistinguishably from FLIP-/+ MEFs, and therefore either was used as a control for FLIP-/-MEFs. Endotoxin-free poly(I:C) was obtained from Invivogen (San Diego, CA). For poly(I:C) stimulation experiments, MEFs were transfected with 6 μg/ml of poly(I:C) using lipofectamine 2000 (LF) (Invitrogen, Carlsbad, CA) at 8 μl/ml as described . LPS was obtained from Sigma-Aldrich (St. Louis, MO). Anti-FLIP monoclonal (Dave-2) and anti-β-actin polyclonal antibodies were purchased from Abcam (Cambridge, MA). Mouse IFN-β ELISA kit and the mouse IFN-β antibody were purchased from PBL Interferon Source (Piscataway, NJ). The anti-caspase-8 monoclonal antibody, 1G12, was obtained from Axxora (San Diego, CA). Sytox green nuclear stain was purchased from Invitrogen (Carlsbad, CA). Homogeneous caspase assay kit was purchased from Roche Applied Sciences (Palo Alto, CA). Alexa-488 Caspase-3 substrate was obtained from Biotium (Hayward, CA). Z-IETD-fmk and z-VAD-fmk, a caspase-8 inhibitor and a broad-spectrum caspase inhibitor, respectively, and membrane Fas ligand (mFasL) were purchased from R&D systems (Minneapolis, MN). Golgiplug™, obtained from BD Biosciences (San Jose, CA) was used at the recommended concentration (1 μl/106 cells) for 4 hours.
MEFs were grown in 6-well dishes to a density of 106/well and processed using the protocol as described . Anti-FLIP antibody was used to probe the blot at a concentration of 1 μg/ml (1:1000). Afterwards, the blots were stripped using Stripping buffer (Pierce, Rockford, IL) and probed with anti β-actin antibody at 1:5000 dilution. Anti-caspase-8 and anti-IFN-β antibodies were used at 1:1000 dilution.
RNA isolation and quantitative RT-PCR
Total RNA was extracted from the MEFs using the RNeasy RNA extraction kit from Qiagen (Germantown, MD) and cDNA synthesis was performed using 1 ug of total RNA according to the manufacturer's instructions (Invitrogen). Fluorescent quantitative real time PCR was performed using the Applied Biosystems HT 7900 system with the ABI Sybr Green PCR mastermix, and the data were analyzed using the ABI's SDS 2.1 software (Applied Biosystems, Foster City, CA). Mouse RT-PCR primer sequences are as follows: IFN-β forward primer-CCCTATGGAGATGACGGAGA and reverse primer-ACCCAGTGCTGGAGAAATTG, IFN-α4-forward primer CTGCTGGCTGTGAGGACATA and reverse primer-AGGAAGAGAGGGCTCTCCAG, IL-6 forward primer-AGTTGCCTTCTTGGGACTGA and reverse primer-TCCACGATTTCCCAGAGAAC, GAPDH forward primer-GCACAGTCAAGGCCGAGAAT and reverse primer-5'-GCCTTCTCCATGGTGGTGAA.
Sytox green viability assay
For apoptosis assays, MEFs were seeded at a density of 104 cells/well, followed by transfection with poly(I:C) at 6 μg/ml in the presence of 8 μl LF per ml of culture medium or poly(I:C) alone at 100 μg/ml or LF alone. Membrane FasL (1 ng/ml) was used as a positive control as it is known to cause apoptosis in FLIP-/- MEFs . Sytox green dye (5 μM) was added simultaneously along with various treatments, and the plates were read on a Cytofluor Series 4000 fluorescence plate reader (Perseptive Biosystems Inc., Framingham, MA) at 485 nm excitation and 530 nm emission after 6 hour treatment. The fluorescence on the Y-axis is representative of cells undergoing cell death.
Homogenous caspase assay
MEFs were seeded at 104 cells/well, cultured overnight, and either pretreated or not with z-IETD-fmk (100 μM) or z-VAD-fmk (100 μM) for 30 minutes followed by transfection with LF and poly(I:C) together, with appropriate controls such as poly(I:C), LF, or the caspase inhibitors (data not shown); and the caspase activity was measured using a fluorimetric caspase assay according to the manufacturer's instructions (Roche Applied Sciences), as described previously .
Alamar Blue Viability assay
To assess viability, WT or FLIP-/- MEFs were seeded into 96-well plates at a density of 20,000 cells/well. After 24 h in culture, cells were subjected to various experimental conditions and 3 h prior to the end of treatment, Alamar Blue (10% final concentration; BIOSOURCE International, Inc., Camarillo, CA) was added. Fluorescence of monolayers was assessed in a Cytofluor Series 4000 plate reader (Perseptive Biosystems Inc., Framingham, MA) at 530 nm excitation and 590 nm emission, and relative viability was expressed in arbitrary fluorescence units.
Trypan Blue dye exclusion Viability assay
To assess viability, FLIP-/- MEFs were seeded into 96-well plates at a density of 20,000 cells/well. After 24 h in culture, cells were subjected to various experimental conditions for 14 hours. Cells were washed two times with PBS, trypsinized, spun to collect, resuspended in 200 μl PBS, diluted 1:1 with Trypan blue solution, the cells that excluded the dye were counted on the hemocytometer, and the % of viable cells reported.
Statistical analysis was performed using the Graphpad statistical package (GraphPad Software Inc., La Jolla, CA). Data are expressed as mean ± SEM, and values of p < 0.05 were considered statistically significant. A two-tailed t test was used to compare mean values for two-group comparisons. To compare responses between multiple groups, data were analyzed either by one-way ANOVA with Bonferroni's Multiple Comparison post hoc test or by two-way analysis of variance and the Bonferroni-post-hoc comparison test was used to compare mean values between groups.
FLIP protects MEFs against cytoplasmic poly(I:C)-induced cell death
FLIP-/- MEFs treated with LF/poly(I:C) showed a dose-dependent increase in fluorescence, indicative of cell death, as compared to poly (I:C) (data not shown), LF, or untreated cells (Figure 1A). Compared with wild-type MEFs at 6 hours, FLIP-/-cells were markedly more sensitive to cell death in response to LF/poly(I:C). Also, mFasL caused massive cell death in FLIP-/-MEFs as compared to wild type MEFs, consistent with previous studies . Previous studies have shown that intracellular dsRNA induces apoptosis by a FADD and caspase-8-dependent mechanism [17, 18]. We therefore assessed caspase activation in LF/poly(I:C)-treated MEFs using a homogeneous caspase activity assay. Cells were pretreated with the broad-specificity caspase inhibitor zVAD-fmk or the caspase-8-selective inhibitor, z-IETD-fmk. LF/poly(I:C) and mFasL induced a marked increase in caspase activity in FLIP-/-cells compared to wild-type cells (Figure 1B), which was attenuated by pretreatment with zVAD-fmk or zIETD-fmk (Figure 1B). Further, we used the Alamar Blue metabolic assay to assess viability. Compared to WT MEFs, FLIP-/- MEFs showed a significant decline in fluorescence, indicative of cell death, in response to cytoplasmic dsRNA (Additional file 1). We also assessed cell viability by a trypan blue exclusion viability assay. As expected, treatment with LF/poly(I:C) markedly reduced viability, and this was attenuated by z-VAD-fmk (Additional file 2). Caspase activation was also detected by flow cytometric analysis using Nucview™Alexa-488-caspase 3 fluorogenic substrate, which detects caspase-3 activity in live cells. Again, FLIP-/- cells showed increased fluorescence compared to wild-type MEFs, indicative of caspase-3 activity, and this was partially reversed by pretreatment with z-IETD-fmk (data not shown). These results suggest that FLIP protects MEFs from cytoplasmic dsRNA-induced caspase activation.
FLIP suppresses LF/poly(I:C)-induced NF-κB- and IRF3-mediated gene expression in MEFs
In order to confirm results obtained by mRNA expression, IFN-β protein was assessed by ELISA. In response to LF/poly(I:C), FLIP-/-MEFs generated more IFN-β than wild-type cells or FLIP-/-cells reconstituted with FLIP (data not shown), and this overproduction was unaffected when FLIP-/-cells were pretreated with the caspase 8 inhibitor to prevent cell death during the incubation (data not shown). This result suggests that caspase-8 catalytic activity is not involved in generation of IFN-β in response to cytoplasmic dsRNA (vide infra).
We also examined levels of intracellular IFN-β in MEFs treated with Golgiplug™ (brefeldin A), which prevents cytokine secretion . Compared to WT MEFs, FLIP-/- cells showed increased intracellular levels of IFN-β in response to LF/poly(I:C) (Figure 2B).
Reconstitution of FLIP reverses the enhanced NF-KB and IRF3 activation in FLIP-/- MEFs in response to cytoplasmic dsRNA
Caspase-8 catalytic activity is not required for intracellular dsRNA-mediated signaling
There is compelling evidence that the death receptor signaling proteins TRADD, FADD, and caspase-8 are important components of cellular responses to cytoplasmic dsRNA. Michallet et al showed that TRADD is an essential component of the RIG-like helicase antiviral pathway . Their studies showed that TRADD, a crucial adaptor of the TNFRI, was recruited by IPS-1 and regulated complex formation with TRAF3/TANK and FADD/RIP1, leading to the activation of IRF3 and NF-κB. Balachandran et al and Takahashi et al showed that FADD is required for both IRF3- and NF-κB-mediated activation in response to poly(I:C). Kawai et al further demonstrated that FADD and RIP1 interact with IPS-1.
We now show that the caspase-8 homologue FLIP is a negative regulator of cytoplasmic dsRNA-induced activation of IRF3 and NF-κB. FLIP is homologous in structure to caspase-8, but is catalytically inactive due to critical mutations in the catalytic domain . FLIP associates with FADD by homophilic interaction of the death effector domains (DED) contained within each molecule . One explanation for our results is that in the absence of FLIP there is increased availability of FADD for formation of the RLH signaling module of TRADD-FADD-RIP1 , thus accounting for the increased activation NF-κB and IRF3 in FLIP-/- cells. Additionally, FLIP, via its DED, interacts with NF-kappaB-inducing kinase (NIK) and IkappaB kinase (IKK) . Since these molecules are involved in the dsRNA induction of NF-κB activation , FLIP binding and/or sequestering of NIK and IKK could hinder their ability to promote NF-κB signaling.
Our studies also show that caspase activity may not be required for activation of IRF3 and NF-κB in response to intracellular dsRNA. Using z-VAD-fmk at doses (100 μM) that abrogated all intracellular caspase activity induced by LF/poly(I:C), we found no effect of caspase blockade on LF/poly(I:C)-induced IRF3-and NF-κB-mediated gene expression. These results are in agreement with Balachandran et al who showed that activation of an IFN-β promoter by LF/poly(I:C) was similar in caspase-8-/-and WT MEFs. Furthermore, in their studies, although z-VAD-fmk (100 μM) prevented apoptosis induced by a Fas agonist antibody, the caspase inhibitor did not impair LF/poly(I:C)-induced IFN-α production . Takahashi et al showed that LF/poly(I:C)-induced IRF3 activation was unaffected and early NF-κB activation was reduced in caspase-8-/- MEFs. Most recently, Rajput et al, reported that there was enhanced activation of IRF3 by poly(I:C) in caspase-8-/- MEFs and that RIG-I-mediated activation of IRF-3 induced by intracellular dsRNA was negatively regulated by a caspase-8-dependent cleavage of RIP1 protein . They further reported that siRNA-mediated knock-down of caspase-8 had no effect on NF-κB activation by Sendai virus infection. Together, it appears that caspase-8 activity may not be required for IRF3 or NF-κB activation induced by cytoplasmic dsRNA.
In conclusion, we demonstrate a pivotal role for FLIP in protecting cells from the apoptosis and attenuating cytokine responses induced by cytoplasmic dsRNA. We have identified FLIP as a crucial molecule that regulates the response in MEFs: FLIP suppresses both inflammatory and apoptotic pathways. Strategies to increase expression of FLIP would be expected to dampen the excessive inflammation as well as apoptosis.
We would like to acknowledge the financial support from NIH grant GM071398 (JH).
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