- Research article
- Open Access
Kinetic discrimination of self/non-self RNA by the ATPase activity of RIG-I and MDA5
BMC Biology volume 13, Article number: 54 (2015)
The cytoplasmic RIG-like receptors are responsible for the early detection of viruses and other intracellular microbes by activating the innate immune response mediated by type I interferons (IFNs). RIG-I and MDA5 detect virus-specific RNA motifs with short 5′-tri/diphosphorylated, blunt-end double-stranded RNA (dsRNA) and >0.5–2 kb long dsRNA as canonical agonists, respectively. However, in vitro, they can bind to many RNA species, while in cells there is an activation threshold. As SF2 helicase/ATPase family members, ATP hydrolysis is dependent on co-operative RNA and ATP binding. Whereas simultaneous ATP and cognate RNA binding is sufficient to activate RIG-I by releasing autoinhibition of the signaling domains, the physiological role of the ATPase activity of RIG-I and MDA5 remains controversial.
A cross-analysis of a rationally designed panel of RNA binding and ATPase mutants and truncated receptors, using type I IFN promoter activation as readout, allows us to refine our understanding of the structure-function relationships of RIG-I and MDA5. RNA activation of RIG-I depends on multiple critical RNA binding sites in its helicase domain as confirmed by functional evidence using novel mutations. We found that RIG-I or MDA5 mutants with low ATP hydrolysis activity exhibit constitutive activity but this was fully reverted when associated with mutations preventing RNA binding to the helicase domain. We propose that the turnover kinetics of the ATPase domain enables the discrimination of self/non-self RNA by both RIG-I and MDA5. Non-cognate, possibly self, RNA binding would lead to fast ATP turnover and RNA disassociation and thus insufficient time for the caspase activation and recruitment domains (CARDs) to promote downstream signaling, whereas tighter cognate RNA binding provides a longer time window for downstream events to be engaged.
The exquisite fine-tuning of RIG-I and MDA5 RNA-dependent ATPase activity coupled to CARD release allows a robust IFN response from a minor subset of non-self RNAs within a sea of cellular self RNAs. This avoids the eventuality of deleterious autoimmunity effects as have been recently described to arise from natural gain-of-function alleles of RIG-I and MDA5.
The cytoplasmic RIG-I-like receptors (RLRs) provide the first line of defense against virus infection [1, 2]. They recognize RNA species harboring 5′-triphosphate or diphosphate ends and/or double-stranded features (5′(p)ppdsRNA) [3–7] that are physiologically absent from the cytosol (see  for review). The highly conserved RLR family  comprises three members: RIG-I; MDA5; and LGP2. RIG-I and MDA5 detect virus infection and induce an interferon (IFN) response, whereas LGP2 acts as a regulator of RIG-I/MDA5-mediated activation (see [9, 10] for review). RIG-I and MDA5 are composed of amino-terminal tandem caspase activation and recruitment domains (CARDs), a central helicase domain (hel) and a C-terminal domain (CTD) (Fig. 1a). RIG-I or MDA5 CARDs, which are released upon cognate RNA binding, mediate signal transduction by interacting with the CARD of the membrane-bound mitochondrial antiviral signaling (MAVS) adaptor [1, 11–14]. Indeed, RNA-bound RIG-I  or MDA5 [16, 17] activate MAVS by promoting its multimerization through multiple, mixed CARD-CARD interactions. Multimerized MAVS acts as a central node to recruit the kinases responsible for converting several latent transactivators of cytokines including type I and III IFN genes. The minimal RNA required to activate RIG-I appears to be short 5′(p)ppdsRNA (10–20 nucleotides) leading initially to monomeric RNA-RIG-I complexes [18–21], which can then multimerize by K63-linked polyubiquitin chain-mediated interaction between the exposed CARDs [22, 23]. In the case of MDA5, the transduction unit is a multimer formed by the co-operative head-to-tail binding of MDA5 monomers along a >0.5–2 kb dsRNA [16, 24, 25].
Sf2 helicase/ATPase family members, including RLRs, are characterized by the coupling of nucleic acid and ATP binding to a conformational switch which, in turn, can trigger various downstream functions [12, 26]. At the same time, nucleic acid binding results in the allosteric activation of the ATPase. The sensitivity, duration and (ir)reversibility of the switch is controlled by the kinetics of ligand binding, the ATPase activity and eventual downstream effector interactions. In the case of RIG-I and MDA5, evolution has fine-tuned these receptors to exclusively detect and robustly respond to only the tiny subset of foreign RNA species that harbor a particular molecular pattern amongst the sea of cellular self RNA. Exactly how this is achieved is incompletely understood and is the subject of this study. The central sf2 hel domain comprises two recA-like domains (hel1 and hel2), with a helical insertion domain (hel2i) located at the beginning of hel2 and a pincer domain in elbow, the latter two being specific to the RLR family (Fig. 1a). Structural and biochemical studies of RIG-I and MDA5 proteins have revealed the canonical roles of the conserved motifs Ia-Ic, IIa (hel1) and IV-V (hel2) in the interaction with double-stranded RNA (dsRNA) and Q, I (Walker 1), Ia, II (Walker B), III (hel1) and VI (hel2) in the ATP binding and ATP hydrolysis [27–30]. According to several structural and biochemical studies, ligand-free RIG-I binds ATP poorly [28, 30]. The ATPase activity of RIG-I and MDA5 is stimulated only in the presence of bound dsRNA ligands [27, 28, 31], since the accurate positioning of key residues responsible for ATP hydrolysis depends on conformational changes induced by RNA binding [28, 30]. Furthermore, dsRNA has only restricted access to RIG-I hel. Indeed, the multipartite dsRNA binding site on hel (spread across hel1, hel2 and hel2i) is kept in a flexible open conformation and is partially hidden by the interaction of CARD2 with hel2i that maintains RIG-I in an auto-repressed conformation . Accordingly, the affinity of a CARD-deleted RIG-I construct for 5′pppdsRNA increases by four-fold . The high affinity of RIG-I CTD for 5′(p)ppdsRNA (0.5 nM) ensures its specific and efficient capture [5, 32–34]. As a result, the dsRNA moiety can compete efficiently with CARD2 for cis-binding to the hel domain. This results in hel wrapping around the dsRNA in a closed conformation that is stabilized by ATP binding [21, 30]. Indeed, while the isolated RIG-I hel has no/low ATPase activity even in the presence of RNA [28, 33], the hel-CTD fragment exhibits strong ATPase activity  thanks to the primary binding of the cognate RNA to the CTD [28, 33].
MDA5 shares with RIG-I a very similar structure of the hel domain and CTD . However, the recruitment of its dsRNA agonist is unlikely to result from a primary capture mediated by its CTD since MDA5 CTD only has a very weak affinity to dsRNA (3 μM for 24-mer dsRNA) [36, 37]. MDA5 hel has a slightly higher affinity (1.5 μM for 24-mer dsRNA), whereas the affinity rises by five-fold for full-length MDA5 (300 nM for 24-mer dsRNA) . Notably, the cooperative binding of MDA5 on longer dsRNA increases its affinity . In cells, MDA5 is activated mostly, if not only, by >2 kb long viral dsRNA [6, 39], higher-order viral RNA structures  or >0.5 kb of the synthetic dsRNA mimic poly(I:C) . The differently orientated CTD of MDA5 binds to both the hel-bound dsRNA and hel2i , while hel2i of one monomer binds to the pincer domain of the next monomer according to a model of the head-to tail oligomer . The structure of the inactive state of MDA5 is unknown.
The ATPase activity of RIG-I and MDA5 appears to have a central physiological role since ATPase defective and gain-of-function MDA5 and RIG-I alleles are associated with either improved viral clearance  or autoimmune diseases [42–45]. Furthermore, mutations disrupting the ATPase activity of both RIG-I [27, 28, 46, 47] and MDA5 [16, 27, 43, 48] can be associated with loss- or gain-of-function. However, the precise underlying molecular mechanisms remain puzzling. From experiments using a RIG-I construct lacking CARDs (hel-CTD) interacting with a short 5′pppdsRNA and ATP, a rapid on/off binding cycle of 1–5 s duration was interpreted as reflecting ATP-hydrolysis protein translocation along the dsRNA [49, 50]. Translocation of RIG-I, dependent on its ATPase activity, has also been invoked to explain oligomerization of RIG-I on longer 5′pppdsRNAs . In the case of MDA5, ATP hydrolysis has been shown to drive the dissociation of MDA5 from dsRNA, thus controlling the efficiency of the nucleation process leading to self-oligomerization on dsRNA . As a result, binding to short dsRNA is kinetically unstable explaining why MDA5 is activated only by >0.5–2 kb long dsRNA .
In this work, we further investigate the phenotype of RIG-I and MDA5 molecules harboring substitutions disrupting either the CARD2-hel2i interaction, the RNA binding or the ATPase activity alone or in combination. This allows us to demonstrate, for the first time, that all ATPase-deficient RIG-I and MDA5 receptors that are constitutively active rely on an intact RNA binding capability of their hel domain. Altogether our data led us to propose a model of RIG-I and MDA5 activation from auto-repressed forms in which the ATPase activity allows both helicases to kinetically discriminate invading non-self RNA from the cellular self RNA.
Functional study of RIG-I CARD2
In the absence of an agonist RNA, RIG-I is in an inactive auto-repressed state due to the binding of CARD2 to hel2i that also hinders dsRNA binding to the hel . Accordingly, when overexpressed in Huh7.5 cells, which are intrinsically deficient in RIG-I, MDA5 and the response to type I IFN (see Additional file 1 for details), wt RIG-I was unable to activate the human IFNβ promoter (Fig. 1b). Previously we reported that the mutation F539D leads to constitutive RIG-I activity consistent with this hel2i residue being key in mediating the sequestration of the CARDs according to the crystal structure of full-length duck RIG-I . Here, again based on the crystal structure, we designed an additional three human RIG-I mutants, this time on the CARD2 side of the CARD-hel2i interface. All three mutants, RIG-I_CARD[P112A,M149A], RIG-I_CARD[P112A,T116K,M149A], RIG-I_CARD[P112A,M149A,L185E], were found to be inactive despite being well-expressed (Fig. 1b and Additional file 2). Since we expected these mutants would mirror the F539D mutation and also exhibit constitutive activity, their loss-of-function phenotype suggests that the CARDs bearing these combined mutations are unable to transduce the activation signal to MAVS. The single RIG-I_CARD[P112A] substitution exhibited a 50 % reduction in its ability to activate the IFNβ promoter upon RNA stimulation after poly(I:C) or a 61-mer-5′pppdsRNA stimulation. This is in contrast to the previously reported loss of constitutive activity of isolated RIG-I CARDs carrying the same P112A mutation . Interestingly, when the P112A constructs were expressed in 293T cells, which is endowed with a minimal functional RLR and IFN response, they exhibited a significantly higher constitutive activity over that observed with wt RIG-I (see Additional file 3). This suggests that despite being inherently less efficient (P112A) and unable to be activated by cognate RNA, [P112A,M149A], those mutants could directly or indirectly stimulate an endogenous RLR response, the underlying mechanisms of which remain unclear.
Further insights in RNA binding sites of RIG-I hel domain
Within the helicase IIa motif, Q380 is a phosphate binding site for the 5′ strand of dsRNA . The Q380P substitution was introduced into the hel1 subdomain of wt RIG-I. RIG-I Q380P did not elicit signal transduction upon stimulation with poly(I:C) or 5′pppdsRNA (Fig. 1b). The combined K508A, Q511A, V514A and K518A substitutions in the hel2i subdomain interface with the dsRNA ligand could also abolish the recognition of poly(I:C) and 5′pppdsRNA in Huh7.5 cells (Fig. 1b), a phenotype that was also observed in 293T cells (Additional file 3). The comparison of RIG-I hel-CTD/RNA (PDB ID 4AY2) and MDA5 hel-CTD/RNA (PDB ID 4GL2)  structures suggested to us that hel2 residues 666–671 of hRIG-I, a partially ordered loop in most crystal structures, may contact the 5′ppp end of dsRNA. Additional file 4 shows that this is not the case since substitution of this 6 aa long loop by the corresponding 7 aa long loop from MDA5 or LGP2, or by an unrelated sequence SGSGSS, hardly affected the stimulation by 5′pppdsRNA or poly(I:C).
The constitutively active RIG-I E373Q ATPase mutant relies on both hel and CTD RNA binding sites
To evaluate the role of the ATPase activity of RIG-I in its ability to transduce a signal in cellula, the functional impact of substitutions in the helicase motifs I, II and III was studied (Fig. 1a). The K270A (motif I) mutant, which abrogates ATP binding , exhibited a significant residual response to the stimulation by 5′pppdsRNA or poly(I:C). This response was abrogated when K270A was associated with mutations previously reported to reduce the RNA binding capability of either the hel or the CTD domains, that is, by introducing the hel T697A/E702A substitutions  (called here hel°), or the CTD K888A/K907A substitutions  (called here CTD°) (Fig. 2). In contrast to K270A, we found that the E373Q (motif II) mutant displayed a significant and reproducible constitutive activity (Fig. 2) and could be further activated by both dsRNAs. When associated to hel°, E373Q became inactive as does wt RIG-I. When associated to CTD°, E373Q exhibited a response profile similar to that of its wt counterpart, namely, no constitutive activity and significantly reduced response to both dsRNAs (Fig. 2). The T409S/S411A (TS/AA) ATPase mutation (motif III) resulted in a limited response profile with no constitutive activity and a low response to both RNAs of similar magnitude to those observed with wt-CTD° and E373Q-CTD°. When TS/AA was combined with hel° the response to either dsRNA disappeared (Fig. 2). Importantly, the phenotype of E373Q was distinct from that of the constitutively active F539D mutant . Indeed, F539D remained active even when associated with either CTD° or hel° indicating a destabilization of the auto-repressed state of RIG-I. This destabilization, however, is not complete (the CARDs are not completely free) since a cognate RNA induced an additional signal to the F539D constitutive activity that was annihilated when this substitution was associated with either CTD° or hel° RNA binding mutants. Similar results were obtained when working with 293T as host cells (Additional file 3).
The constitutive activity of MDA5 ATPase mutants relies on an intact hel RNA binding site
As quoted above, the ectopic expression of hMDA5 (see Fig. 3a for domain organization) resulted in a significant activation of the human IFNβ promoter (Fig. 3b), and the response could be significantly enhanced by stimulation with Phi6 dsRNA or poly(I:C) (Fig. 3b), a finding also illustrated in Additional file 5A. All the individual K335A, E444Q, T488A/S490A (TS/AA) and G821S substitutions located in the ATPase resulted in a strong constitutive activity far exceeding the response of wt MDA5 to dsRNA stimulation (Fig. 3b), with E444Q displaying the highest and G821S the lowest activity, respectively (see also Fig. 3c). None of the ATPase mutants exhibited an additional response to Phi6 dsRNA or poly(I:C). The constitutive activity of these mutants was maintained when associated to CTD° (H927A ), showing that an intact RNA binding site on the CTD was not required. In contrast, altering the RNA binding site on MDA5 hel (R728A, hel° ) reduced the activity to the background level observed with wt MDA5. Although partially obscured by the presence of endogenous RLR and response to interferon, similar results were obtained with wt and E444Q mutant in 293T host cells (Additional file 3).
The constitutive activity of MDA5 ATPase mutants is disrupted by V protein and relies on MDA5 self-oligomerization
Paramyxovirus V protein binds tightly to the hel2 domain of MDA5 , inducing a steric clash with the bound dsRNA (see the structure superposition displayed in Additional file 5B), and inhibiting MDA5 function . Accordingly, all MDA5 ATPase mutants lost most of their constitutive activity in the presence of measles virus V (MeV V). Similar results were obtained with a C-terminally truncated V protein (MeV V-STOP) that lacks the RIWY motif that has been described to inhibit positive regulation of MDA5 signal transduction by the PP1α/γ phosphatases  (Fig. 3c). In fact, MeV V-STOP exhibited the strongest inhibitory effect on both the constitutive activity of ATPase mutants and on dsRNA-induced activation of wt MDA5. As a control, V-E235A, which is deficient in binding to MDA5  (as detailed in Additional file 5), showed a minimal inhibitory effect, as expected.
When the E444Q mutation was combined with I841K/E842R (IE/KR) substitutions that disrupt dsRNA driven MDA5 self-assembly , the constitutive activity was drastically reduced indicating the requirement of an intact MDA5 self-oligomerization process. However, both wt and E444Q MDA5 with IE/KR substitution retained a small but significant response to the stimulation with Phi6 and poly(I:C) (Fig. 3d). The use of 293T cells instead of Huh7.5 cells resulted in similar phenotype ranking (Additional file 3).
DECH/DQCH mutation in the ATPase results in reduced kinetics of ATP hydrolysis
We further studied the DECH to DQCH mutants, since the isolated E/Q mutation in the DEAD motif of another helicase/ATPase, Vasa, exhibited only very slow ATP hydrolysis and product release, allowing trapping of bound RNA . Indeed both purified duck RIG-I (Fig. 4a) and chicken MDA5 (Fig. 4b) E/Q mutant hydrolyzed ATP much slower than their wild-type counterparts. Moreover, this decrease in ATPase efficiency was not accompanied by a measurable change in the affinity for dsRNA as determined by electrophoretic mobility shift assay (EMSA) (Fig. 4d,e). Furthermore, deleting the CARDs from MDA5-E444Q resulted in a ten-fold increase in the hydrolysis slope (MDA5 hel-CTD-E444Q, Fig. 4c). This suggests a more stable access of the dsRNA in the absence of the CARDs since dsRNA/hel-CTD complex formation was quantitatively indistinguishable in EMSA (Fig. 4f). Interestingly, EMSA of MDA5 hel-CTD constructs showed three species of shifted bands that might correspond to the formation of monomers and oligomers, such supershifting being not observed with full-length MDA5 (Fig. 4, compare e and f).
In the absence of the CTD, RIG-I remains auto-repressed due to the pincer, while MDA5 remains inactive even when the pincer and the last β-strand of its hel domain are deleted
As reported previously , RIG-I with a C-terminal truncation in the pincer-CTD linker to remove the CTD domain (RIG-I 1–797, denoted CARD-hel) is unable to be activated by poly(I:C) (Fig. 5 and Additional file 6). When a similar truncation is made to hMDA5, the resulting CARD-hel construct (aa 1–895) displayed only the background activity observed with the ectopic expression of full-length MDA5, and was not activated by poly(I:C) (Fig. 5a and Additional file 6). This suggests that, as for RIG-I, MDA5 CARD-hel is maintained in an auto-repressed form. Correlatively, the CARD-hel with E/Q mutation from both RIG-I and MDA5 do not exhibit any constitutive activity as their wild-type counterparts and in marked contrast with their full-length counterparts (compare Figs. 3 and 5).
From the RIG-I and MDA5 crystal structures, the pincer domain likely contributes to maintaining the architecture of the hel domain in addition to its role in allosteric stabilization of the ATPase core . We thus questioned its role in maintaining RIG-I and MDA5 in their auto-repressed and inactive forms, respectively. Indeed, further truncation of RIG-I CARD-hel from the pincer domain alone (RIG-I 1–744, denoted Δ[pincer-CTD]), or together with the deletion of the last β-strand of hel2 (RIG-I 1–734, denoted Δ[β13pincer-CTD]), resulted in strong constitutive activity albeit lower than that observed with the CARDs alone (Fig. 5b). Surprisingly, similarly truncated MDA5 constructs (aa 1–836 and aa 1–824) did not exhibit activity above the basal background observed with full-length MDA5, suggesting that the MDA5 pincer is not required in maintaining its inactive state. Isolated CARDs from both RIG-I (aa 1–228) and MDA5 (aa 1–294) exhibited, as expected, a constitutive activity (see also Additional file 6 for other CARD constructs). These particular phenotypes of RIG-I and MDA5 truncated constructs were also observed in 293T cells (Additional file 3).
CARD sequestering by the hel domain as a common feature for auto-repressed forms of RIG-I and MDA5
Despite intensive investigations, the mechanism of RIG-I and MDA5 activation remains only partly understood. The structure of ligand-free full-length and CARD-hel RIG-I reveals an auto-repressed state with the CARD2 domain bound to the hel2i subdomain . This interaction is further supported by the 50 μM affinity measured between the isolated CARD and hel domains . This binding involves a hydrophobic network between CARD2 P112, T116, M149 and L185, and hel2i F539 . That this network drives the exposure of CARDs and signal transduction is supported by the constitutive phenotype of the F539D mutant even when associated to the hel° or CTD° domain that are deficient in RNA binding. The converse mutation of multiple CARD2 residues that include M149 results in inactive RIG-I. M149 is located at the RIG-I CARD2/MAVS CARD interface in the crystal structure of chimeric constructs , suggesting that these mutants are inactive because they cannot interact correctly with MAVS despite the CARDs being released. This further supports, as we previously suggested , that the CARD2 surface involved in the recruitment of the signaling effectors is inaccessible in the auto-repressed form of RIG-I, thus ensuring a strict dichotomy between the ‘off’ and ‘on’ activation state. The CARD-hel domain is also auto-repressed showing that the CTD is not required to maintain this state [30, 57] (Fig. 5). On the contrary, the pincer domain is required to maintain the auto-repressed state since upon its deletion, CARD-hel become constitutively active, a finding that was initially misinterpreted as indicative of CTD bearing a repressor activity when testing the truncated RIG-I 1–734 (denoted Δ[β13-pincer-CTD]) .
In the case of MDA5, the facts that the CARD-hel construct has a minimal level of constitutive activity identical to that observed with full-length MDA5 and that isolated CARDs are constitutively active  (Fig. 5 and details in Additional file 6) suggest that, in the resting state, MDA5 might also adopt an auto-repressed state with the CARDs sequestered. Contrary to RIG-I, the pincer domain does not appear to be involved in maintaining this state. The ten-fold higher ATPase activity of MDA5-E444Q construct lacking the CARDs (compare Fig. 4b and c) further suggests a competition between dsRNA and CARDs for binding to the hel domain as it is the case for RIG-I. Likewise, the formation of MDA5 oligomers suggested by supershifted bands in the absence of CARDs (Fig. 4f) compared to full-length (Fig. 4e) argues that the CARDs may mask MDA5 self-oligomerization sites. How MDA5 hel domain maintains the CARDs in an inactive state is unknown but it appears to be less robust than for RIG-I, since biochemical studies have failed to detect either the binding between bacterially expressed MDA5 CARDs and hel  or contact surfaces that would be protected from deuterium exchange . Interestingly, the CARD2 surface involved in recruiting the signaling effectors has a similar location in RIG-I and MDA5 . Importantly, the CTD of both RIG-I and MDA5 appears to be essential in alleviating their auto-repressed/inactive forms since CARD-hel constructs lacking the CTD lose their ability to be activated by their cognate RNA.
Multiplicity of critical RNA binding sites of RIG-I hel domain
In accordance with the canonical functions of the various conserved helicase motifs  and the footprint spanning 9–10 bp of dsRNA according to crystal structures , the SF2 helicase family conserved motifs primarily involved in RNA binding are motifs Ia [29, 30], Ib and Ic [28, 29], IIa [28–30], IV  and V . Consequently, critical residues for dsRNA recognition in cellula appear widely distributed all over the hel domain as functionally demonstrated with Q380 (IIa, this work), Q507, K508, Q511, V514 and K518 (hel2i, α-helix 12, this work), the participation of which is cumulative as shown by the partial reduction of dsRNA recognition exhibited by individual substitution of Q511A  or combination of only some of them (this work), and T697/D702 (V/Va) . A series of crystal structures shows the hel2i residues K508 and Q511 contacting several different base pairs along the dsRNA, which has been interpreted to reflect a sequential scanning movement of the hel2i domain along a 10-mer dsRNA . Overall, the successful recognition of 5′pppdsRNA bound to RIG-I CTD by the hel domain relies on a network of critical residues ideally arranged to support a reciprocal allosteric control with ATP fixation and hydrolysis.
Model of ATPase-mediated discrimination of non-self RNA by RIG-I
The key result from our work is the demonstration that the constitutive activity of RIG-I ATPase mutants is dependent on an intact RNA binding ability. This suggests that this constitutive activity is stimulated by the binding of cell-intrinsic RNAs and that the ATPase activity is required to avoid self-activation of RIG-I. From the available information including our present work, we propose the following model of RIG-I recognition of a cognate RNA leading to signal transduction (Fig. 6a). In the resting state, RIG-I is kept in an auto-repressed form with CARD2 binding to hel2i that impedes direct access of RNA to the hel domain, a state apparently stabilized by the pincer domain. Upon viral infection, RIG-I CTD selectively traps non-self 5′pppdsRNA ectopically present in the cytosol with high affinity (nM range [31, 32, 60]) (Fig. 6a, step 1). This favors the cis-binding of the dsRNA moiety to the hel domain favoring the co-operative binding of ATP [28, 57] (Fig. 6a, step 2). ATP fixation together with RNA binding stabilize the closed conformation of RIG-I (Fig. 6a, step 3a). RIG-I K270A, which binds weakly to ATP, is poorly active because dsRNA cannot bind stably to RIG-I hel as shown by the enhanced recycling of bound cognate RNA [61, 62]. Thus, both RNA and ATP binding to hel are needed for efficient eviction of CARD2 from hel2i and the constitution of the ATP-locked-RIG-I/5′pppdsRNA complex that can act as an active transduction unit (Fig. 6a, step 4a). At the same time, the ATPase is activated with ATP hydrolysis promoting eviction of the bound RNA from the hel domain as shown by the ATP hydrolysis-dependent recycling of cognate RNA  (Fig. 6a, step 3b). However, because the 5′pppdsRNA is firmly maintained in close proximity by remaining bound to the CTD (with notably the 5′ppp moiety enhancing the lifetime of this complex ), it can immediately rebind in cis to hel to resume another cycle of ATPase activity (Fig. 6a, step 3a). This multiple repetition of RNA/hel association/dissociation powered by the ATPase motor maintains sufficient CARD exposure (Fig. 6a, rolling steps 3a/4a/3b) to ensure a sustained number of activated RIG-I molecules per time unit above the critical threshold required for commitment, that is, ubiquitination and interaction/activation with/of MAVS and switch-on of the IFNβ promoter (Fig. 6a, rolling step 4a). Because the CTD (even with a weaker RNA binding activity as in the CTD° constructs) is strictly required and accommodates itself into a pocket in hel2i when hel is occupied by the RNA, one cannot exclude a possible contribution of the CTD to hel2i interaction in the full eviction of the CARDs from hel2i, as recently suggested .
In this model, any serendipitous binding of a non-cognate, self RNA (for example, a stem-loop structure) directly to RIG-I hel (Fig. 6b, step 2b) would be rapidly counteracted by RNA dissociation from RIG-I by the ATPase motor (Fig. 6b, step 3b) in an irreversible manner, because non-cognate, self RNA would lack the strong triphosphate anchoring to the CTD. Indeed, artificial non-optimal RNA ligands associate with increased ATPase activity, increased recycling of bound RNA and inability to activate the IFN response in cells . Consequently, the CARDs would be either never fully exposed, or only too transiently, to result in enough simultaneous activated RIG-I required for downstream oligomerization with ubiquitin chains and MAVS (Fig. 6b, step 4b). In the case of RIG-I-E373Q, serendipitous binding of self RNA (Fig. 6c, step 2b) coupled with slow ATP hydrolysis and product release delays the eviction of the RNA from hel, and consequently delays CARD2 resequestration (Fig. 6c, step 3a favored over step 3b) resulting in a high enough number of activated RIG-I-E373Q molecules per time unit (because of the increased half-life of the active RIG-I conformation) to give rise to signalling (Fig. 6c, step 4c). Interestingly, the alternative E373A substitution that is a natural constitutive variant associated with atypical Singleton-Merten syndrome  also displays a similar slow rate of ATP hydrolysis (Additional file 7). By analogy with the reduced RNA binding affinity to the yeast Has1p helicase with T/A or S/A substitution in motif III hydroxyls (SAT) , the reason why the TS/AA RIG-I mutant is inactive might be the reduced ability of hel to bind any RNA including self RNA. Thus, the ability of wt RIG-I to escape illegitimate activation by self RNA is kinetically controlled by fast ATP turnover that quickly dissociates non-cognate RNA from the hel, thus allowing reestablishment of the auto-repressed state.
Model of ATPase-mediated discrimination of non-self RNA by MDA5
In the resting state, our functional data support that MDA5 is in an inactive (possibly auto-repressed) form since MDA5 CARDs are constitutively active but CARDs-hel are not. As suggested by the higher ATPase activity resulting from the deletion of the CARDs from the MDA5-E444Q mutant, and by analogy with RIG-I, MDA5 CARDs may bind to hel to compete with RNA. As for RIG-I, the CTD is strictly required to alleviate the inactive conformation very likely because, according to the crystal structure of MDA5 [Hel-CTD + dsRNA] complex, MDA5 CTD should tightly contact hel2i when hel is occupied by RNA, this presumably freeing the CARDs for signal transduction. All together our data and previously published work suggest the following model for MDA5 discrimination of self from non-self RNA. A viral dsRNA binds to MDA5 hel (Fig. 7a, step 1), which allows CTD binding to hel2i that secures RNA binding to hel by inducing the release of the CARDs (Fig. 7a, step 2). This also results in a conformational change that exposes the self-oligomerization surface, which engages the hel2i of one monomer to the pincer domain of the next MDA5 monomer. This nucleates an assembly cascade of other MDA5 molecules on the same dsRNA (Fig. 7a, step 3) and formation of a multivalent CARD platform endowed with efficient signalling power (Fig. 7a, step 4). At the same time, dsRNA binding to hel favors the allosteric binding of ATP to the ATPase motor. This results in ATP hydrolysis (Fig. 7a, step 5) which releases the dsRNA from the hel domain of MDA5. Consequently, disassembly of the oligomer is promoted with each MDA5 monomer returning back to either reassemble (Fig. 7a, step 5) or to the inactive state (Fig. 7a, step 6). The key observation we report here of the dependence of the constitutive activity of MDA5 ATPase mutants on an intact RNA binding ability demonstrates that serendipitous binding of wt MDA5 to cellular (self) dsRNA most likely occurs (Fig. 7b). In this case, the resulting complex is too short-lived to recruit another MDA5 molecule before self RNA is expelled by the ATPase motor (that is, step 3 is pre-empted by step 5, Fig. 7b, step 4b). What makes the difference between scenario A (non-self RNA) and B (self RNA) is mainly the length of the RNA duplex: in the physiological context of a low endogenous expression of MDA5, the probability of the MDA5 nucleation process, namely recruitment of a second MDA5 molecule attracted by one bound MDA5 with exposed oligomerization surface, is predicted to increase with dsRNA length because both MDA5 rebinding to the adjacent dsRNA sequence and the frequency of recruitment of MDA5 monomers along the same RNA is favored by dsRNA lengthening. In other words, in the case of MDA5, the dsRNA length would statistically act as a surrogate RNA anchor, a role played by the CTD of RIG-I. Another difference is the ATP binding being dispensable for MDA5 signalling. Instead, it is MDA5 self-oligomerization that further stabilize MDA5 binding to dsRNA, thus creating a multimeric signalling platform. As for RIG-I, the ATPase of MDA5 is kinetically required for its desensitization, and reducing the rate of ATP hydrolysis prevents timely release of self RNA serendipitously bound to MDA5 hel (E444Q mutant, Fig. 7c step 2a). Consequently, multiple activated MDA5 molecules accumulate so as to constitute a long-lived multivalent platform that keeps transducing the downstream signal (Fig. 7c, step 3 and 4c). As discussed for RIG-I, the hel domain of the homologous mutants K335A in motif I and TS/AA in motif III are predicted to have a reduced RNA binding ability. However, this lower affinity for dsRNA appears still sufficient to engage the nucleation of MDA5 oligomerization that could not be counteracted because of the associated deficiency in ATP binding and/or hydrolysis.
We propose that RIG-I and MDA5 use their ATPase motors to kinetically avoid the formation of long-enough lived signal transducing units resulting from the binding of an illegitimate self RNA. In the case of RIG-I, accurate recognition of 5′pppdsRNA is ensured by: (i) strong binding to the CTD; (ii) cis-recognition of the dsRNA moiety by hel locked by cooperative ATP binding; and (iii) reiteration of the cis-binding of the CTD-anchored dsRNA to hel via multiple ATP hydrolysis cycles to sustain enough numbers of activated RIG-I per time unit. In the case of MDA5, the ATPase activity discards any RNA bound to MDA5 hel that does not have a dsRNA structure long enough to allow a timely efficient nucleation of MDA5 into an active oligomeric signalling platform. Interestingly, a potential source of natural cellular (self) dsRNA that RIG-I and/or MDA5 might need to discriminate against, has just been uncovered . Altogether, our work provides a framework to understand at the molecular level the contribution of several natural gain-of-function variants, including the MDA5 ATPase-deficient R337G variant, and RIG-I C268F and E373A that are associated with severe auto-immune disorders, including interferonopathy and atypical Singleton-Merten syndrome [42–45] or enhanced clearing of hepatitis C virus .
The cDNA coding for wild-type and variants of human Flag-tagged RIG-I and myc-tagged MDA5 were subcloned into pEF-BOS expression vector and measles virus V protein (Moraten strain) constructs in pCG vector using PCR amplification of cDNA fragments and the InFusion (Clontech, Mountain View, CA, USA) recombinant technique . MDA5 constructs were built on the T946 variant (pEF-MDA5-c-myc plasmid ). This variant shows genetic linkage with type I diabetes  alone or in association with R843H . It was later claimed to be associated with both a constitutive activity and a deficiency in ATP hydrolysis [43, 45]. However, Additional file 5A shows that T946 and A946 variants exhibited a similar activity profile in agreement with previous observations [65, 66]. Every RIG-I, MDA5 and MeV V insert construct after subcloning in the expression vector was entirely verified by sequencing (Eurofins, Ebersberg, Germany). All plasmids will be deposited in the Addgene plasmid repository service.
Poly(I:C) and RNA
Poly(I:C) and Phi6 dsRNA was purchased from Amersham Biosciences (Amersham, UK) and Thermo Scientific (Waltham, MA, USA), respectively. Rabies leader 5′ppp-RNA (GGACGCUUAACAACAAAACCAGAGAAGAAAAAGACA-GCGUCAAUUGCAAACGAAAAAUGUGC) was T7 transcribed and purified by excising the band from a denaturing urea-PAGE . The 61-mer-5′pppdsRNA was obtained by annealing two T7 transcribed and purified complementary 61-mer-5′ppp-ssRNA (GGUCCUGUCUGUUGUCGGU-CUCGUUUGUUGCGUGUCCGUGUUCGCCUUGGUUCCCCGGUGCC) and (CCAGGACAGACAACAGCCAGA-GCAAACAACGCACAGGCACAAGCGGAACCAAGGGGCCACGG). Both 61-mer-5′ppp-ssRNA contain only three nucleotides to avoid the formation of secondary structure and the production of double-stranded side products RNA often generated by the T7 polymerase .
Human IFNβ promoter luciferase assay
To limit the risk of signals being overshadowed by those possibly coming from endogenous or IFN-induced RIG-I or MDA5, as previously quoted , the analysis of functional phenotype of RIG-I and MDA5 proteins bearing rationally designed amino acid substitutions was performed in the Huh7.5 cell line defective in MDA5 and IFN receptor expression and expressing the inactive T55I RIG-I [69–73], a phenotype verified experimentally in Additional file 1. The phenotype of few key RIG-I and MDA5 constructs was also analyzed in 293T cells, which is equipped with a low but functional endogenous RLR with normal response to type I IFN (see Additional file 3).
The human IFNβ promoter luciferase assay was performed essentially as described [18, 30]. Briefly, Huh7.5 cells were co-transfected with RIG-I or MDA5 expressing vectors together with the reporter pb-IFN-luc followed one day later by transfection of either poly(I:C) (Amersham Biosciences), Phi6 dsRNA (Thermo Scientific) or 61-mer-5′pppdsRNA . Unless otherwise indicated, the data were expressed as mean of normalized luciferase activity and SD from three independent experiments, each done in independent triplicates.
Immunoblotting was performed as detailed elsewhere [18, 74]. Transfected cells were lysed in NP40 buffer with 6M urea (20 mM Tris HCl pH 8, 150 mM NaCl, 0.6 % NP-40, 2 mM EDTA) for 20 minutes on ice. The proteins were then separated from the cell debris by centrifugation at 7,000 g during 10 minute. The proteins were denatured by the addition of Laemmli 1 x loading buffer before analysis by SDS-PAGE and immunoblotting using anti-Flag (1:1,000; M2; Sigma, St. Louis, MO, USA), anti-C-Myc (1:50) 9E10, anti-GAPDH (1:2,000; Millipore, Billerica, MA, USA) monoclonal antibodies and rabbit polyclonal anti-P/V antiserum (1:40,000 ).
Electrophoretic mobility shift assay (EMSA)
EMSA was performed to compare the binding affinity between wild-type protein and mutated protein of duck RIG-I (dRIG-I) and chicken MDA5 (chMDA5). 12 bp and 24 bp palindromic duplex RNA (5′-pGGUAGCGCUACC-3′) (12dsRNA) (5′-pGGGACGUCAUGCGCAUGACGUCCC-3′) (24dsRNA) was cy3 labeled using a Mirus kit (Madison, WI, USA). The labeled dsRNA was dissolved with the buffer (20 mM Hepes pH 6.8, 2mM EDTA). Reactions (5 μl) contained 1.8 μM labeled dsRNA and varying concentrations of protein. The reaction mixtures were incubated for 10 minutes at room temperature in EMSA buffer (20 mM Hepes pH 7.5, 150 mM NaCl, 2 mM MgCl2, 2 mM ATP, 5 % glycerol, 0.1 mg/ml BSA). They were then loaded on a 2.5 % low melting temperature agarose gel and run with 0.5 x TBE at room temperature for 15 minutes. The gels were imaged by the fluorescent imager Typhoon Trio (Amersham Biosciences).
ATPase activity assays
ATP hydrolysis by dRIG-I and chMDA5 was measured by the Malachite green assay (BioAssay Systems, Hayward, CA, USA). Then 0.5 μM dRIG-I was preincubated with four-fold excess of a 12-mer dsRNA or 8 μM chMDA5 was preincubated with four-fold excess of a 24-mer dsRNA, for 10 minutes at 28° in ATP hydrolysis buffer (20 mM Hepes pH 7.5, 100 mM NaCl, 1 % glycerol, 2 mM DTT, 4 mM MgCl2). The reaction was initiated by adding 2 mM ATP. Reaction aliquots of 10 μl were quenched at time points between 15 seconds and 30 minutes by mixing with 10 μl of quenching buffer (20 mM Hepes pH 7.5, 100 mM NaCl, 1 % glycerol, 2 mM DTT, 100 mM EDTA). Then, 80 μl of five times diluted Malachite green reagent was added and developed for 60 minutes at room temperature. The absorbance at 622 nm was measured with a plate reader (Infinite 200 PRO; Tecan, Maennedorf, Switzerland).
Caspase activation and recruitment domain
Electrophoretic mobility shift assay
Mitochondrial antiviral signaling
Yoneyama M, Onomoto K, Jogi M, Akaboshi T, Fujita T. Viral RNA detection by RIG-I-like receptors. Curr Opin Immunol. 2015;32C:48–53.
Gerlier D, Lyles DS. Interplay between innate immunity and negative-strand RNA viruses: towards a rational model. Microbiol Mol Biol Rev. 2011;75:468–90.
Hornung V, Ellegast J, Kim S, Brzozka K, Jung A, Kato H, et al. 5′-Triphosphate RNA is the ligand for RIG-I. Science. 2006;314:994–7.
Schmidt A, Schwerd T, Hamm W, Hellmuth JC, Cui S, Wenzel M, et al. 5′-triphosphate RNA requires base-paired structures to activate antiviral signaling via RIG-I. Proc Natl Acad Sci U S A. 2009;106:12067–72.
Goubau D, Schlee M, Deddouche S, Pruijssers AJ, Zillinger T, Goldeck M, et al. Antiviral immunity via RIG-I-mediated recognition of RNA bearing 5′-diphosphates. Nature. 2014;514:372–5.
Kato H, Takeuchi O, Mikamo-Satoh E, Hirai R, Kawai T, Matsushita K, et al. Length-dependent recognition of double-stranded ribonucleic acids by retinoic acid-inducible gene-I and melanoma differentiation-associated gene 5. J Exp Med. 2008;205:1601–10.
Kato H, Takahasi K, Fujita T. RIG-I-like receptors: cytoplasmic sensors for non-self RNA. Immunol Rev. 2011;243:91–8.
Zou J, Chang M, Nie P, Secombes CJ. Origin and evolution of the RIG-I like RNA helicase gene family. BMC Evol Biol. 2009;9:85.
Zhu Z, Zhang X, Wang G, Zheng H. The laboratory of genetics and physiology 2: emerging insights into the controversial functions of this RIG-I-like receptor. Biomed Res Int. 2014;2014:960190.
Rodriguez KR, Bruns AM, Horvath CM. MDA5 and LGP2: accomplices and antagonists of antiviral signal transduction. J Virol. 2014;88:8194–200.
Kolakofsky D, Kowalinski E, Cusack S. A structure-based model of RIG-I activation. RNA. 2012;18:2118–27.
Rawling DC, Pyle AM. Parts, assembly and operation of the RIG-I family of motors. Curr Opin Struct Biol. 2014;25:25–33.
Pourcelot M, Arnoult D. Mitochondrial dynamics and the innate antiviral immune response. Febs J. 2014;281:3791–802.
Feng M, Ding Z, Xu L, Kong L, Wang W, Jiao S, et al. Structural and biochemical studies of RIG-I antiviral signaling. Protein Cell. 2013;4:142–54.
Wu B, Peisley A, Tetrault D, Li Z, Egelman EH, Magor KE, et al. Molecular imprinting as a signal-activation mechanism of the viral RNA sensor RIG-I. Mol Cell. 2014;55:511–23.
Wu B, Peisley A, Richards C, Yao H, Zeng X, Lin C, et al. Structural basis for dsRNA recognition, filament formation, and antiviral signal activation by MDA5. Cell. 2013;152:276–89.
Hou F, Sun L, Zheng H, Skaug B, Jiang QX, Chen ZJ. MAVS forms functional prion-like aggregates to activate and propagate antiviral innate immune response. Cell. 2011;146:448–61.
Louber J, Kowalinski E, Bloyet LM, Brunel J, Cusack S, Gerlier D. RIG-I Self-oligomerization is either dispensable or very transient for signal transduction. PLoS One. 2014;9, e108770.
Kohlway A, Luo D, Rawling DC, Ding SC, Pyle AM. Defining the functional determinants for RNA surveillance by RIG-I. EMBO Rep. 2013;14:772–9.
Weber M, Gawanbacht A, Habjan M, Rang A, Borner C, Schmidt AM, et al. Incoming RNA virus nucleocapsids containing a 5′-triphosphorylated genome activate RIG-I and antiviral signaling. Cell Host Microbe. 2013;13:336–46.
Zheng J, Yong HY, Panutdaporn N, Liu C, Tang K, Luo D. High-resolution HDX-MS reveals distinct mechanisms of RNA recognition and activation by RIG-I and MDA5. Nucleic Acids Res. 2015;43:1216–30.
Jiang X, Kinch LN, Brautigam CA, Chen X, Du F, Grishin NV, et al. Ubiquitin-induced oligomerization of the RNA sensors RIG-I and MDA5 activates antiviral innate immune response. Immunity. 2012;36:959–73.
Peisley A, Wu B, Xu H, Chen ZJ, Hur S. Structural basis for ubiquitin-mediated antiviral signal activation by RIG-I. Nature. 2014;509:110–4.
Berke IC, Yu X, Modis Y, Egelman EH. MDA5 assembles into a polar helical filament on dsRNA. Proc Natl Acad Sci U S A. 2012;109:18437–41.
Peisley A, Lin C, Wu B, Orme-Johnson M, Liu M, Walz T, et al. Cooperative assembly and dynamic disassembly of MDA5 filaments for viral dsRNA recognition. Proc Natl Acad Sci U S A. 2011;108:21010–5.
Fairman-Williams ME, Guenther UP, Jankowsky E. SF1 and SF2 helicases: family matters. Curr Opin Struct Biol. 2010;20:313–24.
Bamming D, Horvath CM. Regulation of signal transduction by enzymatically inactive antiviral RNA helicase proteins MDA5, RIG-I, and LGP2. J Biol Chem. 2009;284:9700–12.
Civril F, Bennett M, Moldt M, Deimling T, Witte G, Schiesser S, et al. The RIG-I ATPase domain structure reveals insights into ATP-dependent antiviral signalling. EMBO Rep. 2011;12:1127–34.
Luo D, Ding SC, Vela A, Kohlway A, Lindenbach BD, Pyle AM. Structural insights into RNA recognition by RIG-I. Cell. 2011;147:409–22.
Kowalinski E, Lunardi T, McCarthy AA, Louber J, Brunel J, Grigorov B, et al. Structural basis for the activation of innate immune pattern-recognition receptor RIG-I by viral RNA. Cell. 2011;147:423–35.
Jiang F, Ramanathan A, Miller MT, Tang GQ, Gale M, Patel SS, et al. Structural basis of RNA recognition and activation by innate immune receptor RIG-I. Nature. 2011;479:423–7.
Vela A, Fedorova O, Ding SC, Pyle AM. The thermodynamic basis for viral RNA detection by the RIG-I innate immune sensor. J Biol Chem. 2012;287:42564–73.
Cui S, Eisenacher K, Kirchhofer A, Brzozka K, Lammens A, Lammens K, et al. The C-terminal regulatory domain is the RNA 5′-triphosphate sensor of RIG-I. Mol Cell. 2008;29:169–79.
Lu C, Xu H, Ranjith-Kumar CT, Brooks MT, Hou TY, Hu F, et al. The structural basis of 5′ triphosphate double-stranded RNA recognition by RIG-I C-terminal domain. Structure. 2010;18:1032–43.
Gee P, Chua PK, Gevorkyan J, Klumpp K, Najera I, Swinney DC, et al. Essential role of the N-terminal domain in the regulation of RIG-I ATPase activity. J Biol Chem. 2008;283:9488–96.
Takahasi K, Kumeta H, Tsuduki N, Narita R, Shigemoto T, Hirai R, et al. Solution structures of cytosolic RNA sensor MDA5 and LGP2 C-terminal domains: identification of the RNA recognition loop in RIG-I-like receptors. J Biol Chem. 2009;284:17465–74.
Li X, Lu C, Stewart M, Xu H, Strong RK, Igumenova T, et al. Structural basis of double-stranded RNA recognition by the RIG-I like receptor MDA5. Arch Biochem Biophys. 2009;488:23–33.
Berke IC, Modis Y. MDA5 cooperatively forms dimers and ATP-sensitive filaments upon binding double-stranded RNA. Embo J. 2012;31:1714–26.
Feng Q, Hato SV, Langereis MA, Zoll J, Virgen-Slane R, Peisley A, et al. MDA5 detects the double-stranded RNA replicative form in picornavirus-infected cells. Cell Rep. 2012;2:1187–96.
Pichlmair A, Schulz O, Tan CP, Rehwinkel J, Kato H, Takeuchi O, et al. Activation of MDA5 requires higher-order RNA structures generated during virus infection. J Virol. 2009;83:10761–9.
Hoffmann F, Schmidt A, Dittmann Chevillotte M, Wisskirchen C, Hellmuth JC, Willms S, et al. Polymorphisms in MDA-5 link protein function to clearance of hepatitis C virus. Hepatology. 2014;61:460–70.
Jang MA, Kim EK, Now H, Nguyen NT, Kim WJ, Yoo JY, et al. Mutations in DDX58, which encodes RIG-I, cause atypical Singleton-Merten syndrome. Am J Hum Genet. 2015;96:266–74.
Funabiki M, Kato H, Miyachi Y, Toki H, Motegi H, Inoue M, et al. Autoimmune disorders associated with gain of function of the intracellular sensor MDA5. Immunity. 2014;40:199–212.
Rice GI, del Toro DY, Jenkinson EM, Forte GM, Anderson BH, Ariaudo G, et al. Gain-of-function mutations in IFIH1 cause a spectrum of human disease phenotypes associated with upregulated type I interferon signaling. Nat Genet. 2014;46:503–9.
Robinson T, Kariuki SN, Franek BS, Kumabe M, Kumar AA, Badaracco M, et al. Autoimmune disease risk variant of IFIH1 is associated with increased sensitivity to IFN-alpha and serologic autoimmunity in lupus patients. J Immunol. 2011;187:1298–303.
Kageyama M, Takahasi K, Narita R, Hirai R, Yoneyama M, Kato H, et al. 55 Amino acid linker between helicase and carboxyl terminal domains of RIG-I functions as a critical repression domain and determines inter-domain conformation. Biochem Biophys Res Commun. 2011;415:75–81.
Yoneyama M, Kikuchi M, Natsukawa T, Shinobu N, Imaizumi T, Miyagishi M, et al. The RNA helicase RIG-I has an essential function in double-stranded RNA-induced innate antiviral responses. Nat Immunol. 2004;5:730–7.
Yoneyama M, Kikuchi M, Matsumoto K, Imaizumi T, Miyagishi M, Taira K, et al. Shared and unique functions of the DExD/H-box helicases RIG-I, MDA5, and LGP2 in antiviral innate immunity. J Immunol. 2005;175:2851–8.
Myong S, Cui S, Cornish PV, Kirchhofer A, Gack MU, Jung JU, et al. Cytosolic viral sensor RIG-I is a 5′-triphosphate-dependent translocase on double-stranded RNA. Science. 2009;323:1070–4.
Hwang H, Kim H, Myong S. Protein induced fluorescence enhancement as a single molecule assay with short distance sensitivity. Proc Natl Acad Sci U S A. 2011;108:7414–8.
Patel JR, Jain A, Chou YY, Baum A, Ha T, Garcia-Sastre A. ATPase-driven oligomerization of RIG-I on RNA allows optimal activation of type-I interferon. EMBO Rep. 2013;14:780–7.
Peisley A, Jo MH, Lin C, Wu B, Orme-Johnson M, Walz T, et al. Kinetic mechanism for viral dsRNA length discrimination by MDA5 filaments. Proc Natl Acad Sci U S A. 2012;109:E3340–3349.
Motz C, Schuhmann KM, Kirchhofer A, Moldt M, Witte G, Conzelmann KK, et al. Paramyxovirus V proteins disrupt the fold of the RNA sensor MDA5 to inhibit antiviral signaling. Science. 2013;339:690–3.
Ferrage F, Dutta K, Nistal-Villan E, Patel JR, Sanchez-Aparicio MT, De Ioannes P, et al. Structure and dynamics of the second CARD of human RIG-I provide mechanistic insights into regulation of RIG-I activation. Structure. 2012;20:2048–61.
Davis ME, Wang MK, Rennick LJ, Full F, Gableske S, Mesman AW, et al. Antagonism of the phosphatase PP1 by the measles virus V protein is required for innate immune escape of MDA5. Cell Host Microbe. 2014;16:19–30.
Xiol J, Spinelli P, Laussmann MA, Homolka D, Yang Z, Cora E, et al. RNA clamping by Vasa assembles a piRNA amplifier complex on transposon transcripts. Cell. 2014;157:1698–711.
Rawling DC, Kohlway AS, Luo D, Ding SC, Pyle AM. The RIG-I ATPase core has evolved a functional requirement for allosteric stabilization by the Pincer domain. Nucleic Acids Res. 2014;42:11601–11.
Saito T, Hirai R, Loo YM, Owen D, Johnson CL, Sinha SC, et al. Regulation of innate antiviral defenses through a shared repressor domain in RIG-I and LGP2. Proc Natl Acad Sci U S A. 2007;104:582–7.
Linder P, Jankowsky E. From unwinding to clamping - the DEAD box RNA helicase family. Nat Rev Mol Cell Biol. 2011;12:505–16.
Wang Y, Ludwig J, Schuberth C, Goldeck M, Schlee M, Li H, et al. Structural and functional insights into 5′-ppp RNA pattern recognition by the innate immune receptor RIG-I. Nat Struct Mol Biol. 2010;17:781–7.
Anchisi S, Guerra J, Garcin D. RIG-I ATPase activity and discrimination of self-RNA versus non-self-RNA. MBio. 2015;6:e02349–02314.
Peisley A, Wu B, Yao H, Walz T, Hur S. RIG-I forms signaling-competent filaments in an ATP-dependent, ubiquitin-independent manner. Mol Cell. 2013;51:573–83.
Rocak S, Emery B, Tanner NK, Linder P. Characterization of the ATPase and unwinding activities of the yeast DEAD-box protein Has1p and the analysis of the roles of the conserved motifs. Nucleic Acids Res. 2005;33:999–1009.
Portal MM, Pavet V, Erb C, Gronemeyer H. Human cells contain natural double-stranded RNAs with potential regulatory functions. Nat Struct Mol Biol. 2014;22:89–97.
Andrejeva J, Childs KS, Young DF, Carlos TS, Stock N, Goodbourn S, et al. The V proteins of paramyxoviruses bind the IFN-inducible RNA helicase, mda-5, and inhibit its activation of the IFN-beta promoter. Proc Natl Acad Sci U S A. 2004;101:17264–9.
Shigemoto T, Kageyama M, Hirai R, Zheng J, Yoneyama M, Fujita T. Identification of loss of function mutations in human genes encoding RIG-I and MDA5: implications for resistance to type I diabetes. J Biol Chem. 2009;284:13348–54.
Nejentsev S, Walker N, Riches D, Egholm M, Todd JA. Rare variants of IFIH1, a gene implicated in antiviral responses, protect against type 1 diabetes. Science. 2009;324:387–9.
Marq JB, Hausmann S, Veillard N, Kolakofsky D, Garcin D. Short double-stranded RNAs with an overhanging 5′ ppp-nucleotide, as found in arenavirus genomes, act as RIG-I decoys. J Biol Chem. 2011;286:6108–16.
Li K, Chen Z, Kato N, Gale Jr M, Lemon SM. Distinct poly(I-C) and virus-activated signaling pathways leading to interferon-beta production in hepatocytes. J Biol Chem. 2005;280:16739–47.
Binder M, Eberle F, Seitz S, Mucke N, Huber CM, Kiani N, et al. Molecular mechanism of signal perception and integration by the innate immune sensor retinoic acid-inducible gene-I (RIG-I). J Biol Chem. 2011;286:27278–87.
Eguchi H, Nagano H, Yamamoto H, Miyamoto A, Kondo M, Dono K, et al. Augmentation of antitumor activity of 5-fluorouracil by interferon alpha is associated with up-regulation of p27Kip1 in human hepatocellular carcinoma cells. Clin Cancer Res. 2000;6:2881–90.
Sumpter Jr R, Loo YM, Foy E, Li K, Yoneyama M, Fujita T, et al. Regulating intracellular antiviral defense and permissiveness to hepatitis C virus RNA replication through a cellular RNA helicase. RIG-I J Virol. 2005;79:2689–99.
Keskinen P, Nyqvist M, Sareneva T, Pirhonen J, Melen K, Julkunen I. Impaired antiviral response in human hepatoma cells. Virology. 1999;263:364–75.
Brunel J, Chopy D, Dosnon M, Bloyet LM, Devaux P, Urzua E, et al. Sequence of events in measles virus replication: role of phosphoprotein-nucleocapsid interactions. J Virol. 2014;88:10851–63.
Chen M, Cortay JC, Gerlier D. Measles virus protein interactions in yeast: new findings and caveats. Virus Res. 2003;98:123–9.
We thank T Fujita, J Perrault, C Rice, S Goodbourn, D Garcin and Y Jacob for providing us with useful reagents; and T Lunardi, M Lethier and I Ivanov for their help in protein production and mutagenesis. We used the qPCR (B Blanquier) facilities of the SFR Biosciences Gerland-Lyon Sud (UMS344/US8). This work was supported by grants from FINOVI and ANR CARDINNATE (ANR12-BSV3-0010-01) to DG and SC, and ERC Advanced Grant V-RNA (322586) to SC. Materials and data are available upon request (plasmids via Addgene repository).
The authors declare that they have no competing interests.
JL, JB, EU, SC and DG designed the research. JL, JB, and EU designed and/or contributed new reagents and performed research. JL, JB, EU, SC and DG analyzed data. Every author drafted or revised the manuscript, and all authors approved the final version.
Jade Louber and Joanna Brunel contributed equally to this work.
Rationale for choosing the Huh7.5 cell line as a readout host for RLR functional analysis. (PDF 159 kb)
Functional analysis of key ( A ) RIG-I and ( B ) MDA5 protein mutants performed in 293T cells. (PDF 193 kb)
The RIG-I hel2[666–671] loop seems to favor the recognition of dsRNA with 5′ppp independently of its sequence but possibly to its shorter 6 amino acid length. (PDF 150 kb)
MDA5 T946 and A946 variants exhibit similar functional phenotypes and details of V/MDA5 interactions. (PDF 364 kb)
RIGI-I and MDA5 truncated from their CTD domain remain auto-repressed. (PDF 194 kb)
DECH/DACH mutation in ATPase domain of hRIG-I results in much slower ATP hydrolysis ability. (PDF 154 kb)
About this article
Cite this article
Louber, J., Brunel, J., Uchikawa, E. et al. Kinetic discrimination of self/non-self RNA by the ATPase activity of RIG-I and MDA5. BMC Biol 13, 54 (2015). https://0-doi-org.brum.beds.ac.uk/10.1186/s12915-015-0166-9
- self from non-self