- Research Article
- Open Access
Transcriptomic analysis of human norovirus NS1-2 protein highlights a multifunctional role in murine monocytes
BMC Genomics volume 18, Article number: 39 (2017)
The GII.4 Sydney 2012 strain of human norovirus (HuNoV) is a pandemic strain that is responsible for the majority of norovirus outbreaks in healthcare settings. The function of the non-structural (NS)1-2 protein from HuNoV is unknown.
In silico analysis of human norovirus NS1-2 protein showed that it shares features with the murine NS1-2 protein, including a disordered region, a transmembrane domain and H-box and NC sequence motifs. The proteins also contain caspase cleavage and phosphorylation sites, indicating that processing and phosphorylation may be a conserved feature of norovirus NS1-2 proteins. In this study, RNA transcripts of human and murine norovirus full-length and the disordered region of NS1-2 were transfected into monocytes, and next generation sequencing was used to analyse the transcriptomic profile of cells expressing virus proteins. The profiles were then compared to the transcriptomic profile of MNV-infected cells.
RNAseq analysis showed that NS1-2 proteins from human and murine noroviruses affect multiple immune systems (chemokine, cytokine, and Toll-like receptor signaling) and intracellular pathways (NFκB, MAPK, PI3K-Akt signaling) in murine monocytes. Comparison to the transcriptomic profile of MNV-infected cells indicated the pathways that NS1-2 may affect during norovirus infection.
Human noroviruses cause seasonal self-limiting gastroenteritis, with outbreaks common in densely populated centers such as hospitals, cruise ships, and rest homes. It is estimated that 18% of all acute gastroenteritis worldwide is caused by norovirus . In the US, norovirus mortality rates are higher in individuals aged over 65 years, whereas hospitalization is more common in children under 5 years of age . The majority of outbreaks in healthcare institutes are caused by the genogroup II.4 strains . The current pandemic strain is Sydney 2012, which arose as a recombination event between New Orleans 2009, Apeldoorn 2008 and Osaka 2007 viruses . The GII.4 Sydney strain (henceforth called HuNoV) is antigenically different to its parent strains showing low to nil blockade activity with monoclonal antibodies raised against previous pandemic norovirus strains . Currently, there is no vaccine for norovirus and anti-viral treatments have yet to be developed .
Noroviruses are a group of positive-sense, single-stranded RNA viruses that are divided into 5 genogroups. The virus consists of three open reading frames (orfs), with orf1 encoding non-structural proteins essential for virus replication and orfs 2 and 3 encode viral proteins 1 and 2, respectively, that self-assemble into capsids. In addition, genogroup V, murine norovirus (MNV) has an extra open reading frame, termed orf 4 that encodes a virulence factor involved in apoptosis . The orf1 encoding polyprotein is further cleaved into 6 proteins by the viral protease, to give rise to NS1-2 (p48), NS3 (NTPase), NS4 (p22), NS5 (VpG), NS6 (protease) and NS7 (RdRp) .
The NS1-2 protein is unique to noroviruses and contains a highly disordered proline-rich N-terminus , a putative C-terminal transmembrane domain, and caspase cleavage sites . The protein sequence shows homology to the NlpC/P60 superfamily of circular permutated enzymes based on the presence of H-box and NC motifs predicted to form a catalytic domain. These permuted papain-like NlpC/P60 enzymes function as peptidases, amidases, and acyltransferases . In addition, they are predicted to contain lipid-binding sites and play a role in the ubiquitin signaling pathway .
Cellular expression of NS1-2 protein shows a cytoplasmic distribution. The GI NS1-2 interacts with the vesicular protein SNARE  and causes Golgi disassembly . The Golgi localization and disassembly was inhibited when the predicted hydrophobic transmembrane domain of NS1-2 was removed. The GIII bovine norovirus NS1-2 on the other hand does not co-localize with Golgi or ER markers . During murine norovirus infection, NS1-2 shows cytoplasmic punctate distribution, with partial localization with ER and at the replication complex situated near the microtubule organizing center, implying that the protein may have additional roles in cellular manipulation beyond that of virus replication [16, 17]. There is very limited data on the role of norovirus NS1-2 protein during in vivo infection. In mice, MNV persistence and tropism for proximal colon was linked to the presence of a glutamate instead of aspartate at position 94 in the NS1-2 protein, indicating that the NS1-2 protein may play a role in maintenance of viral reservoirs .
It is unclear which cell type human norovirus infects during an in vivo infection, but in vitro studies showed that B cells can take up human norovirus in the presence of intestinal bacteria, with increased viral RNA in the supernatant over time, indicative of virus replication . However, for the purposes of a transcriptomic study, the presence of bacterial RNA contaminants is not desirable. More recently, human norovirus replication has been shown in specialized enteroid cultures derived from intestinal stem cells in the presence of bile . These stem cells are derived from patients undergoing intestinal biopsies for a variety of pathological conditions, which would complicate transcriptomic analysis. MNV grown in monocytes has been used a model system to study norovirus pathogenesis, including intracellular signaling and effects on immune-regulatory molecules [7, 21, 22]. Since murine monocytes are well characterised in terms of both differences and similarities to its human counterpart [23, 24], and MNV infections have been well studied [25, 26], an established murine monocyte cell line was used in this study.
The role of the HuNoV NS1-2 is unknown and this study uses transcriptomic analysis through RNA sequencing to identify the cellular pathways targeted by the HuNoV NS1-2 protein, compares it to the effects of MNV NS1-2 protein, and overall to MNV-infected cells using murine monocytes.
RAW-Blue™ cells (InvivoGen) were maintained in DMEM supplemented with 10% FCS and 200 ug/ml Zeocin™ (InvivoGen) at 37 °C with 5% CO2, and routinely passaged when 70–80% confluency was reached. Antibiotics were not added during MNV infection or RNA transfection experiments.
Virus and RNA transcripts
MNV-1 (CW1-P3) was initially generated via reverse genetics , and purified as previously described . MNV NS1-2 (nt 1–1028) and NS1-2 dis (nt 1–431) were cloned from full-length MNV-1 cDNA using forward primers containing a T7 promoter (underlined), the MNV 5′ UTR (lowercase), and nt 6–25 at the N-terminus of the MNV genome (5′-GAAATTAATACGACTCACTATAgtgaaATGAGGATGGCAACGCCATC-3′), and reverse primers containing stop codon (bold) and unique restriction enzyme sites (italics) (NS1-2 (nt 1024–1046): 5′-AGCAAGGTCGAAGGGTTATTCGGC-3′) and (NS1-2 dis (nt 409–431): 5′-GGTGGTCTGCAGTTACTCCAAGATAGAGCCGATCACAG-3′). The PCR products were confirmed for authenticity by sequencing. The Sydney GII.4 NS1-2 transcripts from 5′ to 3′ end, containing a T7 promoter, HuNoV 5′UTR, nucleotides 5–993 (NS1-2 full length) and nucleotides 5–409 (NS1-2 disordered) were obtained as synthetic genes from GenScript using the non-structural polyprotein sequence (Norovirus Hu/GII.4/Sydney/NSW0514/2012/AU GenBank AFV08794.1). Each gene had unique enzyme restriction sites flanking the sequences to allow for cloning into pUC8 vectors. The NS1-2 genes from both MNV and HuNoV were cloned into pUC8 vectors, linearized, then capped and poly(A)-tailed RNA transcripts were generated using the mMESSAGE mMACHINE T7 ultra transcription kit (Ambion). The RNA transcripts were purified, to remove unincorporated NTPs, enzymes, and buffer components, using the MEGAClear transcription clean-up kit (Ambion). Purified RNA from both HuNoV and MNV NS1-2 proteins were stored in 4 ug aliquots at −80 °C.
Infection and transfection
MNV infection was performed in triplicate, at an MOI of 5 for 12 h as described previously . Control cells were mock infected with media alone. NS1-2 and NS1-2 dis RNA for both MNV and HuNoV were transfected separately into murine monocytes using a Neon transfection system (Invitrogen); 4 ug of RNA was electroporated with 1 × 106 cells using 1 pulse for 20 milliseconds at 1730 V. The electroporated cells were immediately placed into 2 ml of pre-warmed media (per well of 6-well plate) and incubated for 12 h. Control cells were mock transfected without the RNA. All transfections were performed in triplicate. The infected and transfected samples were collected for total RNA purification and the presence of virus protein expression was confirmed by western blot (MNV NS1-2 and NS1-2 dis) or mass spectrometry analysis (HuNoV NS1-2 and NS1-2 dis). Mass spectrometry was performed by the Centre for Protein Research, Dept. of Biochemistry, University of Otago (Dunedin, NZ). MNV infection was confirmed by western blot analysis using validated antibodies for NS1-2 and viral capsid proteins .
The cell monolayer was washed with Dulbecco’s PBS (Sigma), and cells were lysed in 1 ml of TRIzol reagent (Invitrogen). RNA was extracted using the chloroform method; briefly, 200 ul chloroform was added to TRIzol samples, mixed vigorously, and incubated at RT for 2 mins. Samples were centrifuged and the RNA-containing top phase was collected (~350 ul). An equal volume of 70% ethanol was added before purifying RNA via the PureLink RNA mini kit (Invitrogen) as per manufacturers instructions. The RNA was eluted in RNase and endotoxin-free water, and stored at −80 °C. RNA quality was checked using a Bioanalyzer (Agilent Technologies) before transcriptomic analysis. Next generation sequencing service was provided by the Otago Genomics and Bioinformatics Facility using Illumina TruSeq™ RNA libraries on an Illumina HiSeq2000 platform, with 2 × 100 base pair paired end reads.
Sequencing reads were first trimmed for sequencing adaptor and then for quality at Phred score of Q20. Only paired end reads longer than 50 nucleotides were kept using the SolexaQA package . Reads were mapped against the mouse genome version 10 using TopHat  and Bowtie 2 . Read count were summarized at the transcript level using RefSeq annotation from the mapping using bed tools  and in-house PERL script. The differential expression analysis was performed using the EdgeR Bioconductor package . The library size was corrected to take into account the sequencing depth . Transcripts with less than 1 count per million (CPM) per replicate were removed. Read counts were then normalized using the trimmed mean of M-value (TMM) approach. Biological coefficient of variation was estimated using the triplicates. Differential expression (DE) analysis using a quantile adjusted conditional maximum likelihood (qCML) approach was conducted. The p-values were then adjusted using the Benjamini-Hochberg procedure with a threshold of 5% false discovery rate (FDR).
Flow cytometry analysis
Raw-Blue cells were transfected or infected as indicated above and harvested at 12hpi into 70% ethanol. The fixed cells were permeabilised with PBS buffer containing 0.1% saponin and 0.1% bovine serum albumin. Cells were incubated with rabbit anti-TLR antibodies (TLR7 (Abcam 45371) and TLR8 (Abcam 180610); 1/50 dilution) for 20 min, washed and labeled with goat anti-rabbit Alexa488 antibody (Invitrogen) for a further 20 min. Labeled cells were washed thoroughly before being analysed using BD Fortessa. Each sample contained 20,000 gated cells for analysis using FlowJo 10.1.
Alignment and phylogenetic analysis
Multiple sequence alignments were performed using the MUSCLE tool . The alignment for phylogenetic analysis was edited to eliminate poorly aligned positions and divergent regions using Gblocks software . Phylogenetic analysis was performed using MrBayes 3.2.3  on the Phylogeny.fr web server  under WAG substitution model with 10,000 generations. The phylogenetic reconstruction was then visualized using FigTree 1.4.2 (http://tree.bio.ed.ac.uk/software/figtree). All polyprotein sequences were obtained from GenBank: GI.1 Norwalk 1968 AAB50465.1, GI.2 Southampton 1991 AAA92983.1, GI.6 Kingston 2010 AFH88382.1, GI.8 Nagoya 2008 AII73782.1, GI.9 AHA91653.1, GII AKE07105.1, GII.1 Hawaii 1971 AFS33557.1, GII.2 Malaysia 1978 AFX1658.1, GII.2 Taiwan AGT39205.1, GII.3 Korea 2006 ADK23786.1, GII.3 China 1978 AFX1655.1, GII.4 Japan 2011 BAU24947.1, GII.4 Osaka 2007 BAJ13911.1, GII.4 New Orleans 2010 AEX91909.1, GII.4 Sydney 2012 AFV08794.1, GII.6 Guangzhou 2011 AGC96534.1, GII.12 Taiwan 2010 AGT39196.1, GII.14 Saga 2008 ADE28700.1, GII.17 AKB94549.1, GII.17 ALG05459.1, GIII Jena AFQ00092.1, GIV NSW 2010 AFJ21375.1, GIV.2 feline AFD30969.1, GV MNV AEY83582.1, and GV rat AFV48050.1.
Results and discussion
Phylogeny and secondary structure of HuNoV NS1-2
The sequences of the available norovirus orf1 proteins from Genbank were used to construct a phylogenetic tree showing the divergence of the NS1-2 proteins. The NS1-2 proteins cluster distinctly into their respective genogroups (Fig. 1a). The exceptions are the GII.1 Hawaii strain from 1971, which is different to the more current GII strains, and the GIII bovine strain clusters closely with the GI strains. There is significant variation between the GII strains, with the GII.4 Sydney (2012) NS1-2 protein clustering more closely with the GII.3 noroviruses than its parenteral GII.4 New Orleans strain consistent with the Sydney strain only sharing the orf2/3 capsid component with the New Orleans strain . It is also interesting to note that the more recently emerging GII.17 and GII.14 strains are clustered separately to the GII.4 strains in terms of their NS1-2 identity (Fig. 1a). Alignment of NS1-2 proteins from norovirus genogroups shows that the HuNoV Sydney NS1-2 shares 42%, 36%, and 37% amino acid identity to the Norwalk (GI), Jena (GIII; bovine), and MNV (GV) NS1-2 proteins, respectively (Clustal Omega). Despite the low sequence homology, HuNoV NS1-2 shares certain traits with the other norovirus NS1-2 proteins. They all have a proline-rich disordered N-terminus (discussed in ) and a predicted transmembrane domain at the C-terminus based on concentration of hydrophobic residues . The NS1-2 proteins also contain predicted caspase cleavage sites identified in GII.4 and GIII (DLxD*xWLS; probability 0.8), between the two GII.4 proteins (EMWD*GEIY; probability 0.7), and the two GI proteins (SARD*GVxx; probability 0.76) (Fig. 1b), as determined by Cascleave 2.0 . The GV MNV NS1-2 has functional caspase-3 cleavage sites at residues 118 (DxxD*APSH) and 128 (DAMD*AKEP) . The norovirus NS1-2 proteins also share the H-box and NC motifs (Fig. 1b) of the circular permutated NlpC/P60 family of peptidases . Circular permutation allows proteins to adopt different enzymatic abilities within the same structure, and often leads to increased stability or reduced degradation by cellular proteases . The proteins in the NlpC/P60 family are present in a wide array of prokaryotes and eukaryotic cells and function as peptidases, amidases, phospholipases, and acyltransferases. In the majority of the NlpC/P60 proteins, the catalytic domain is composed of a histidine (from H-box), a cysteine (from NC motif), and a third polar residue . In bacterial NlpC/P60 cysteine peptidase enzymes, the most commonly present polar amino acid is a histidine, followed by asparagine, glutamate, glutamine, and aspartate . In mammalian cells, the NlpC/P60 family includes LRAT (acyltransferase), HRev107-3, and TIG3 (class II tumor suppressors with phospholipase activity). Figure 1b shows the alignment of the conserved regions of norovirus NS1-2 proteins with mammalian NlpC/P60 proteins, highlighting the H-box and NC motifs and the additional polar residue. The polar residue determines substrate specificity; in HRev107-3, this residue is an arginine (Fig. 1b; red box) that is required to stabilize the phosphate group of phospholipid substrates . In viral NS1-2 proteins, there is an acidic aspartate or glutamate instead of the basic arginine residue, suggesting that the HuNoV and MNV NS1-2 proteins may not function as a phospholipase or may utilize a different substrate. A viral NlpC/P60 protein, G6R from Vaccinia virus, also does not contain the arginine residue but was predicted to bind lipids based on the charge and hydrophobicity of the residues present in the catalytic binding groove . The bacteria Mycobacterium avium subspecies paratuberculosis, which causes chronic intestinal disease in ruminants, contains a protein MAP_1204 belonging to the NlpC/P60 family that contains an acidic glutamate as the third polar residue, and this protein functions as a hydrolase . The tyrosine residue upstream of NC motif in LRAT is required for its acyltransferase activity to generate all-trans-retinyl esters [12, 45], and this residue is conserved in the norovirus NS1-2 proteins. In addition, LRAT, HRev107-3 and RIG1/TIG3 have all been shown to induce apoptosis in cancer cells, and the presence of the NC motif is crucial for this function . MNV-induced apoptosis has been attributed to the non-structural polyprotein, but has not been isolated to any individual protein in orf1 . The structures of human LRAT and TIG proteins have been resolved, but due to circular permutation of the NlpC/P60 family, these mammalian proteins cannot be used to predict the structure of the norovirus NS1-2 proteins.
The analysis of HuNoV NS1-2 sequence using the Predictor of Natural Disordered Regions (PONDR®)  server showed 37% of the protein, consisting of amino acids 1 to 124 at the N-terminus, is disordered (Fig. 2a). This profile is similar to the previously published disorder profiles of GI.1, GI.2, GIII, and GV (MNV) NS1-2 proteins . The predicted caspase cleavage site at amino acid 134 (EMWD-GEIY; 0.7 probability), at the termination of the inherently disordered region (yellow arrow; Fig. 2a) was chosen as the termination site for NS1-2 dis for this study. Figure 2a also shows the location of the H-box and NC motif (blue arrows), and the predicted transmembrane domain (red double arrow; PSIPRED) in the highly conserved/ordered region of the protein. The HuNoV NS1-2 secondary structure, hydropathy, and flexibility predictions are comparable to the previously published MNV NS1-2 protein analysis . The disordered region of HuNoV NS1-2 contains limited secondary structure, and has residues that are predominately hydrophilic, flexible, and immunogenic, when compared to the full-length NS1-2 protein. Comparison of the inherently disordered regions shows areas of conservation between the HuNoV and MNV NS1-2 dis proteins that are not apparent with whole protein alignment (Fig. 2b). These similarities could play a role in interactions this disordered region has with other molecules. Analysis of MNV NS1-2 dis and HuNoV NS1-2 dis sequences using Prosite motif finder  showed that MNV NS1-2 dis protein did not match up to any known sequences, whereas the HuNoV NS1-2 dis showed sequence similarity to a putative Mycobacterium virulence protein predicted to bind to and inhibit IgG responses (NCBI-CDD 275319). The conserved motifs in MNV and HuNoV NS1-2 dis correspond to putative MHC-I epitope binding sites when compared against the Immune Epitope Database , indicating that the disordered part of NS1-2 may induce an immune response. Antibodies generated against full length MNV NS1-2 also bound the disordered N-terminal region of the protein, indicating that the disordered region is immunogenic , hence this disordered region may serve as a target for cell-mediated immune responses against norovirus.
The Disorder-Enhanced Phosphorylation Sites Predictor (DISPHOS 1.3)  predicted that the threonine-61 of HuNoV NS1-2 is phosphorylated, with a probability of 0.9 and 0.87, in human and murine cells, respectively (Fig. 2a and b; blue circle). Murine NS1-2 analysis using DISPHOS suggests that the protein may be phosphorylated at threonine-15 and tyrosine-47 (0.5 probability; Fig. 2b; blue circles). Threonine phosphorylation on kinase-type proteins are required for catalytic activity . In eukaryotic cells, phosphorylation activates a variety of cellular pathways, including cell cycle regulation, apoptosis and immune cell activation . RNA viruses, such as HIV and Hepatitis C, utilize host kinases to phosphorylate viral proteins in order to increase the viral proteome to aid virus replication [54, 55]. Hepatitis C virus NS5A protein contains a phosphorylated threonine amongst proline-rich disordered residues that is crucial for replication center formation and production of virions . In MNV-infected monocytes, NS1-2 is partially localized to the replication complex but it is not known what role it plays in replication .
HuNoV NS1-2 and NS1-2 dis induced transcriptomic profile
HuNoV NS1-2 and NS1-2 dis RNA transfections were carried out in triplicate, and cells electroporated without RNA were used as controls (mock-transfected). Cellular RNA was extracted and sequenced using Illumina TruSeq™ RNA libraries on an Illumina HiSeq2000 platform with 2 × 100 base pair paired end reads. The quality control, read mapping, read count, and differential expressed genes were performed as described in methods. The PCA plots of HuNoV NS1-2 and NS1-2 dis transfected cell samples showed that the triplicate samples clustered together and there is good separation between mock and viral protein transfected cells (Additional file 1: Figure S1). Smearplots of genes that are upregulated and downregulated in NS1-2 and NS1-2 dis are shown in Fig. 3a and b, respectively. Transfection of HuNoV NS1-2 altered the expression of 1735 genes, whereas HuNoV NS1-2 dis transfected cells had 1269 genes that changed compared to mock transfected samples (Cut off at 5% FDR, with 2-fold change). Of these differentially expressed (DE) genes, 1197 were shared between the two conditions (Fig. 3c). This left 538 DE genes found solely in the HuNoV NS1-2 transfected cells, suggesting that the ordered region of the viral protein in context with the disordered region was required for these cellular interactions. HuNoV NS1-2 dis transfected cells had 72 DE genes that were attributed solely to the disordered protein. The differentially expressed genes were further analysed by DAVID  and Panther  databases to categorise pathways and protein classes that were specifically up- or down-regulated in the presence of HuNoV NS1-2 and NS1-2 dis proteins.
Figure 3d shows the shared gene between the HuNoV NS1-2 and NS1-2 dis proteins classified into Panther pathways . Using the Panther-db, majority of the DE genes are classified under inflammation mediated by chemokine and cytokine, integrin signalling, Toll-like receptor signalling, apoptosis, and ubiquitin proteasome pathways. The DE genes can also be classified separately into pathways that are either up- or down-regulated using Kegg classification. Table 1 shows that the upregulated genes belong to the pathways involved in proteasome, apoptosis, antigen processing and presentation, and gap junction interactions. The genes in RIG-I-like, NOD-like, and MAPK intracellular signalling pathways are also upregulated. The downregulated genes belong to the pathways involved in lysosomes, cell adhesion molecules, and transendothelial migration. In addition, the genes in p53, mTOR, and phosphatidylinositol signalling pathways are downregulated. There are some pathways where select genes are both up- and down-regulated, and these include cytokine-cytokine receptor interactions, Toll-like receptor signalling, focal adhesion, and regulation of actin cytoskeleton.
At first glance, these Kegg and Panther pathways appear to be diverse but they do contain similarities; the PI3-K and chemokine pathways require GTPases to function, and all the intracellular pathways use phosphorylation as a means of molecular activation [60, 61]. Further categorisation of these DE genes as molecular function (Kegg classification) showed that the types of proteins altered in response to HuNoV NS1-2 and NS1-2 dis can be classified as 43% phosphoproteins and 31% nucleotide-binding proteins, with 25% comprising solely of ATP-binding proteins (Table 2).
The 538 DE genes present solely in HuNoV NS1-2 group mainly into the lysosome, proteasome, and RIG-1-like receptor signalling Kegg pathways (Fig. 4a). Panther classification of the same DE genes group to integrin-signalling, Toll-like receptors, and ubiquitin-proteasome pathways (Fig. 4b). When looking at the class of proteins that are altered by presence of HuNoV NS1-2, phosphoproteins made up 53% and acetylation constitutes 25% of the DE genes (data not shown). This suggests that the ordered region of the NS1-2 protein may play a role in regulating phosphorylated and/or acetylated proteins, as shown for mammalian proteins with the H-box and NC motif, such as LRAT and retinoic acid responder 3 (RARRES3) . When looking at the cellular placement of the proteins altered by HuNoV NS1-2, 26% of the proteins are cytoplasmic and 29% are nuclear. Transfection of HuNoV NS1-2 into cells results in a diffuse cytoplasmic distribution with no nuclear localisation detected. Previous studies with Norwalk virus and MNV NS1-2 proteins have shown the same distribution pattern [13, 16]. The effects on nuclear proteins by HuNoV NS1-2 are more likely to be due to changes in transport across nuclear membrane that are related to modifications such as phosphorylation, rather than direct presence of NS1-2 in the nucleus.
The DE genes altered by the expression of HuNoV NS1-2 dis alone do not classify well into either Kegg or Panther pathways likely due to the small size of the gene set. Off the 77 DE genes, only 4 belong to the Ras pathway with GTPase function. The other DE genes do not correlate to any specific Kegg or Panther pathway, but do contain proteins that bind cations and/or specific motifs, such as zinc finger domains and kelch motifs (discussed below).
Taken together, the transcriptomic profile of murine cells expressing HuNoV NS1-2 and NS1-2 dis suggests that the virus protein affects multiple pathways. One of the possibilities based on in silico analysis is that HuNoV NS1-2 performs an enzymatic function. The enzymatic function of NS1-2 protein is likely to be related to phosphorylation, acetylation, or NTPase activity based on the pathways that are altered in cells expressing virus protein. The data also suggests that the disordered region of the NS1-2 protein may bind specific motifs or cations in substrate host protein that may lead to the enzymatic activity by the ordered region of the viral protein containing the H-box and NC motifs. As discussed previously, HuNoV NS1-2 contains the catalytic Y residue and NC motif in mammalian LRAT proteins required for acyltransferase activity and apoptosis, respectively.
Comparison of HuNoV NS1-2 dis and MNV NS1-2 dis
Since the DE genes in HuNoV NS1-2 dis did not correlate well into distinct pathways, the changes in HuNoV NS1-2 dis transfected cells were compared to those in MNV NS1-2 dis cells. The disordered region of the HuNoV and MNV NS1-2 proteins share 153 DE genes when compared to mock-transfected cells. There is good correlation between the up- and down-regulated genes between the two viral proteins. Analysis of the up and downregulated DE genes present in both HuNoV NS1-2 dis and MNV NS1-2 dis using the String-db  showed presence of 2 distinct clusters involved in interferon regulation and cell cycle/apoptosis, with a further smaller cluster of genes with uncharacterised function (Fig. 5a). The upregulated genes of interest include the Schlafen gene family, STAT1 and IRF transcription factors, indicating interferon-dependent activation in the NS1-2 dis protein transfected monocytes [64, 65]. Further, the genes induced by IFN upregulation, such as Oas enzymes, are also upregulated in both HuNoV and MNV NS1-2 dis samples, indicating that the NS1-2 dis protein activates a pro-inflammatory profile in monocytes. Analysis of the DE genes using Panther-db showed that they belong to the biological processes of nucleotide metabolism, cell cycle, IFN-mediated immunity, MHC-I, and T cells (Fig. 5b). The DE genes can also be grouped into protein families (Fig. 5c), with the highest number of genes in the melanoma-like 3 antigen family, the majority of which includes uncharacterised genes. Other protein families of interest, aside from the previously mentioned Schlafen and IFN proteins, include proteins with Kelch and EH domains, required for protein-protein interactions and intracellular sorting. The DE genes also include protein families with zinc finger motifs and helicases required for DNA binding (Fig. 5a and c). Overall, the number of immune response pathways triggered by the disordered region of NS1-2 from both HuNoV and MNV warrants further study in the context of virus infection.
Comparison of HuNoV NS1-2 with MNV NS1-2 and correlation to MNV infection
The HuNoV NS1-2 transcriptomic profile was compared to MNV NS1-2 transfected cells, and then overall to MNV infected cells. Figure 6 shows these up- and down-regulated genes classified into Kegg pathways. A closer look at the shared pathways shows changes in intracellular signalling molecules such as MAPK, and proteins that activate key immune responses, such as cytokines and chemokines. These DE genes and their fold changes are shown in Table 3. The genes present in MNV NS1-2 transfected cells followed similar regulation patterns to HuNoV NS1-2. In each case, the genes upregulated in HuNoV NS1-2 were also upregulated in MNV NS1-2 and consequently in MNV infected cells, showing a strong correlation between transfection of virus protein and whole virus infection in these specific pathways in monocytes.
The combination of chemokine and cytokine mRNA that is upregulated in MNV infected cells suggests a Th1 profile, and this is further supported by down-regulation of genes such as IL10ra and CSF3R (G-CSF receptor)  that support an anti-inflammatory phenotype (Table 3). Overall, the transcriptomic profile suggests that MNV infected cells are pro-apoptotic, and affect MAPK, NFκB, and PI3K-Akt intracellular signalling pathways. The genes outlined in metabolic pathways affect the fatty acid and arachidonic acid regulation, with enzymatic activities such as oxidoreductase and transferase functions (Table 3). The proteins encoded by genes affected by MNV infection are localised at the endoplasmic reticulum and mitochondria. MNV NS1-2 expression induces a similar trend in intracellular signalling and metabolic pathways, apoptosis, and immune responses as MNV-infected cells, indicating that NS1-2 protein is a contributing factor to this phenotype, as these changes are not seen in mock-transfected or untreated monocytes. This same trend in all the pathways is seen with cells expressing HuNoV NS1-2 (Table 3), suggesting a similar role as MNV NS1-2 during virus infection. Previous work has shown that downregulation of survivin and upregulation of TNF and traf1 contributes to apoptosis during MNV infection . The TNFα and Traf1 upregulation was also observed in this study, both in MNV infected and in NS1-2 transfected cells (Table 3). The chemokines secreted during an in vitro MNV infection correlate to a Th1 phenotype, and this has been previously shown by microarray analysis for mRNA and ELISA assays to detect secreted chemokines . There is also an upregulation of serum TNFα and IFNβ , and an increase in inflammatory dendritic cells in the intestines of mice , during an MNV infection that further supports a Th1 phenotype.
The DE genes in the TLR pathway in this study indicate a moderate decrease in TLR4, TLR7, and TLR9 and a strong decrease in TLR8 mRNA in HuNoV NS1-2 transfected and MNV-infected cells. The changes in MNV NS1-2 transfected cells were not statistically significant (Table 3). The role of TLR regulation during norovirus infections is currently unknown, though the presence of viral RNA is known to upregulate intracellular TLR7/8 and TLR9 . Previous studies have shown that there is good correlation between the mRNA and protein levels of TLRs, hence decreased mRNA levels indicate downregulation of the expressed TLR proteins . To analyse this further, intracellular expression of TLR7 and TLR8 was analysed using flow cytometry in NS1-2-transfected cells and MNV-infected monocytes at the same time point as transcriptomic analysis. Figure 7a shows that expression of TLR7 does not change significantly in NS1-2 transfected or MNV-infected cells when compared to mock-transfected and untreated cells. However, expression of TLR8 (Fig. 7b) is decreased by 40% (HuNoV NS1-2), 35% (MNV NS1-2), and 37% (MNV infected) when compared to control cells. Interactions between TLR and single-stranded RNA viruses are not completely understood. Generally, TLR7/8 expression is increased upon recognition of viral single-stranded RNA, as shown for human parechovirus . Some RNA viruses can modulate TLR expression either via direct binding to TLR or via modulating downstream effectors . Hepatitis C virus encodes a non-structural disordered protein, NS5A which impairs TLR2 signalling by targeting MyD88 . Studies with HIV-positive patients showed that the mRNA expression of TLR7/8 decreased during disease progression, and that activation of the TLR7/8 receptors led to suppression of HIV replication in monocytes . In T cells however, HIV causes an upregulation of TLR7 resulting in T-cell anergy . The consequences of down regulating TLR8 appear to be cell-specific. In mice, decreased TLR8 expression leads to an increase in TLR7 in dendritic cells but not in monocytes .
This study undertook transcriptomic analysis of cells transfected with HuNoV NS1-2 to identify the cellular pathways affected by the virus protein. Our data indicates that the HuNoV NS1-2 protein targets multiple pathways in murine cells. The intracellular pathways include Jak-STAT, MAPK, p53, PI3K-Akt signaling, and the immune processes affected are apoptosis, chemokine and cytokine secretion, and TLR pathways. This phenotype suggests that HuNoV NS1-2 has a role in regulation of innate immunity, in particular affecting intracellular signaling pathways in response to cell surface receptor expression. The disordered region of HuNoV NS1-2 protein is predicted to be immunogenic and upon protein expression caused an upregulation of genes belonging to MHC-I, IFN, and T-cell mediated immunity pathways. Comparison of transfected HuNoV NS1-2 cells with MNV NS1-2 expressing cells showed a similar transcriptomic profile. Evaluation of the transcriptomic profile of MNV-infected monocytes correlated well with previous studies showing that MNV affects apoptosis and cytokine/chemokine secretion in monocytes. The RNAseq data indicates that NS1-2 protein may be responsible for these cellular immune functions. The role of TLR7/8 expression in MNV infection has not been previously reported, and our data shows that TLR8 expression in MNV infection is decreased at 12hpi, with no discernable change in TLR7 expression. The TLR7/8 profile is also present in NS1-2 transfected cells, showing a role for NS1-2 in modulating TLR signaling during infection. This study is the first to report the multiple pathways targeted by NS1-2 and identifies key areas that future research can focus on. In particular, the putative enzymatic function of NS1-2 that may be responsible for affecting multiple pathways needs to be determined.
Enzyme-linked immunosorbent assay
Kyoto encyclopedia of genes and genomes
Lecithin retinol acyltransferase
Mitogen-activated protein kinase
Major histocompatibility complex
Nuclear factor-kappa light chain chain enhancer of activated B cells
Protein analysis through evolutionary relationships
Tumor necrosis factor
Ahmed SM, Hall AJ, Robinson AE, Verhoef L, Premkumar P, Parashar UD, Koopmans M, Lopman BA. Global prevalence of norovirus in cases of gastroenteritis: a systematic review and meta-analysis. Lancet Infect Dis. 2014;14(8):725–30.
Hall AJ, Lopman BA, Payne DC, Patel MM, Gastanaduy PA, Vinje J, Parashar UD. Norovirus disease in the United States. Emerg Infect Dis. 2013;19(8):1198–205.
Kambhampati A, Koopmans M, Lopman BA. Burden of norovirus in healthcare facilities and strategies for outbreak control. J Hosp Infect. 2015;89(4):296–301.
Eden JS, Tanaka MM, Boni MF, Rawlinson WD, White PA. Recombination within the pandemic norovirus GII.4 lineage. J Virol. 2013;87(11):6270–82.
Debbink K, Lindesmith LC, Donaldson EF, Costantini V, Beltramello M, Corti D, Swanstrom J, Lanzavecchia A, Vinje J, Baric RS. Emergence of new pandemic GII.4 Sydney norovirus strain correlates with escape from herd immunity. J Infect Dis. 2013;208(11):1877–87.
Debbink K, Donaldson EF, Lindesmith LC, Baric RS. Genetic mapping of a highly variable norovirus GII.4 blockade epitope: potential role in escape from human herd immunity. J Virol. 2012;86(2):1214–26.
McFadden N, Bailey D, Carrara G, Benson A, Chaudhry Y, Shortland A, Heeney J, Yarovinsky F, Simmonds P, Macdonald A, et al. Norovirus regulation of the innate immune response and apoptosis occurs via the product of the alternative open reading frame 4. PLoS Pathog. 2011;7(12):e1002413.
Karst SM, Zhu S, Goodfellow IG. The molecular pathology of noroviruses. J Pathol. 2015;235(2):206–16.
Baker ES, Luckner SR, Krause KL, Lambden PR, Clarke IN, Ward VK. Inherent structural disorder and dimerisation of murine norovirus NS1-2 protein. PLoS One. 2012;7(2):e30534.
Sosnovtsev SV, Belliot G, Chang KO, Prikhodko VG, Thackray LB, Wobus CE, Karst SM, Virgin HW, Green KY. Cleavage map and proteolytic processing of the murine norovirus nonstructural polyprotein in infected cells. J Virol. 2006;80(16):7816–31.
Anantharaman V, Aravind L. Evolutionary history, structural features and biochemical diversity of the NlpC/P60 superfamily of enzymes. Genome Biol. 2003;4(2):R11.
Xu Q, Rawlings ND, Chiu HJ, Jaroszewski L, Klock HE, Knuth MW, Miller MD, Elsliger MA, Deacon AM, Godzik A, et al. Structural analysis of papain-like NlpC/P60 superfamily enzymes with a circularly permuted topology reveals potential lipid binding sites. PLoS One. 2011;6(7):e22013.
Ettayebi K, Hardy ME. Norwalk virus nonstructural protein p48 forms a complex with the SNARE regulator VAP-A and prevents cell surface expression of vesicular stomatitis virus G protein. J Virol. 2003;77(21):11790–7.
Fernandez-Vega V, Sosnovtsev SV, Belliot G, King AD, Mitra T, Gorbalenya A, Green KY. Norwalk virus N-terminal nonstructural protein is associated with disassembly of the Golgi complex in transfected cells. J Virol. 2004;78(9):4827–37.
Salim O, Clarke IN, Lambden PR. Functional analysis of the 5′ genomic sequence of a bovine norovirus. PLoS One. 2008;3(5):e2169.
Hyde JL, Sosnovtsev SV, Green KY, Wobus C, Virgin HW, Mackenzie JM. Mouse norovirus replication is associated with virus-induced vesicle clusters originating from membranes derived from the secretory pathway. J Virol. 2009;83(19):9709–19.
Hyde JL, Gillespie LK, Mackenzie JM. Mouse norovirus 1 utilizes the cytoskeleton network to establish localization of the replication complex proximal to the microtubule organizing center. J Virol. 2012;86(8):4110–22.
Nice TJ, Strong DW, McCune BT, Pohl CS, Virgin HW. A single amino acid change in murine norovirus NS1/2 is sufficient for colonic tropism and persistence. J Virol. 2012;87(1):327–34.
Jones MK, Watanabe M, Zhu S, Graves CL, Keyes LR, Grau KR, Gonzalez-Hernandez MB, Iovine NM, Wobus CE, Vinje J, et al. Enteric bacteria promote human and mouse norovirus infection of B cells. Science. 2014;346(6210):755–9.
Ettayebi K, Crawford SE, Murakami K, Broughman JR, Karandikar U, Tenge VR, Neill FH, Blutt SE, Zeng XL, Qu L, et al. Replication of human noroviruses in stem cell-derived human enteroids. Science. 2016;353(6306):1387–93.
Waugh E, Chen A, Baird MA, Brown CM, Ward VK. Characterization of the chemokine response of RAW264.7 cells to infection by murine norovirus. Virus Res. 2014;181:27–34.
Zhu S, Regev D, Watanabe M, Hickman D, Moussatche N, Jesus DM, Kahan SM, Napthine S, Brierley I, Hunter 3rd RN, et al. Identification of immune and viral correlates of norovirus protective immunity through comparative study of intra-cluster norovirus strains. PLoS Pathog. 2013;9(9):e1003592.
Ingersoll MA, Spanbroek R, Lottaz C, Gautier EL, Frankenberger M, Hoffmann R, Lang R, Haniffa M, Collin M, Tacke F, et al. Comparison of gene expression profiles between human and mouse monocyte subsets. Blood. 2010;115(3):e10–9.
Yang J, Zhang L, Yu C, Yang XF, Wang H. Monocyte and macrophage differentiation: circulation inflammatory monocyte as biomarker for inflammatory diseases. Biomark Res. 2014;2(1):1.
Wobus CE, Thackray LB, Virgin HW. Murine norovirus: a model system to study norovirus biology and pathogenesis. J Virol. 2006;80(11):5104–12.
Perry JW, Taube S, Wobus CE. Murine norovirus-1 entry into permissive macrophages and dendritic cells is pH-independent. Virus Res. 2009;143(1):125–9.
Ward VK, McCormick CJ, Clarke IN, Salim O, Wobus CE, Thackray LB, Virgin HW, Lambden PR. Recovery of infectious murine norovirus using pol II-driven expression of full-length cDNA. Proc Natl Acad Sci U S A. 2007;104(26):11050–5.
Davies C, Brown CM, Westphal D, Ward JM, Ward VK. Murine norovirus replication induces G0/G1 cell cycle arrest in asynchronously growing cells. J Virol. 2015;89(11):6057–66.
Cox MP, Peterson DA, Biggs PJ. SolexaQA: At-a-glance quality assessment of Illumina second-generation sequencing data. BMC Bioinformatics. 2010;11:485.
Trapnell C, Pachter L, Salzberg SL. TopHat: discovering splice junctions with RNA-Seq. Bioinformatics. 2009;25(9):1105–11.
Langmead B, Salzberg SL. Fast gapped-read alignment with Bowtie 2. Nat Methods. 2012;9(4):357–9.
Quinlan AR, Hall IM. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics. 2010;26(6):841–2.
Robinson MD, Oshlack A. A scaling normalization method for differential expression analysis of RNA-seq data. Genome Biol. 2010;11(3):R25.
Dillies MA, Rau A, Aubert J, Hennequet-Antier C, Jeanmougin M, Servant N, Keime C, Marot G, Castel D, Estelle J, et al. A comprehensive evaluation of normalization methods for Illumina high-throughput RNA sequencing data analysis. Brief Bioinform. 2013;14(6):671–83.
Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32(5):1792–7.
Talavera G, Castresana J. Improvement of phylogenies after removing divergent and ambiguously aligned blocks from protein sequence alignments. Syst Biol. 2007;56(4):564–77.
Huelsenbeck JP, Ronquist F. MRBAYES: Bayesian inference of phylogenetic trees. Bioinformatics. 2001;17(8):754–5.
Dereeper A, Guignon V, Blanc G, Audic S, Buffet S, Chevenet F, Dufayard JF, Guindon S, Lefort V, Lescot M, et al. Phylogeny.fr: robust phylogenetic analysis for the non-specialist. Nucleic Acids Res. 2008;36(Web Server issue):W465–9.
Wang M, Zhao XM, Tan H, Akutsu T, Whisstock JC, Song J. Cascleave 2.0, a new approach for predicting caspase and granzyme cleavage targets. Bioinformatics. 2014;30(1):71–80.
Bliven S, Prlic A. Circular permutation in proteins. PLoS Comput Biol. 2012;8(3):e1002445.
Aramini JM, Rossi P, Huang YJ, Zhao L, Jiang M, Maglaqui M, Xiao R, Locke J, Nair R, Rost B, et al. Solution NMR structure of the NlpC/P60 domain of lipoprotein Spr from Escherichia coli: structural evidence for a novel cysteine peptidase catalytic triad. Biochemistry. 2008;47(37):9715–7.
Ren X, Lin J, Jin C, Xia B. Solution structure of the N-terminal catalytic domain of human H-REV107—a novel circular permutated NlpC/P60 domain. FEBS Lett. 2010;584(19):4222–6.
Senkevich TG, Wyatt LS, Weisberg AS, Koonin EV, Moss B. A conserved poxvirus NlpC/P60 superfamily protein contributes to vaccinia virus virulence in mice but not to replication in cell culture. Virology. 2008;374(2):506–14.
Bannantine JP, Lingle CK, Adam PR, Ramyar KX, McWhorter WJ, Stabel JR, Picking WD, Geisbrecht BV. NlpC/P60 domain-containing proteins of Mycobacterium avium subspecies paratuberculosis that differentially bind and hydrolyze peptidoglycan. Protein Sci. 2016;25(4):840–51.
Xue L, Rando RR. Roles of cysteine 161 and tyrosine 154 in the lecithin-retinol acyltransferase mechanism. Biochemistry. 2004;43(20):6120–6.
Tsai FM, Shyu RY, Lin SC, Wu CC, Jiang SY. Induction of apoptosis by the retinoid inducible growth regulator RIG1 depends on the NC motif in HtTA cervical cancer cells. BMC Cell Biol. 2009;10:15.
Herod MR, Salim O, Skilton RJ, Prince CA, Ward VK, Lambden PR, Clarke IN. Expression of the murine norovirus (MNV) ORF1 polyprotein is sufficient to induce apoptosis in a virus-free cell model. PLoS One. 2014;9(3):e90679.
Li X, Romero P, Rani M, Dunker AK, Obradovic Z. Predicting Protein Disorder for N-, C-, and Internal Regions. Genome Inform Ser Workshop Genome Inform. 1999;10:30–40.
Sigrist CJ, de Castro E, Cerutti L, Cuche BA, Hulo N, Bridge A, Bougueleret L, Xenarios I. New and continuing developments at PROSITE. Nucleic Acids Res. 2013;41(Database issue):D344–7.
Vita R, Overton JA, Greenbaum JA, Ponomarenko J, Clark JD, Cantrell JR, Wheeler DK, Gabbard JL, Hix D, Sette A, et al. The immune epitope database (IEDB) 3.0. Nucleic Acids Res. 2015;43(Database issue):D405–12.
Iakoucheva LM, Radivojac P, Brown CJ, O’Connor TR, Sikes JG, Obradovic Z, Dunker AK. The importance of intrinsic disorder for protein phosphorylation. Nucleic Acids Res. 2004;32(3):1037–49.
Yaffe MB, Elia AE. Phosphoserine/threonine-binding domains. Curr Opin Cell Biol. 2001;13(2):131–8.
Cohen P. The regulation of protein function by multisite phosphorylation—a 25 year update. Trends Biochem Sci. 2000;25(12):596–601.
Bretana NA, Lu CT, Chiang CY, Su MG, Huang KY, Lee TY, Weng SL. Identifying protein phosphorylation sites with kinase substrate specificity on human viruses. PLoS One. 2012;7(7):e40694.
Giroud C, Chazal N, Briant L. Cellular kinases incorporated into HIV-1 particles: passive or active passengers? Retrovirology. 2011;8:71.
Cordek DG, Croom-Perez TJ, Hwang J, Hargittai MR, Subba-Reddy CV, Han Q, Lodeiro MF, Ning G, McCrory TS, Arnold JJ, et al. Expanding the proteome of an RNA virus by phosphorylation of an intrinsically disordered viral protein. J Biol Chem. 2014;289(35):24397–416.
Huang DW, Sherman BT, Lempicki RA. Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nat Protoc. 2009;4(1):44–57.
Mi H, Muruganujan A, Thomas PD. PANTHER in 2013: modeling the evolution of gene function, and other gene attributes, in the context of phylogenetic trees. Nucleic Acids Res. 2013;41(Database issue):D377–86.
Chowdhury S, Sarkar RR. Comparison of human cell signaling pathway databases--evolution, drawbacks and challenges. Database (Oxford). 2015;2015:bau126.
Hemmings BA, Restuccia DF. PI3K-PKB/Akt pathway. Cold Spring Harb Perspect Biol. 2012;4(9):a011189.
Fentress SJ, Behnke MS, Dunay IR, Mashayekhi M, Rommereim LM, Fox BA, Bzik DJ, Taylor GA, Turk BE, Lichti CF, et al. Phosphorylation of immunity-related GTPases by a Toxoplasma gondii-secreted kinase promotes macrophage survival and virulence. Cell Host Microbe. 2010;8(6):484–95.
Hsu TH, Jiang SY, Chang WL, Eckert RL, Scharadin TM, Chang TC. Involvement of RARRES3 in the regulation of Wnt proteins acylation and signaling activities in human breast cancer cells. Cell Death Differ. 2015;22(5):801–14.
Franceschini A, Szklarczyk D, Frankild S, Kuhn M, Simonovic M, Roth A, Lin J, Minguez P, Bork P, von Mering C, et al. STRING v9.1: protein-protein interaction networks, with increased coverage and integration. Nucleic Acids Res. 2013;41(Database issue):D808–15.
van Zuylen WJ, Garceau V, Idris A, Schroder K, Irvine KM, Lattin JE, Ovchinnikov DA, Perkins AC, Cook AD, Hamilton JA, et al. Macrophage activation and differentiation signals regulate schlafen-4 gene expression: evidence for Schlafen-4 as a modulator of myelopoiesis. PLoS One. 2011;6(1):e15723.
Coccia EM, Del Russo N, Stellacci E, Testa U, Marziali G, Battistini A. STAT1 activation during monocyte to macrophage maturation: role of adhesion molecules. Int Immunol. 1999;11(7):1075–83.
Dekkers PE, Juffermans NP, Hove T, de Jonge E, van Deventer SJ, van Der Poll T. Granulocyte colony-stimulating factor receptors on granulocytes are down-regulated after endotoxin administration to healthy humans. J Infect Dis. 2000;181(6):2067–70.
Bok K, Prikhodko VG, Green KY, Sosnovtsev SV. Apoptosis in murine norovirus-infected RAW264.7 cells is associated with downregulation of survivin. J Virol. 2009;83(8):3647–56.
Chen X, Leach D, Hunter DA, Sanfelippo D, Buell EJ, Zemple SJ, Grayson MH. Characterization of intestinal dendritic cells in murine norovirus infection. Open Immunol J. 2011;4:22–30.
Xagorari A, Chlichlia K. Toll-like receptors and viruses: induction of innate antiviral immune responses. Open Microbiol J. 2008;2:49–59.
Abdi J, Mutis T, Garssen J, Redegeld F. Characterization of the Toll-like receptor expression profile in human multiple myeloma cells. PLoS One. 2013;8(4):e60671.
Triantafilou K, Vakakis E, Orthopoulos G, Ahmed MA, Schumann C, Lepper PM, Triantafilou M. TLR8 and TLR7 are involved in the host’s immune response to human parechovirus 1. Eur J Immunol. 2005;35(8):2416–23.
Nian H, Geng WQ, Cui HL, Bao MJ, Zhang ZN, Zhang M, Pan Y, Hu QH, Shang H. R-848 triggers the expression of TLR7/8 and suppresses HIV replication in monocytes. BMC Infect Dis. 2012;12:5.
Dominguez-Villar M, Gautron AS, de Marcken M, Keller MJ, Hafler DA. TLR7 induces anergy in human CD4(+) T cells. Nat Immunol. 2015;16(1):118–28.
Demaria O, Pagni PP, Traub S, de Gassart A, Branzk N, Murphy AJ, Valenzuela DM, Yancopoulos GD, Flavell RA, Alexopoulou L. TLR8 deficiency leads to autoimmunity in mice. J Clin Invest. 2010;120(10):3651–62.
ZL was funded by a Career Development award (12-057) from the Health Research Council of New Zealand (HRC). HRC had no role in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.
Availability of data and materials
The datasets analysed during the current study available from the corresponding author on reasonable request.
ZL performed the experiments for RNAseq assays, analysed the transcriptomic data, and wrote the manuscript. GG analysed the RNAseq data using EdgeR package. ESB designed the MNV constructs and optimized the RNA transfection protocols. VKW was involved in the design of the study, data analysis, and manuscript writing. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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