- Research article
- Open Access
De novo assembly and transcriptome analysis of Atlantic salmon macrophage/dendritic-like TO cells following type I IFN treatment and Salmonid alphavirus subtype-3 infection
BMC Genomics volume 16, Article number: 96 (2015)
Interferons (IFN) are cytokines secreted by vertebrate cells involved in activation of signaling pathways that direct the synthesis of antiviral genes. To gain a global understanding of antiviral genes induced by type I IFNs in salmonids, we used RNA-seq to characterize the transcriptomic changes induced by type I IFN treatment and salmon alphavirus subtype 3 (SAV-3) infection in TO-cells, a macrophage/dendritic like cell-line derived from Atlantic salmon (Salmo salar L) head kidney leukocytes.
More than 23 million reads generated by RNA-seq were de novo assembled into 58098 unigenes used to generate a total of 3149 and 23289 differentially expressed genes (DEGs) from TO-cells exposed to type I IFN treatment and SAV-3 infection, respectively. Although the DEGs were classified into genes associated with biological processes, cellular components and molecular function based on gene ontology classification, transcriptomic changes reported here show upregulation of genes belonging to the canonical type I IFN signaling pathways together with a broad spectrum of antiviral genes that block virus replication in host cells. In addition, the transcriptome shows a profile of genes associated with apoptosis as well as genes that activate adaptive immunity. Further, our findings show that the profile of genes expressed by TO-cells is comparable to orthologous genes expressed by mammalian macrophages and dendritic cells in response to type I IFNs. Twenty DEGs randomly selected for qRT-PCR confirmed the validity of the transcriptomic changes detected by RNA-seq by showing that the genes upregulated by RNA-seq were also upregulated by qRT-PCR and that genes downregulated by RNA-seq were also downregulated by qRT-PCR.
The de novo assembled transcriptome presented here provides a global description of genes induced by type I IFNs in TO-cells that could serve as a repository for future studies in fish cells. Transcriptome analysis shows that a large proportion of IFN genes expressed in this study are comparable to IFNs genes expressed in mammalia. In addition, the study shows that SAV-3 is a potent inducer of type I IFNs and that the responses it induces in TO-cells could serve as a model for studying IFN responses in salmonids.
Salmonid alphavirus (SAV) causes pancreas disease (PD) in Atlantic salmon (Salmo salar L) and rainbow trout (Oncorhynchus mykiss) characterized by necrosis of the exocrine pancreas, cardiomyopathy and skeletal myopathy . It was first reported in 1984  and later characterized as a member of the family Togaviridae . Salmonid alphavirus has a positive sense, ssRNA genome which is approximately 12 kb . The genome is a capped and polyadenylated positive strand RNA made of two open reading frames (ORFs) that encode structural and nonstructural proteins. Non-structural proteins are encoded by the 5′ end while structural proteins that form the envelope glycoproteins and the capsid are coded by the 3′ end . Our previous studies have shown that type I interferon (IFN) inhibits the replication of SAV-3 in TO-cells  which has stimulated further interest to elucidate the transcriptomic changes induced by type I IFNs in salmonids.
Antiviral responses generated in response to viral infection are essential for the survival of the host. However, the assembly of an antiviral response starts at cellular level during which programmed intrinsic cell responses are initiated in a process termed ‘cell-autonomous immunity’ . Chief among responses that remodel the cell’s transcriptome in response to infection is the IFN cytokine family. These cytokines induce pleiotropic biological effects by producing profiles of gene repertoires that serve as powerful signals for marshalling host defenses against microbial invasion in host cells. As pointed out by MacMicking , IFNs induce the expression of a broad spectrum of genes as part of an antimicrobial program designed to combat infection in all nucleated cells. Although named after their ability to interfere with virus replication in treated cells, IFNs have immunodulatory, cell differentiative, anti-angiogenic and anti-proliferative effects on cells . In higher vertebrates, examination of recently identified IFN inducible genes (ISGs) using a systems biology approach reveal a highly diverse but integrated host defense program dedicated at protecting the interior of a vertebrate cell [7,9]. While these studies have opened new insights on the role of type I IFN responses in protecting mammalian cells against viral infections, studies in teleosts fish are still in their early stages and as such little is known on protective mechanisms of different ISGs on fish cells. Hence, to gain a global insight on type I IFN pathway related genes expressed in fish cells, we used a RNA-seq to analyze the transcriptomic changes induced by type I IFN and SAV-3 infection in TO-cells. In this study we wanted to find out whether TO-cells, a continuous cell line originating from Atlantic salmon (Salmo salar L) headkidney cells characterized to possess dendritic/macrophage like properties, would express the same profile of genes as those generated from mammalian phagocytic cells. By comparing the profile of ISGs generated from type I IFN treated cells with SAV-3 infected cells, we wanted to find out whether SAV-3 infection would produce the same profile of genes comparable to those produced by type I IFN treatment in TO-cells. The transcriptome presented herein shows that type I IFN induces the expression of a broad spectrum of ISGs and that SAV-3 is a potent inducer of type I IFN responses in TO-cells.
Cell culture, virus infection and IFN treatment
TO-cells originating from Atlantic salmon (Salmo salar L) head kidney leukocytes characterized to possess macrophage/dendritic-like properties [10,11], were propagated at 20°C in HMEM (Eagle’s minimal essential medium [MEM] with Hanks’ balanced salt solution [BSS]) supplemented with L-glutamine, MEM nonessential amino acids, gentamicin sulfate, and 10% FBS. The virus used to inoculate the TO-cells has previously been described  and characterized by sequencing to be salmonid alphavirus subtype 3 (SAV-3) (Genebank accession JQ799139). One batch of TO-cells was treated with 500 ng/ml of Atlantic salmon recombinant Type I in triplicates and another was infected with SAV-3 at MOI 1 when the cells were 80% confluent. Thereafter, both the type I IFN treated and SAV-3 infected cells were incubated at 15°C in maintenance media using HMEM growth media supplemented with 2% FBS. The mock group was only treated with maintenance media. After 48 hours when the cells were confluent, they were harvested and used for RNA extraction to test for type I IFN responses. All studies in TO-cells were carried out in triplicates. The recombinant type I IFN used in this study was made in our laboratory as previously described by Xu et al. .
Total RNA was isolated using the RNeasy mini Kit (Qiagen, Hilden, Germany) with on-column DNase treatment according to the manufacturer’s instructions. The concentration and the quality of RNA were analyzed using a Nanodrop ND1000 (Nanodrop Technologies, Wilmington, USA) and Agilent 2100 Bioanalyzer (Agilent Technologies, USA).
Library construction, sequencing and data analysis for RNA-Seq
Equal quantities of total RNA from triplicates of the type I IFN treated, SAV-3 infected and mock-TO-cells were mixed to prepare the pooled RNA sample for RNA-Seq. Total RNA samples were treated with DNase I to degrade any possible DNA contamination. Then the mRNA was enriched using oligo(dT) magnetic beads. The mRNA was fragmented into short fragments (about 200 bp) by mixing with the fragmentation buffer. Thereafter, the first strand of cDNA was synthesized using random hexamer-primer. A buffer containing dNTPs, RNase H and DNA polymerase I was added to synthesize the second strand. The double strand cDNA was purified with magnetic beads. End reparation and 3′-end single nucleotide A (adenine) addition was then performed. Finally, sequencing adaptors were ligated to the fragments and the fragments were enriched by PCR amplification. During quality check (QC step), Agilent 2100 Bioanaylzer and ABI StepOnePlus Real-Time PCR System (Biorad.com) were used to qualify and quantify the sample library. Thereafter, library products were ready for RNA-sequencing using Illumina HiSeqTM 2000, BGI-Hong Kong. Clean reads were obtained after removal of adaptor sequences, and removal of reads having greater than 10% of unknown bases as well as removal of reads with low quality bases (base with quality value ≤ 5) greater than 50% in a read.
Functional annotation and gene ontology classification
Once a library of clean reads was prepared, the reads were then used for transcriptome de novo assembly using the Trinity progam (http://trinityrnaseq.sourceforge.net/). Thereafter, assembled unigenes were used for annotation so that they could be classified for gene functioning by searching different protein databases. To do this, we used BlastX (version 2.2.23) alignment against four public protein databases; NCBI non-redundant (NR), Swiss-Prot, Kyoto Encyclopedia of Genes and Genomes (KEGG) and Cluster of Orthologous Groups (COG) at e-value < 0.00001. The best alignments from the four databases were used to determine the direction of the unigenes. As for conflicting results between the different databases, the priority order NR, Swissprot, KEGG and COG was used. Data obtained from BlastX was used to extract the coding regions (CDS) from unigene sequences and translate them into peptide sequences. Unigenes with no hits in BlastX were analyzed using ESTScan to predict their CDS and to decide their sequence direction. Unigenes with NR annotation were further analyzed with Blast2go (http://www.blast2go.org/) to obtain their gene ontology (GO) annotations, and were then further classified according to GO functions using the Web Gene Ontology (WEGO) annotation software.
Identification of differentially expressed genes
The mapped read counts for each gene were normalized for RNA length and for the total read number in each lane using the reads per kilobase per million (RPKM) method, which facilitates comparison of the number of transcript levels generated between samples. The cutoff value for determining gene transcriptional activity was based on 95% confidence interval for all RPKM values for each gene. We used a rigorous algorithm to identify differentially expressed genes (DEGs) based on comparing the exposed with unexposed group to generate the DEGs. In this study, DEGs were generated based on comparing the RPKM mapped reads from type I IFN treated cells (IFN) versus mock TO-cells (TO), designated asTO-VS-IFN, while the second comparison was based on SAV-3 infected cells (SAV3) versus mock TO-cells (TO), designated as TO-VS-SAV3. Genes with a threshold of false discovery rate (FDR) <0.001 and an absolute value log2ratio > 1 were considered differentially expressed. All identified DEGs were mapped to GO annotations using the Blast2GO software (http://www.blast2go.org/).
Validation of RNA-Seq data
To confirm the differential expression of genes revealed by RNA-Seq, 12 genes identified to be co-upregulated and 8 genes identified to be co-downregulated in TO-VS-IFN and TO-VS-SAV3 were randomly chosen for qRT-PCR validation.
qRT-PCR was performed by using the QuantiFast SYBR Green RT-PCR Kit (Qiagen) and the LightCycler 480 system (Roche). For each gene, 100 ng total RNA was used as a template in a mixture of specific primers (10 μM) (Table 1) and Master Mix in a final volume of 25 μl following manufacture’s instruction. The mixtures were first incubated for reverse transcription at 50°C for 10 min and subsequently for PCR initial activation at 95°C for 5 min, followed by 40 amplification cycles (10 s at 95°C and 30 s at 60°C). The specificity of the PCR products from each primer pair was confirmed by melting-curve analysis and agarose gel electrophoresis. The 2–[delta][delta]Ct method was used to calculate the fold increase in gene expression relative to the control group. All quantifications were normalized to β-actin (endogenous gene).
We constructed three libraries comprising of the type I IFN treatment (IFN), SAV3 infection and mock group of TO-cells only (TO) from RNA-seq data that yielded a total of 23,113,874, 24,608,338 and 23,421,631 clean reads, respectively. A summary of the number of reads and the composition of reads generated from the RNA-seq data is shown in Table 2 while steps taken to assemble the transcriptome from clean reads are shown in Figure 1. After filtration, the percentage of clean reads in each library ranged from 97.22% to 98.23% (Figure 2). Of the total reads, genes that match to unique reads accounted for 71.31%, 78.48% and 69.27% for the IFN, SAV3 and TO groups (Table 2), respectively.
Identification of differentially expressed genes
Using the Trinity program, we detected a total of 58,098 unigenes from the clean reads established above. Thereafter, unigenes were screened using the criteria FDR ≤0.001 and |log2Ratio| ≥1 to identify the DEGs. Based on this approach a total of 3,149 and 23,289 DEGs were identified from the comparisons of TO-VS-IFN and TO-VS-SAV3, respectively (Figure 3). For the TO-VS-IFN, 2156 DEGs were upregulated (3.7%) and 993 DEGs were downregulated (1.7%) whereas the TO-VS-SAV3 produced 1030 up-regulated DEGs (1.8%) and 22,259 down-regulated DEGs (38.3%).
Gene ontology analysis of DEGs
Venn diagram analysis identified 956 co-upregulated (Figure 4B) and 734 co-downregulated (Figure 4A) DEGs in TO-VS-IFN and TO-VS-SAV3 while 36 DEGs were downregulated in the TO-VS-SAV3 and upregulated in the TO-VS-IFN (Figure 4C). Based on gene ontology (GO) classification, 21, 14 and 10 functional groups were identified and classified as biological process, cellular component and molecular function, for the co-upregulated DEGs (Figure 5A), respectively. Similarly, 21, 15 and 13 functional groups were identified and classified as biological processes, cellular component and molecular function for the co-downregulated DEGs, respectively (Figure 5B). Generally, unigenes linked to biological regulation, cellular process, response to stimuli, signaling, single organism processes, cell and cell part, binding and catalytic activity were highly expressed both in the co-upregulated (Figure 5A) and co-downregulated groups (Figure 5B). However, the major difference between the co-upregulated and co-downregulated groups is that cell-killing unigenes classified under biological processes were only expressed in the co-upregulated and not the co-downregulated unigenes while antioxidant and structural molecule activity unigenes classified under molecular functions were only expressed in the co-downregulated and not the co-upregulated DEGs (Figure 5A and B). Further, Figure 5C shows GO classification of genes down-regulated in response to SAV-3 (TO-VS-SAV3) only in which 23, 16 and 12 functional groups were differentially expressed. The major differences between the three groups (Figure 5A, B and C) are that the biological adhesion, extracellular matrix part, channel regulator activity and structural molecule activity functional groups were only differentially expressed in the co-downregulated unigenes (Figure 5B) and the “TO-VS-SAV3 downregulated unigenes only” (Figure 5C) while the nucleoid and rhythmic process functional groups were only differentially expressed in the group downregulated by SAV-3 infection (Figure 5C). The cell killing functional group was higher in the co-upregulated unigenes (Figure 5A), less expressed in the group downregulated unigenes by SAV-3 infection only (Figure 5C) and absent in the co-downregulated unigenes (Figure 5B).
The X-axis shows the classification of unigenes in GO terms while the Y-axis shows the number of matched unigenes. Both the co-upregulated and co-downregulated unigenes were classified into biological process (blue), cellular components (red) and molecular function (green) (A and B). For the co-upregulated unigenes (A), biological process, cellular components and molecular functions accounted for 21, 14 and 10 functional groups while for the co-downregulated unigenes (B), biological process, cellular components and molecular functions accounted for 21, 15 and 13 functional groups. Comparing the co-upregulated (A) and the co-downregulated (B) unigenes shows that the cell-killing unigenes classified under biological process (blue) shown in asterisk (*) were only expressed in the co-upregulated group (A) while antioxidants and structural molecule activity unigenes classified under molecule function (green) (marked as ¤) were only expressed in the co-downregulated group. C shows GO classification of unigenes that were only downregulated in response to SAV-3 infection only of which the biological process, cellular components and molecular functions accounted for 23, 16 and 18 functional groups, respectively. Although the molecular function group showed 18 functional groups only 12 were differentially expressed (C). The major differences among the three groups (A, B and C) are that biological adhesion, extracellular matrix part, channel regulator activity and structural molecule activity functional groups (marked as †) were only differentially expressed in the co-downregulated unigenes (B) and the TO-VS-SAV3 downregulated unigenes only (C) while the nucleoid and rhythmic process functions (marked as ¥) were only expressed in the group downregulated by SAV-3 infection (C). The cell killing (marked as §) functional group was less expressed in C, absent in B and higher in A and finally the antioxidant activity (marked as #) functional group was only expressed in B.
RNA-seq transcriptome profiling of type I IFN and SAV-3 induced genes
After identifying the 956 co-upregulated (Figure 4B) and 734 co-downregulated genes (Figure 4A) in the TO-VS-IFN and TO-VS-SAV3 together with the differentially regulated genes (36 DEGs) of the TO-VS-IFN versus TO-VS-SAV3 shown in Figure 4C, we manually narrowed the scope of DEGs to 60 genes induced by type I IFNs in both the TO-VS-IFN and TO-VS-SAV3 groups in order to gain a comprehensive understanding of the transcriptomic changes induced by type I IFN treatment and SAV-3 infection in TO-cells from the 60 selected genes obtained from the entire transcriptome. And as such, we identified 16 genes associated with type I IFN signaling pathway (Table 3), 22 genes belonging to different antiviral effector families (Table 4), 12 genes associated with adaptive immune responses (Table 5) and 10 apoptosis associated genes (Table 6) as shown below.
Genes of type I IFN signaling pathway
The repertoire of pathogen recognition receptors (PRRs), signal transducers and regulatory factors expressed in response to type I IFN treatment and SAV-3 infection in TO-cells is shown in Table 3. Generally, the fold increase was twofold higher for the type I IFN induced genes (TO-VS-IFN) than the SAV-3 induced genes (TO-VS-SAV3). Among the toll-like receptors (TLRs) only TLR3 and TLR8 were upregulated while for the RIG-like receptors (RLRs) the fold increase of LGP2 was higher than RIG-I and MDA5. Four IFN regulatory factors (IRFs) were up regulated of which the fold increase of IRF3 and IRF7 was higher than the fold increase of IRF1 and IRF2. Up-regulation of genes associated with signal transduction included tyrosine-protein kinase JAK1, STAT1 and STAT2 while the negative regulatory factors for IFN signaling upregulated included SOCS1 and SOCS3. In addition, the IFN promoter stimulating protein 1 (IPS-1) that function as an adaptor for the downstream signaling of MDA5 and RIG-I induced responses was also upregulated.
Repertoire of antiviral effector genes
The repertoire of antiviral genes upregulated in response to type I IFN treatment (TO-VS-IFN) and SAV-3 infection (TO-VS-SAV3) is shown in Table 4. The fold increase in genes expressed in response to type I IFN was generally twofold higher than the fold increase for genes expressed in response to SAV-3 infection. In the TRIM family, four genes were upregulated namely TRIM 16, 21, 25 and 39 while in the IFIT family only IFIT1 and IFIT5 were upregulated. Among the GTPases only Mx and VLIG-1 were detected and the fold increase of VLIG-1 was highest among all antiviral genes upregulated in response to both type I IFN treatment and SAV-3 infection in TO-cells. For the IFI family, only IFI27 and IFI44 were upregulated with the fold increase of IFI44 being higher than IFI27. Other families of antiviral genes co-upregulated included PKR, viperin, ISG15, vig-2, CsMig1 and MIP-2. Only four antiviral genes were co-downregulated by type I IFN treatment and SAV-3 infection in TO-cells and these include EBPD, CXCd1, CLEAC4E and complement protein component C7-1 precursor.
Adaptive immune genes
The profile of co-upregulated genes associated with adaptive immune responses is shown in Table 5. Generally, the fold increase of genes expressed in response to type I IFN treatment (TO-VS-IFN) was higher than the fold increase for genes expressed in response to SAV-3 (TO-VS-SAV3) infection except for the chemokines CXC10 and CXCR3. IL-2 receptor had the highest fold increase both for the type I IFN treated and SAV-3 infected cells. As shown in Table 5, co-upregulated genes associated with adaptive immune responses were grouped into genes associated with activation of cytotoxic T-lymphocytes (MHC-1a and 1b), chemokines (CXC10, CCL19, CXCR3), cytokine receptors (IL-2 receptor subunit beta precursor and IL-10 receptor-β-chain precursor) and humoral immune response genes (IgH locus A and B). On the other hand, co-downregulated genes included IL-12 receptor subunit β-2-like and perforin-1-like genes.
Repertoire of apoptosis associated genes
The repertoire of co-upregulated and co-downregulated genes associated with apoptosis is shown in Table 6. Similar to observations made for DEGs associated with the IFN signaling pathways, antiviral effectors and adaptive immunity, fold increases of genes expressed in response to type I IFN treatment (TO-VS-IFN) were higher than fold increases for genes expressed in response to SAV-3 infection (TO-VS-SAV3) except for the apoptosis associated speck-like protein. Among the co-upregulated genes, XIAF-1 had the highest fold increase, followed by Galectin-9 and TRIM-16 (Table 6). Other upregulated genes include CASP8 and FADD-like apoptosis regulator, caspase-8-like, caspase-1 precursor and apoptosis regulator BAX. Down-regulated genes include programmed cell death 4a (SAV3-4a) and death-associated protein kinase 2 (DAPK2).
Figure 6A and B shows relative expression of upregulated genes derived from RNA-seq data representative of the IFN signaling pathway (TLR3, LGP2, IRF7B and STAT1), antiviral genes (viperin and IFIT5), apoptosis associated genes (gelactin-9, TRIM16 and galectin-3-binding) and adaptive immune response genes (CCL19, PBEF and MHC-I) analyzed by qRT-PCR. Consistent with RNA-seq data (Tables 1, 2, 3, 4 and 5), genes generated from type I IFN treatment were higher than genes expressed from SAV-3 infection although the fold increase was not similar to observations made from RNA-seq data (Figure 6A and B). Figure 6C shows DEGs co-downregulated by type I IFN and SAV3 by qRT-PCR that were also downregulated by RNA-seq. In summary, data in Figure 6 confirms the validity of data generated by RNA-Seq by showing that the genes upregulated by qRT-PCR were also found up regulated by RNA-seq and that genes that were downregulated by RNA-seq data were also found downregulated by qRT-PCR.
De novo assembly and transcriptome analysis
RNA-seq has emerged to be a valuable tool for studying transcriptomic changes that occur in response to microbial invasion in host cells although studies using RNA-seq on fish are limited. To our knowledge this is the first report on the use of RNA-seq to study IFN responses in fish cells. Although several computer based de novo assembly tools (e.g. Trans-AbySS, Oasis, SOAP2denovo and Trinity) have been developed, only the trinity program was used for sequence assembly in this study given that several studies have shown that Trinity is a powerful tool that has proved to be useful for annotating transcriptomes for different vertebrate species across taxa [12,13]. Compared to other de novo transcriptome assemblers, Trinity recovers more full length transcripts from RNA-seq data without a reference genome with a sensitivity similar to methods that rely on genome alignments  and as such Trinity was considered to be a better tool for use in TO-cells given the limited number of annotated genes that would serve as reference genes in salmonids. Using Trinity, this study demonstrates that short reads from illumina RNA-seq can be assembled into protein sequences used to identify DEGs in fish cells that can be matched to orthologous genes found in mammals. Therefore, from a comparative immunology standpoint, de novo assembly of transcriptomes can be used to compare orthologs of immune genes expressed in lower vertebrates, such as teleosts fish, with those found in higher vertebrates. For example, the DEGs generated in this study were matched to genes associated with IFN signaling pathway, antiviral effector functions, apoptosis associated genes and genes that activate adaptive immune responses that conform to IFN inducible genes expressed in higher vertebrates. And as such, given the limitation on annotated genes induced by type I IFN in fish, we used a comparative approach and compared genes expressed in this study with orthologous genes expressed in mammalian cells to gain a better understanding of the transcriptomic changes that occur in response to type I IFN treatment and SAV3-virus infection in TO-cells as discussed in detail below.
Genes of the type I IFN signaling pathway
Recognition of pathogen associated molecular patterns (PAMPs) by PRRs constitutes the first line of defense used by host cells in sensing microbial invasion. Three PRR families were upregulated namely TLRs, RLRs and NLRs in this study. Among the TLRs, only TLR3 and TLR8 that are sensors of nucleic acids released in the endosomal compartments of macrophages and DCs  were upregulated, which augments the notion that TO-cells possess macrophage/dendritic cell like properties . Unlike TLRs, RLRs comprising of MDA5, RIG-I and LGP2 are primary sensors of the 5′-triphosphate RNA expressed by viruses in the cytoplasm  and their upregulation in the case of SAV-3 infection in TO-cells supports the consensus view that they bind to the 5′-ppp-RNA expressed by alphaviruses during replication . While TLRs use the MyD88/TRIF adaptor, RIG-I and MDA5 uses the IPS-1 adaptor in their downstream signaling , which was also upregulated in this study. Further studies in mammalia show that RLR signaling converges on pathways utilized by TLR3 and TLR8 resulting in the production of similar ISGs .
Type I IFNs bind to the IFNα receptor (IFNAR), which activates JAK1 and TYK2 that phosphorylates STAT1 and STAT2, which form heterodimers, and in association with IRF9, forming a trimeric complex of IFN-stimulated gene factor 3 (ISGF3) that translocates to the nucleus where it binds IFN-stimulated response elements (ISRE) in the promoters of ISGs genes to drive their expression . ISGs interfere with virus replication to establish a cellular antiviral state. Of the four upregulated IRFs, expression of IRF3 and IRF7 was higher than IRF1 and IRF2 suggesting that IRF3 and IRF7 played a major role in inducing type I IFN responses in TO-cells. In additions, these findings suggest that IRF3 and IRF7 regulate the TLR3 and TLR8 pathways which is in line with observations in mammalia where it has been shown that IRF3 and IRF7 are master regulators of TLR3 and TLR8 pathways . Finally, SOCS1 and SOCS3 block JAK activity and STAT recruitment to the receptor thereby creating a negative signaling that prevents excess cytokine signaling that could impair the normal homeostasis and cellular function of IFN producing cells [18,19]. Hence, the expression of SOCS1 and SOCS3 in this study could have been for regulating the negative feedback of IFN signaling induced in TO-cells. Overall, genes expressed in response to type I IFN treatment and SAV-3 infection in this study conform to genes of the canonical type I IFN signaling pathway expressed in higher vertebrate cells.
Antiviral effector genes
Antiviral genes induced by type I IFN exert their effector functions by inhibiting the replication of virus at different stages of virus replication cycles. For examples, PKR inhibits cellular mRNA translation which in turn prevent viral protein synthesis  while ISG15 achieves its antiviral function by conjugating to target proteins followed by altering their function . Viperin interferes with assembly and release of virus particles by disrupting the endoplasmic reticulum transport system that translocates viral particles to the plasma membrane . Hence, the upregulation of these genes in this study could opt for similar functions as those reported in higher vertebrates.
The TRIM family is primarily induced by type-I IFNs expressed in macrophages, dendritic cells, lymphocytes and fibroblasts . Recently, various TRIMs have been identified in different fish species [24-26] inclusive of TRIMs 16, 25 and 39 expressed in this study. TRIM proteins block virus infection using different mechanisms . For example, TRIM5α restricts virus entry by binding to the capsid of HIV virus to block uncoating [27,28] while TRIM22 interferes with pre-genomic RNA synthesis and protease activity of hepatitis B virus . Hence, it is likely that TRIM 16, 21, 25 and 39 expressed in TO-cells in this study have antiviral effects targeted at different stages of virus replication. Apart from their antiviral effector functions, TRIMs also participates in the induction of IFN synthesis. For example, TRIM25 is involved in the synthesis of IFN-β through the RIG-I pathway . Thus, it is likely that TRIMs expressed in this study are involved in the synthesis of IFNs. However, there is need for detailed studies to elucidate the mechanisms used by these TRIMs in restricting SAV-3 replication in fish cells and to determine their role in the synthesis of type I IFNs in TO-cells.
The IFIT family encodes genes induced by IFN treatment, virus infection or PAMP recognition and they confer antiviral protection through disruption of protein-protein interactions in the host translation-initiation machinery . Recent revelations show that IFITs can specifically recognize ssRNA bearing a 5′-(5′-ppp-) triphosphate group , thereby acting as a sensor for detecting viral ssRNAs. Single-stranded 5′-ppp-RNAs, which lack 2′-O-methylation of the 5′ cap and bear a 5′-ppp group, are specifically from viruses, which serve as a molecular signature for distinguishing self from non-self mRNAs [33,34]. Crystallography has shown that only single stranded 5′ppp-RNAs bind to IFIT1 and IFIT5 . Hence, it is likely that the IFIT1 and IFIT5 expressed in this study binds to the 5′-ppp-RNA of SAV-3 to create an antiviral state against the virus in TO-cells .
IFN-inducible GTPases currently recognized in humans are made of four families namely the myxovirus resistant proteins (Mxs), guanylate-binding proteins (GBPs), immunity-related GTPase proteins (IRGs) and very large inducible GTPase proteins (VLIGs). Among these only Mx and VLIGs were expressed in response to type I IFN treatment and SAV-3 infection in this study. Thus far, only Mx has been widely studied in salmonids [36-38] while the antiviral effector mechanisms of VLIGs in fish cells are yet to be elucidated.
Other antiviral genes upregulated in response to type I IFN treatment and SAV-3 infection in TO-cells include IFI27, IFI44, CsMig1, MIP-2 and vig-2 protein while the down regulated genes include CXCd1 and CLEAC4E. Although some of these genes, such as vig-2, have previously been reported in fish  their functional mechanisms have not been established this far and there is need to elucidate the antiviral mechanisms of these genes in fish cells.
Type-I IFN apoptosis associated genes
Apoptosis, a form of programmed cell death, is a mechanism used by multicellular organisms to get rid of unwanted cells in a systematic manner [32,40]. The central feature of apoptosis, unlike necrosis, is the containment of cellular materials in membranous structures in which apoptotic particles are phagocytized without leaking the intracellular contents to the extracellular milieu [41,42]. To attain this, apoptotic cells induce signaling pathways using IFN induced genes to facilitate the removal of unwanted cells from the host. Among the apoptosis associated genes expressed in this study, XAF-1 had the highest response to type I IFN treatment and SAV-3 infection followed by Gelactin-9. XIAF-1 has been shown to block the activities of XIAP which is a known inhibitor of apoptosis (IAP) in human cells [43,44] while Galectin-9 is vital for T-cell apoptosis where it participates in killing activated or infected T-cells following an immune response . Other apoptosis associated genes expressed in this study include the apoptosis associated speck-like protein which contains a caspase recruitment domain (CARD) linked to induction of apoptosis signaling pathways  while caspase 8 belong to the family of proteases that function in the initiation and execution of cell disassembly in response to apoptosis signals . Although the functional mechanisms of these genes are well studied in higher vertebrate cells, their mode of action in fish cells is yet to be elucidated.
Adaptive immune response genes
Type I IFNs enhance antigen presentation by upregulation of MHC-I and differentiation of virus specific cytotoxic T-lymphocytes thus providing an important link between innate and adaptive immunity . The repertoire of adaptive immune genes upregulated in this study conforms to genes engaged in activation of the adaptive immune response. For example, expression of MHC class Ia and Ib genes was accompanied by upregulation of chemokines essential for recruitment and activation of T-cells such as CXCR3, which is selectively expressed in activated T-cells and not in other leukocyte subpopulations . CXCR3 functions as a receptor for CXCL10 which plays an important role in the development and maturation of T-cells . CCL19 is strongly chemotactic for naïve CD4 and CD8-T-cell and its expression plays an important role in the homing of naïve T-cell to MHC-I molecules expressing surface antigens on DCs . By executing its chemotactic role, CCL19 initiates the activation of naïve CD4 and CD8 T-cells into effector T-helper (TH) cells and cytotoxic T-lymphocytes (CTLs) , respectively.
Apart from enhancing the maturation of naïve T-cells into cytotoxic T-lymphocytes, type I IFNs also play an important role in the maturation of B-cells. In the present study this notion was supported by upregulation PBEF a cytokine that acts on early B-cell lineage precursor cells and regulates the early and late events leading to maturation of B-cell . In addition, upregulation of IgH locus A and B is suggestive of reorganization of the B-cell receptors induced by type I IFNs during the early developmental stages. Further, upregulation of IL-2-receptor which regulates the activation of naïve T-helpers cells to activated TH2 cells  that in turn play a helper role in the maturation of naïve B-cells into immunoglobulin secreting cells  further supports the role of type I IFNs in activating the adaptive immune response . Although the functional mechanisms of these genes are well studied in higher vertebrates, their upregulation in this study suggest that they could have the same functional roles in fish cells.
Induction of type I IFN responses by SAV-3 in TO-cells
Data presented here suggests that SAV-3 is a potent inducer of type I IFNs in TO-cells. Our previous studies show that despite SAV-3 induces a strong IFN response, the virus replicates vividly in TO cells . When cells are pre-treated with recombinant IFN, 4 to 24 hrs prior to infection, with recombinant IFNα TO cells are protected against virus induced cytopathic effects and virus replication is inhibited . These findings are consistent with observations made for other alphaviruses in mammalia showing that pretreatment with IFN inhibits alphavirus replication of in-vivo [56,57]. For SAV-3 it is not understood why the virus can replicate in vitro under strong IFN responses. Studies in Chikungunya virus (CHIKV), another alphavirus, show that virus replication is resistant to IFN inhibition once replication is established  and it was shown that CHIKV uses the nsP2 to suppress the antiviral effect of IFN by interfering with the JAK-STAT signaling pathway enabling the virus to replicate in the presence of IFN. TO-cells used in this study were not pretreated with IFN prior to SAV-3 infection and concordant with previous findings once infection was established, IFN released through downstream signal transduction had no inhibitory effects in the subsequent replication of the virus . Although we did not determine the mechanisms used by SAV-3 to circumvent the IFN antiviral effects produced by downstream signal transduction, several studies have shown that alphaviruses use different mechanisms to block the antiviral effects of IFN once infection is established [59,60]. Put together, these studies accentuate the importance of timing on the inhibitory effects of IFNs on the replication of alphaviruses in infected cells. Based on data presented here and our previous findings , it can be concluded that TO-cells pretreated with IFNα (4-24hrs) before infection inhibit SAV-3 replication while the IFN response induced from the SAV-3 infection is not sufficient to inhibit virus replication . Thus, there is need for more detailed investigations to elucidate the mechanisms that inhibit the antiviral effects of IFN produced by downstream signal transduction after SAV-3 infection in TO-cells.
Downregulation of host cellular gene expression by SAV-3 infection in TO-cells
It is interesting to note that TO-cells infected by SAV-3 (TO-VS-SAV3) had by far a large proportion (22,259 DEGs) of down-regulated genes compared to IFN treated cells (TO-VS-IFN) (993 DEGs). Similar observations have been made for other alphaviruses [61,62] and several other viral families [63-67] in which virus infection has been shown to downregulate the expression of several genes regulating cellular transcription during virus replication as a survival strategy leading to persistent infections. For example, Gorchakov et al.  have shown that replication of Sindbis virus downregulates major cellular processes such as the transcription and translation of mRNAs in infected cells. In their studies, they noted that inhibition of cellular mRNA transcription is a critical phenomenon used by viruses to suppress the expression of cellular stress inducible genes in vertebrate cells as a survival strategy to enhance their replication. Hence, this would account for the downregulation of a large proportion of genes linked to cellular, biological and molecular functions in TO-cells that were only infected by SAV-3 (TO-VS-SAV3) and not those treated with IFN (TO-VS-IFN) in this study. Similarly, in our previous studies we showed protein shutdown in TO-cells infected with SAV-3 only which was not seen in untreated TO-cells  which augments our current findings. Put together, these studies suggest that SAV-3 infection could be downregulating a wide range of host cellular genes to enhance its replication in TO-cells using mechanisms similar to those seen for other alphaviruses in higher vertebrates [61,62]. However, there is a need for detailed investigations to underpin the exact mechanisms used by this virus to dowgnregulate the expression of host cellular genes and to demonstrate how suppression of these genes could enhance the replication of SAV-3 in TO-cells.
In this study, we present a de novo assembly and analysis of a transcriptome of DEGs generated in response to type I IFN treatment and SAV-3 infection in the macrophage/dendritic like TO-cells derived from Atlantic salmon headkidney leukocytes. Transcriptomic changes reported here show a profile of genes belonging to the canonical type I IFN signaling pathway together with a broad spectrum of antiviral effector genes that block virus replication at different stages of the virus replication cycle. In addition, the transcriptome also shows a profile of genes associated with apoptosis as well as a repertoire of genes associated with activation of adaptive immunity. Our findings also show that the profile of type I IFN pathway related genes expressed by TO-cells is comparable to orthologous genes expressed by mammalian macrophages and dendritic cells. Further, the study shows that SAV-3 is a potent inducer of type I IFN responses in TO-cells and that it could serve as a reliable model for studying IFN protective mechanisms in fish cells. However, it is vital to note the repertoire of type I IFN induced genes reported here only shows a profile of up- and down-regulated genes, but it does not show the exact mechanisms used by these genes to protect host cells. And as such, future studies should seek to elucidate the functional mechanisms used by these genes in protecting fish cells. In summary, this study shows a de novo assembly of a transcriptome of IFN induced genes in response to type I IFN treatment and SAV-3 infection in TO-cells that were matched to their orthologs in higher vertebrates.
The RNA-sequencing data generated in this study has been deposited in the National Center for Biotechnology Information (NCBI) Gene Expression Omnibus (GEO) database accession number GSE64095 (www.ncbi.nih.gov/geo Accession number GSE64095).
Murphy TM, Rodger HD, Drinan EM, Gannon F, Kruse P, Korting W. The sequential pathology of pancreas disease in Atlantic salmon farms in Ireland. J Fish Dis. 1992;15:401–8.
Munro ALS, Ellis AE, Mcvicar AH, Mclay HA, Needham EA. An exocrine pancreas disease of farmed Atlantic salmon in Scotland. Helgolander Meeresuntersuchungen. 1984;37:571–86.
Weston JH, Welsh MD, McLoughlin MF, Todd D. Salmon pancreas disease virus, an alphavirus infecting farmed Atlantic salmon, Salmo salar L. Virology. 1999;256:188–95.
Weston J, Villoing S, Bremont M, Castric J, Pfeffer M, Jewhurst V, et al. Comparison of two aquatic alphaviruses, salmon pancreas disease virus and sleeping disease virus, by using genome sequence analysis, monoclonal reactivity, and cross-infection. J Virol. 2002;76:6155–63.
Strauss JH, Strauss EG. The alphaviruses: gene expression, replication, and evolution. Microbiol Rev. 1994;58:491–562.
Xu C, Guo TC, Mutoloki S, Haugland O, Marjara IS, Evensen O. Alpha interferon and not gamma interferon inhibits Salmonid alphavirus subtype 3 replication In vitro. J Virol. 2010;84:8903–12.
MacMicking JD. Interferon-inducible effector mechanisms in cell-autonomous immunity. Nat Rev Immunol. 2012;12:367–82.
Stark GR, Kerr IM, Williams BRG, Silverman RH, Schreiber RD. How cells respond to interferons. Ann Rev Biochem. 1998;67:227–64.
Schoggins JW, Wilson SJ, Panis M, Murphy MY, Jones CT, Bieniasz P, et al. A diverse range of gene products are effectors of the type I interferon antiviral response. Nature. 2011;472:481–U545.
Pettersen EF, Ingerslev HC, Stavang V, Egenberg M, Wergeland HI. A highly phagocytic cell line TO from Atlantic salmon is CD83 positive and M-CSFR negative, indicating a dendritic-like cell type. Fish Shellfish Immunol. 2008;25:809–19.
Wergeland HI, Jakobsen RA. A salmonid cell line (TO) for production of Infectious Salmon Anaemia Virus (ISAV). Dis Aquat Organ. 2001;44:183–90.
Grabherr MG, Haas BJ, Yassour M, Levin JZ, Thompson DA, Amit I, et al. Full-length transcriptome assembly from RNA-Seq data without a reference genome. Nat Biotechnol. 2011;29:644–52.
Moreton J, Dunham SP, Emes RD. A consensus approach to vertebrate de novo transcriptome assembly from RNA-seq data: assembly of the duck (Anas platyrhynchos) transcriptome. Front Genet. 2014;5:190.
Cervantes JL, Weinerman B, Basole C, Salazar JC. TLR8: the forgotten relative revindicated. Cell Mol Immunol. 2012;9:434–8.
Takeuchi O, Akira S. Innate immunity to virus infection. Immunol Rev. 2009;227:75–86.
Basler CF, Garcia-Sastre A. Sensing RNA virus infections. Nat Chem Biol. 2007;3:20–1.
Jensen S, Thomsen AR. Sensing of RNA viruses: a review of innate immune receptors involved in recognizing RNA virus invasion. J Virol. 2012;86:2900–10.
Ivashkiv LB, Donlin LT. Regulation of type I interferon responses. Nat Rev Immunol. 2014;14:36–49.
Yoshimura A, Naka T, Kubo M. SOCS proteins, cytokine signalling and immune regulation. Nat Rev Immunol. 2007;7:454–65.
Dauber B, Wolff T. Activation of the antiviral kinase PKR and viral countermeasures. Viruses-Basel. 2009;1:523–44.
Skaug B, Chen ZJJ. Emerging role of ISG15 in antiviral immunity. Cell. 2010;143:187–90.
Wang XY, Hinson ER, Cresswell P. The interferon-inducible protein viperin inhibits influenza virus release by perturbing lipid rafts. Cell Host Microbe. 2007;2:96–105.
Mcnab FW, Rajsbaum R, Stoye JP, O’Garra A. Tripartite-motif proteins and innate immune regulation. Curr Opin Immunol. 2011;23:46–56.
Boudinot P, van der Aa LM, Jouneau L, Du PL, Pontarotti P, Briolat V, et al. Origin and evolution of TRIM proteins: new insights from the complete TRIM repertoire of zebrafish and pufferfish. PLoS One. 2011;6:e22022.
Boudinot P, Zou J, Ota T, Buonocore F, Scapigliati G, Canapa A, et al. A tetrapod-like repertoire of innate immune receptors and effectors for coelacanths. J Exp Zool B Mol Dev Evol. 2014;322(6):415–37.
van der Aa LM, Levraud JP, Yahmi M, Lauret E, Briolat V, Herbomel P, et al. A large new subset of TRIM genes highly diversified by duplication and positive selection in teleost fish. BMC Biol. 2009;7:7.
Pertel T, Hausmann S, Morger D, Zuger S, Guerra J, Lascano J, et al. TRIM5 is an innate immune sensor for the retrovirus capsid lattice. Nature. 2011;472:361–5.
Stremlau M, Owens CM, Perron MJ, Kiessling M, Autissier P, Sodroski J. The cytoplasmic body component TRIM5 alpha restricts HIV-1 infection in Old World monkeys. Nature. 2004;427:848–53.
Gao B, Duan ZJ, Xu W, Xiong SD. Tripartite motif-containing 22 Inhibits the activity of hepatitis B virus core promoter, which Is dependent on nuclear-located RING domain. Hepatology. 2009;50:424–33.
Gack MU, Shin YC, Joo CH, Urano T, Liang C, Sun L, et al. TRIM25 RING-finger E3 ubiquitin ligase is essential for RIG-I-mediated antiviral activity. Nature. 2007;446:916–20.
Diamond MS, Farzan M. The broad-spectrum antiviral functions of IFIT and IFITM proteins. Nat Rev Immunol. 2013;13:46–57.
Hofmann K. The modular nature of apoptotic signaling proteins. Cell Mol Life Sci. 1999;55:1113–28.
Abbas YM, Pichmair A, Gorna MW, Superti-Furga G, Nagar B. Structural basis for viral 5′-PPP-RNA recognition by human IFIT proteins. Nature. 2013;494:60–4.
Pichlmair A, Lassnig C, Eberle CA, Gorna MW, Baumann CL, Burkard TR, et al. IFIT1 is an antiviral protein that recognizes 5′-triphosphate RNA. Nat Immunol. 2011;12:624–U177.
Moriette C, LeBerre M, Lamoureux A, Lai TL, Bremont M. Recovery of a recombinant Salmonid alphavirus fully attenuated and protective for rainbow trout. J Virol. 2006;80:4088–98.
Collet B. Innate immune responses of salmonid fish to viral infections. Dev Comp Immunol. 2014;43:160–73.
Munang’andu HM, Fredriksen BN, Mutoloki S, Dalmo RA, Evensen O. Antigen dose and humoral immune response correspond with protection for inactivated infectious pancreatic necrosis virus vaccines in Atlantic salmon (Salmo salar L). Vet Res. 2013;44:7.
Xu C, Guo TC, Mutoloki S, Haugland O, Evensen O. Gene expression studies of host response to Salmonid alphavirus subtype 3 experimental infections in Atlantic salmon. Vet Res. 2012;43:78.
Boudinot P, Salhi S, Blanco M, Benmansour A. Viral haemorrhagic septicaemia virus induces vig-2, a new interferon-responsive gene in rainbow trout. Fish Shellfish Immunol. 2001;11:383–97.
Kerr JF, Wyllie AH, Currie AR. Apoptosis: a basic biological phenomenon with wide-ranging implications in tissue kinetics. Br J Cancer. 1972;26:239–57.
Majno G, Joris I. Apoptosis, oncosis, and necrosis. An overview of cell death. Am J Pathol. 1995;146:3–15.
Hart SP, Haslett C, Dransfield I. Recognition of apoptotic cells by phagocytes. Experientia. 1996;52:950–6.
Leaman DW, Chawla-Sarkar M, Vyas K, Reheman M, Tamai K, Toji S, et al. Identification of X-linked inhibitor of apoptosis-associated factor-1 as an interferon-stimulated gene that augments TRAIL Apo2L-induced apoptosis. J Biol Chem. 2002;277:28504–11.
Liston P, Fong WG, Kelly NL, Toji S, Miyazaki T, Conte D, et al. Identification of XAF1 as an antagonist of XIAP anti-caspase activity. Nat Cell Biol. 2001;3:128–33.
Hernandez JD, Baum LG. Ah, sweet mystery of death! Galectins and control of cell fate. Glycobiology. 2002;12:127R–36.
Masumoto J, Taniguchi S, Nakayama J, Shiohara M, Hidaka E, Katsuyama T, et al. Expression of apoptosis-associated speck-like protein containing a caspase recruitment domain, a pyrin N-terminal homology domain-containing protein, in normal human tissues. J Histochem Cytochem. 2001;49:1269–75.
Chawla-Sarkar M, Lindner DJ, Liu YF, Williams B, Sen GC, Silverman RH, et al. Apoptosis and interferons: Role of interferon-stimulated genes as mediators of apoptosis. Apoptosis. 2003;8:237–49.
Samuel CE. Antiviral actions of interferons. Clin Microbiol Rev. 2001;14:778–809.
Rossi D, Zlotnik A. The biology of chemokines and their receptors. Ann Rev Immunol. 2000;18:217–43.
Groom JR, Richmond J, Murooka TT, Sorensen EW, Sung JH, Bankert K, et al. CXCR3 chemokine receptor-ligand interactions in the lymph node optimize CD4(+) T helper 1 cell differentiation. Immunity. 2012;37:1091–103.
Robbiani DF, Finch RA, Jager D, Muller WA, Sartorelli AC, Randolph GJ. The leukotriene C-4 transporter MRP1 regulates CCL19 (MIP-3 beta, ELC)-dependent mobilization of dendritic cells to lymph nodes. Cell. 2000;103:757–68.
Samal B, Sun YH, Stearns G, Xie CS, Suggs S, Mcniece I. Cloning and characterization of the cDNA-encoding a novel human pre-B-cell colony-enhancing factor. Mol Cell Biol. 1994;14:1431–7.
Pfizenmaier K, Rollinghoff M, Wagner H. Functional-analysis of IL-2 produced by T-cell-hybridomas - IL-2 promotes T-cell growth but does not mediate T-cell or B-cell maturation and differentiation. Curr Top Microbiol. 1982;100:203–9.
DeKruyff RH, Rizzo LV, Umetsu DT. Induction of immunoglobulin synthesis by CD4+ T cell clones. Semin Immunol. 1993;5:421–30.
Mackay CR. Chemokine receptors and T cell chemotaxis. J Expl Med. 1996;184:799–802.
Despres P, Griffin JW, Griffin DE. Antiviral activity of alpha-interferon in Sindbis virus-infected cells is restored by anti-E2 monoclonal-antibody treatment. J Virol. 1995;69:7345–8.
Frolov I, Akhrymuk M, Akhrymuk I, Atasheva S, Frolova EI. Early events in alphavirus replication determine the outcome of infection. J Virol. 2012;86:5055–66.
Fros JJ, Liu WJ, Prow NA, Geertsema C, Ligtenberg M, Vanlandingham DL, et al. Chikungunya virus nonstructural protein 2 inhibits type I/II interferon-stimulated JAK-STAT signaling. J Virol. 2010;84:10877–87.
Yin J, Gardner CL, Burke CW, Ryman KD, Klimstra WB. Similarities and differences in antagonism of neuron alpha/beta interferon responses by Venezuelan equine encephalitis and Sindbis slphaviruses. J Virol. 2009;83:10036–47.
Simmons JD, White LJ, Morrison TE, Montgomery SA, Whitmore AC, Johnston RE, et al. Venezuelan equine encephalitis virus disrupts STAT1 signaling by distinct mechanisms independent of host shutoff. J Virol. 2009;83:10571–81.
Gorchakov R, Frolova E, Frolov I. Inhibition of transcription and translation in Sindbis virus-infected cells. J Virol. 2005;79:9397–409.
Fros JJ, Major LD, Scholte FE, Gardner J, van Hemert MJ, Suhrbier A, et al. Chikungunya virus nsP2-mediated host shut-off disables the unfolded protein response. J Gen Virol. 2014. doi:10.1099/vir.0.071845-0.
Billecocq A, Spiegel M, Vialat P, Kohl A, Weber F, Bouloy M, et al. NSs protein of rift valley fever virus blocks interferon production by inhibiting host gene transcription. J Virol. 2004;78:9798–806.
Dasgupta A. Targeting TFIIH to inhibit host cell transcription by Rift Valley fever virus. Mol Cell. 2004;13:456–8.
Weidman MK, Sharma R, Raychaudhuri S, Kundu P, Tsai W, Dasgupta A. The interaction of cytoplasmic RNA viruses with the nucleus. Virus Res. 2003;95:75–85.
Yuan H, Yoza BK, Lyles DS. Inhibition of host RNA polymerase II-dependent transcription by vesicular stomatitis virus results from inactivation of TFIID. Virology. 1998;251:383–92.
Yuan H, Puckett S, Lyles DS. Inhibition of host transcription by vesicular stomatitis virus involves a novel mechanism that is independent of phosphorylation of TATA-binding protein (TBP) or association of TBP with TBP-associated factor subunits. J Virol. 2001;75:4453–8.
The study was financed by the Research Council of Norway, project “The Atlantic salmon genome sequence as a tool for precision breeding” project number 226275, and the Targeted disease prophylaxis in European Fish farming project, grant agreement 311993. We thank Jiang Li, affiliated to Beijing Genomics Institute (BGI) for assistance with some bioinformatics.
The authors declare that they have no competing interests.
CX = Carried out laboratory experiments and data analysis and preparation of manuscript; HMM = carried out data analysis and preparation of the manuscript; ØE = mobilizing of resources, data analysis, preparation of the manuscript and overall supervision of the project. All authors read and approved submission of the manuscript for publication.
About this article
Cite this article
Xu, C., Evensen, Ø. & Munang’andu, H.M. De novo assembly and transcriptome analysis of Atlantic salmon macrophage/dendritic-like TO cells following type I IFN treatment and Salmonid alphavirus subtype-3 infection. BMC Genomics 16, 96 (2015). https://doi.org/10.1186/s12864-015-1302-1
- Salmonid alphavirus
- De novo assembly