Whereas temporal gene expression in mammalian herpesviruses has been studied extensively, little is known about gene expression in fish herpesviruses. Here we report a genome-wide transcription analysis of a fish herpesvirus, anguillid herpesvirus 1, in cell culture, studied during the first 6 hours of infection using reverse transcription quantitative PCR.
Four immediate-early genes – open reading frames 1, 6A, 127 and 131 – were identified on the basis of expression in the presence of a protein synthesis inhibitor and unique expression profiles during infection in the absence of inhibitor. All of these genes are located within or near the terminal direct repeats. The remaining 122 open reading frames were clustered into groups on the basis of transcription profiles during infection. Expression of these genes was also studied in the presence of a viral DNA polymerase inhibitor, enabling classification into early, early-late and late genes. In general, clustering by expression profile and classification by inhibitor studies corresponded well. Most early genes encode enzymes and proteins involved in DNA replication, most late genes encode structural proteins, and early-late genes encode non-structural as well as structural proteins.
Overall, anguillid herpesvirus 1 gene expression was shown to be regulated in a temporal fashion, comparable to that of mammalian herpesviruses.
Herpesvirus gene expression occurs in a temporally regulated fashion involving three major gene sets [1, 2]. The first set consists of the immediate-early genes, which are defined as those that are transcribed in the absence of de novo protein synthesis. These genes regulate the subsequent expression of other genes. The next set, the early genes, encodes the enzymes involved in nucleotide metabolism and replication of the viral genome, and several envelope glycoproteins. The final set, the late genes, requires viral DNA synthesis for expression and encodes viral structural proteins. There is usually no clear boundary between early and late expression, and an intermediate leaky-late or early-late group has been proposed. Although this widely-used classification of herpesvirus genes may not fully reflect the subtle regulation of viral gene expression in infected cells, it helps understanding of the viral replication cycle, gene functions, virus-host interactions and possibilities for control of disease.
Herpesvirus genes have traditionally been classified kinetically on the basis of individual expression studies in cell culture . Application of specific chemicals to inhibit selectively the expression of early and/or late genes has contributed to the classification and functional characterization of genes. More recently, genome-wide microarray and reverse transcription quantitative (RT-q)PCR expression studies have been performed for several mammalian herpesviruses in the family Herpesviridae[4–11]. However, little is known about expression in members of the family Alloherpesviridae, which infect amphibians and fish.
For channel catfish virus (ictalurid herpesvirus 1, IcHV1) the expression kinetics of a limited number of open reading frames (ORFs), namely ORF3, ORF5, ORF5/6, ORF6, ORF8A/9, ORF9, ORF12/13, ORF39 and ORF46 [12–14], has been studied in cell culture by northern blot analyses. Transcriptional regulation of all 14 ORFs in the terminal direct repeat of the genome has been analysed by northern blot analysis in cell culture  and by RT-PCR and Southern blot analysis in vivo. For this small number of IcHV1 ORFs, temporal expression patterns similar to that of mammalian herpesviruses have been demonstrated. In addition, transcription in cell culture of 20 ORFs in koi herpesvirus (cyprinid herpesvirus 3, CyHV3) has been demonstrated by RT-PCR .
Anguillid herpesvirus 1 (AngHV1) causes a haemorrhagic disease and is associated with increased mortality rates in the Japanese eel (Anguilla japonica) and European eel (Anguilla anguilla) [18, 19]. In this first report on genome-wide transcription of an alloherpesvirus, we characterized expression in cell culture of AngHV1 ORFs that are predicted to encode functional proteins by using RT-qPCR, which permits sensitive quantitation of specific RNAs [20, 21]. Expression of early and late ORFs was selectively blocked by a protein synthesis inhibitor, and expression of late ORFs was inhibited by a viral DNA polymerase inhibitor. The genes were classified on the basis of their expression patterns in the presence of these inhibitors. We identified four putative immediate-early ORFs, and – on the basis of their transcription profiles – clustered all but three of the remaining 125 ORFs into early, early-late and late gene categories. The analysis relied on an AngHV1 map [GenBank:FJ940765.3] that is a substantial improvement on the original map derived from bioinformatic analysis of the complete genome sequence . The updated map was derived from a deep-sequencing transcriptome study , and included redefined ORFs and experimentally supported polyadenylation (polyA) sites. The deep sequencing study also showed that, overall, 98.5% of late transcription of AngHV1 ORFs is directed by the sense DNA strand.
Results and discussion
One-day old eel kidney 1 (EK-1) cell monolayers  in 6-well plates were pre-incubated with either virus growth medium (VGM), VGM containing protein synthesis inhibitor cycloheximide (CHX), or VGM containing viral DNA polymerase inhibitor phosphonoacetic acid (PAA). After the pre-incubation, the cells were infected with the Dutch AngHV-1 isolate CVI500138  at a multiplicity of infection (MOI) of 10 50% tissue culture infective dose (TCID50)/cell in the appropriate VGM. RNA was extracted at t = 0, 1, 2, 4, and 6 h post infection (hpi). Potential contaminating DNA was removed, polyA RNA was extracted and reverse transcribed into cDNA. SYBR Green quantitative (q)PCR reactions were carried out for all AngHV1 ORFs, taking a reaction for the reference β-actin gene of European eel  into account in every qPCR run for each time point. Based on the efficiency of amplification (E) for each primerset, relative expression ratio (R) [7, 27], change in relative gene expression (RΔ), inhibitory effect of CHX at t = 4 and t = 6 hpi (Ri-CHX), and inhibitory effect of PAA at t = 6 hpi (Ri-PAA) were calculated.
Experiments in which cells were untreated were carried out three times, and experiments in which cells were treated with PAA or CHX were carried out twice. The β-actin reference gene Ct-values were highly reproducible; the mean value ± standard deviation of all measurements (n = 656) of all experiments was 16.73 ± 2.14 (coefficient of variation = 12.8%).
Relative expression ratios were calculated independently for each experiment, and the mean and standard deviation values were subsequently calculated for all ORFs and time points. The average coefficient of variation for Ri-CHX for the non-inhibited ORFs at t = 4 and t = 6 hpi was 21.8% and 22.7%, respectively. The average coefficient of variation for Ri-PAA for all ORFs at t = 6 hpi was 16.8%.
Families of 3’-coterminal transcripts
Although herpesvirus genes generally have individual promotors, it is not uncommon for a single polyA site to be shared by two or more genes arranged as a 3’-coterminal family . In the deep-sequencing transcriptome study of AngHV1 , 32 such families were identified. With regard to the current study, the RT-qPCR signals detected for the 58 ORFs that are not in 3’-coterminal families and the 32 ORFs that are located at the 5’-ends of 3’-coterminal families can be considered accurate. However, signals detected for the remaining 36 ORFs might be mixed with those from upstream ORFs, and a more tentative interpretation is implicit in the results discussed below.
AngHV1 gene expression
Gene expression was detected at some time point for all predicted functional protein-coding ORFs in the AngHV1 genome. In general, levels were absent or very low at t = 1 and t = 2 hpi and increased exponentially during the monitored period. ORF1, ORF6A, ORF127 and ORF131 were the first genes becoming detectable, they already showed significant expression at t = 2 hpi. Maximum expression was measured at t = 6 hpi for all ORFs, except for ORF1, ORF86 and ORF130, which peaked at t = 4 hpi.
The net change in transcription at each time interval or RΔ was calculated for each gene (Additional file 1: Table S1). The genes were clustered based on their RΔ-values, and ten groups were distinguished (Figure 1). RΔ-graphs are shown for all gene groups (Figure 2), with the unique expression kinetics of ORF1, ORF6A, ORF127 and ORF131 combined in one (Figure 2A, group IE). The RΔ-graphs of the upstream located 3’-coterminal ORFs are represented by dashed lines.
The RΔ of the 12 members of groups E1-4 is characterized by a very low value at R2-R1, a steep increase between R2-R1 and R4-R2, and a decrease or stabilization at R6-R4 (Figure 2B-E). Differentiation between the E groups is based on the RΔ-value at R6-R4, which varies from practically zero (group E1) to more or less similar at R4-R2 and R6-R4 (group E4).
The RΔ of members of groups EL1 and EL2 is characterized by a very low value at R2-R1, and a more or less linear increase between R2-R1 and R6-R4 (Figure 2F-G). The 9 members of group EL1 show a slightly earlier but less steep increase of RΔ than the 12 members of group EL2. Both members of the ORF109 gene family (ORF109 and ORF125) belong to group EL1, with ORF125 being identified as a low-abundant envelope protein .
Most of the genes fall into group L (n = 89). The RΔ-value is zero or very low at R2-R1, very low or low at R4-R2, and almost maximal at R6-R4 (Figure 2H). Group L comprises both members of the ORF3 gene family (ORF3 and ORF14), both members of the ORF11 gene family (ORF11 and ORF12), three members of the ORF13 gene family (ORF16, ORF17 and ORF24), three members of the ORF68 gene family (ORF69, ORF70 and ORF73), both members of the deoxyguanosine kinase (dGK) gene family (ORF79 and ORF123), and three members of the tumour necrosis factor receptor (TNFR) gene family (ORF108, ORF121 and ORF124).
In the analysis described above, we followed the RT-qPCR-based approach used to study gene expression by Tombácz et al. in pseudorabies virus (PRV; a mammalian herpesvirus in subfamily Alphaherpesvirinae, family Herpesviridae). In general, gene expression profiles are highly comparable for AngHV1 and PRV. The AngHV1 and PRV immediate-early genes and the PRV large latency transcript demonstrate unique expression profiles, genes in group E show maximum increase of gene expression between t = 2 and t = 4 hpi, genes in group L show maximum increase of gene expression between t = 4 and t = 6 hpi, and genes in group EL demonstrate an intermediate expression profile. AngHV1 comprises about twice as much ORFs as PRV, which mainly add up to the EL and L groups.
Immediate-early transcripts of AngHV1
Inhibition of de novo protein synthesis by CHX resulted in an inhibition of relative gene expression (Ri-CHX) of >66% at t = 4 and of >91% at t = 6 hpi for all but 4 ORFs. ORF6A and ORF127 showed almost no inhibition at t = 4 and t = 6 hpi (Figure 3). ORF1 demonstrated an increase in relative expression of 1.3 at t = 4 and of 7.6 at t = 6 hpi. ORF131 exhibited an increase in relative expression of 3.8 at t = 4 and of 4.7 at t = 6 hpi.
In cells not treated with inhibitors, these 4 immediate-early ORFs showed unique expression profiles that were clearly distinct from those of other ORFs (group IE). No imputed amino acid sequence similarities with ORFs in other alloherpesviruses were detected . ORF127 has been shown to encode a low-abundant structural tegument protein .
Early and early-late transcripts of AngHV1
Inhibition of viral DNA polymerase by PAA resulted in an inhibition of gene expression (Ri-PAA) at t = 6 hpi for all but two ORFs (Additional file 2: Table S2). In the presence of PAA, the relative expression of ORF1 was doubled, and that of ORF6A was not affected. Table 1 shows the mean and standard deviations of Ri-PAA-values in the presence of PAA at t = 6 hpi for the 61 ORFs of AngHV1 for which a putative function has been described (listed on the basis of their Ri-PAA-values), with the kinetic classes of ORFs potentially compromised by 3’-coterminality marked with asterisks.
Inhibition of gene expression by PAA ranges from about 30% for ORF87 to 99% for ORF95. A comparable range was described previously for PRV . The ORFs are classified into kinetic classes on the basis of their Ri-PAA-values, with arbitrarily set threshold values. The typical early gene ORF10, encoding the ATPase subunit of terminase, was chosen as the last early gene, and ORF18, encoding a structural tegument protein, as the first early-late gene. ORF75, encoding thymidylate synthetase, was denoted as the last of the early-late genes, and ORF34, encoding a structural tegument protein, as the first of the late genes. There was no clear boundary between early, early-late, and late genes based on their Ri-PAA-values.
A total of 17 early genes were identified (Additional file 2: Table S2). Almost half of these showed a distinct expression profile in the untreated samples (members of groups E1-4), characterized by the largest increase of RΔ between R2-R1 and R4-R2. Among the early genes are those involved in DNA replication (ORF55) and DNA packaging (ORF10), genes encoding a guanosine triphosphatase (GTPase) (ORF15), a serine-threonine protein kinase (ORF87), a protein encoding a TNFR domain (ORF101), and two low-abundant tegument proteins (ORF14 and ORF39). Early genes identified for IcHV1 included the thymidine kinase gene (IcHV1 ORF5), a protein kinase (IcHV1 ORF14), and two putative membrane proteins (IcHV1 ORF6 and IcHV1 ORF8) [14, 15].
A total of 37 early-late genes were identified, with inhibition of expression values intermediate between those of early and late genes (Additional file 2: Table S2). In samples not treated with inhibitors, 4 of the early-late genes were grouped into one of the E groups, and 10 genes were classified in one of the EL groups. Functions have been predicted for 17 of the early-late genes (Table 1). These consist of 9 genes encoding non-structural proteins and 8 encoding structural proteins. Among the non-structural group are proteins involved in DNA replication (ORF21 and ORF37) and enzymes involved in nucleic acid metabolism. Among the structural early-late gene proteins are 4 tegument and 4 envelope proteins, but no capsid proteins. For IcHV1, a membrane protein (IcHV1 ORF7), a tegument protein (IcHV1 ORF11) and a zinc-binding protein (IcHV1 ORF12) were shown to specify both early and late transcripts . Our findings are in general accordance with the properties of proteins encoded by early and early-late genes of mammalian herpesviruses.
Late transcripts of AngHV1
A total of 68 late genes were identified (Additional file 2: Table S2), 6 of which were clustered into one or other of the EL groups, and 62 of which were grouped in the L group. Functions have been assigned to 33 of the late gene proteins (Table 1), 28 of which involve roles as structural proteins. All 7 capsid proteins, as well as 14 tegument proteins and 7 envelope proteins, were identified as being encoded by late genes. Similarly, the three late genes identified for IcHV1 encode the major capsid protein (IcHV1 ORF39) and two membrane proteins (ORF10 and ORF46) [14, 15]. Two of the putative host-immunomodulatory proteins of AngHV1, namely an interleukin 10 homolog encoded by ORF25  and a protein containing a TNFR domain encoded by ORF124 , were also identified as being encoded by late genes.
Location of expression in the AngHV1 genome
A stringent summary of the kinetic classes of AngHV1 ORFs deduced from the Ri-PAA-analysis at t = 6 hpi is shown in Figure 4, with the 36 ORFs potentially compromised by 3’-coterminality and the three ORFs for which no data were obtained left blank. The immediate-early ORFs are located within the terminal direct repeats (ORF1 and ORF6A) and near the right end of the unique region (ORF127 and ORF131). The two or three immediate-early genes of IcHV1 identified in a comparable way are also located in the terminal direct repeats [13–15]. The early, early-late and late genes are seemingly distributed randomly throughout the genome.
Differences in expression kinetics of AngHV1 genes with and without inhibitors
In the present study, we classified the AngHV1 genes on the basis of their expression patterns in the presence of specific inhibitors selectively blocking the expression of early and/or late genes. This classification is not fully consistent with the clustering of genes on the basis of their expression profiles in the absence of an inhibitor. Whereas all immediate-early genes also showed unique expression profiles in cells not treated with inhibitors (IE group), and most late genes were expressed later than the other genes (L group), only half of the early and one-third of the early-late genes clustered in the E and EL groups, respectively. The latter finding may partly be explained by the incomplete blockage of the expression of late genes by the viral DNA polymerase inhibitor, but may also reflect the more complex regulation of viral gene expression during normal infection. The genes with marked differences in expression kinetics between both approaches are of interest for further functional characterization.
We have studied the kinetics of gene expression in AngHV1 by genome-wide transcription analyses using RT-qPCR. Four immediate-early genes were identified on the basis of their unique gene expression profiles in cells not treated with inhibitors, and on the basis of their unchanged or increased gene expression in the presence of a protein synthesis inhibitor. Additional characterization of these genes is required to determine their potential roles in the regulation of gene expression. On the basis of inhibition of gene expression in the presence of a viral DNA polymerase inhibitor, 17 early genes, 37 early-late genes and 68 late genes were identified. This classification broadly complied with cluster analysis of the genes based on their changes in relative gene expression in untreated samples. Our findings on the broad functions of genes assigned to different kinetic classes are in accordance with those from a more limited exercise with IcHV1, and may be extrapolated to related alloherpesviruses. Comparable to mammalian herpesviruses, most of the early and early-late genes encode proteins involved in viral DNA replication, enzymes involved in nucleic acid metabolism, and several envelope glycoproteins. Most of the late genes encode structural proteins. Hence, we suggest that, despite the virtual absence of detectable genetic similarities between the herpesvirus families, fish herpesviruses of the family Alloherpesviridae exhibit patterns of temporally regulated gene expression that are similar to those of mammalian herpesviruses in the family Herpesviridae.
The Dutch AngHV1 isolate CVI500138  was propagated in one-day old ~80% confluent eel kidney 1 (EK-1) cell monolayers . The cells were cultured in monolayers in sterile plastic culture flasks (Falcon, BD Biosciences, Bedford, MA, USA) with virus growth medium (VGM), consisting of Leibovitz’s L-15 medium (Gibco, Invitrogen by Lifetechnologies, Carlsbad, CA, USA) with 2% (v/v) fetal bovine serum (FBS, Bodinco, Alkmaar, The Netherlands), 0.075% (w/v) NaHCO3, 2 mM L-glutamine (Gibco) and antibiotics (0.012% (w/v) kanamycin (Sigma-Aldrich, St. Louis, MO, USA) and 270 IE/ml penicillin G (Astellas Pharma, Tokyo, Japan)) at 26°C in a 5% CO2-incubator (Nuaire, Plymouth, MN, USA). For virus propagation on 6-well plates (Cellstar, Greiner bio-one, Frickenhausen, Germany), 0.26% instead of 0.075% (w/v) NaHCO3 was used.
One-day old EK-1 monolayers in 6-well plates were washed once and pre-incubated for 1 h with either 5 ml of VGM, 5 ml of VGM containing 100 μg/ml protein synthesis inhibitor cycloheximide (CHX, Calbiochem, Merck, Darmstadt, Germany), or with 5 ml of VGM containing 400 μg/ml viral DNA polymerase inhibitor phosphonoacetic acid (PAA, Sigma-Aldrich). After the pre-incubation, the cells were infected with AngHV1 at a multiplicity of infection (MOI) of 10 50% tissue culture infective dose (TCID50)/cell in 2 ml of the appropriate VGM (t = 0). After a 30 min incubation period, cells were washed thrice with the appropriate VGM formulation and incubated for another 30 min, 1.5, 3.5 or 5.5 h. Infections were performed in triplicate with native VGM, and in duplicate for PAA- and CHX-containing VGM.
RNA was extracted at t = 0 (non-infected control), 1, 2, 4, and 6 h post infection (hpi). Infected cells were washed once with the appropriate VGM formulation, and cells were lysed directly in the culture dish by adding 1 ml Trizol Reagent (Invitrogen). RNA was extracted according to manufacturer’s protocol, and dissolved in 200 μl RNase-free water (Sigma-Aldrich) with 2 μl RNaseOUT recombinant ribonuclease inhibitor (Invitrogen). RNA concentration was checked by spectrophotometry using a Nanodrop ND-1000 (Thermo Fisher Scientific, MA, USA).
Potential contaminating DNA was removed by treatment with DNase I (Roche, Basel, Switzerland). Twenty units of DNase I (2 μl) were added to a maximum of 50 μg total RNA (87.5 μl), 10 μl 10× Incubation buffer and 10 units RNaseOUT, and incubated for 20 min at 31°C at 550 rpm on a thermomixer (Eppendorf, Hamburg, Germany). DNase I was inactivated by adding 2 μl 0.2 M EDTA (pH 8.0) and heating for 10 min at 75°C at 550 rpm on a thermomixer. The concentration of DNase-treated RNA in the samples was checked by spectrophotometry.
PolyA RNA was extracted using an Oligotex mRNA kit (Qiagen, Hilden, Germany). In brief, 90 μl DNase-treated total RNA was used as starting material, following the manufacturer’s instructions for the spin-column protocol. PolyA RNA was finally dissolved in 2 × 75 μl of buffer OEB at 70°C. After cooling, 1.5 μl RNaseOUT was added and the sample was stored at −80°C.
Reverse transcription (RT) was carried out using the TaqMan Reverse Transcriptase Reagent kit (Applied Biosystems by Lifetechnologies, Carlsbad, CA, USA). The total volume of RT mix prepared on ice was 100 μl per reaction, containing 10 μl RT buffer (10×), 22 μl MgCl2 (25 mM), 20 μl dNTP mixture (2.5 mM of each dNTP), 5 μl oligo dT (50 μM), 2 μl RNase Inhibitor (20 U/μl), 2.5 μl MultiScribe Reverse Transcriptase (50 U/μl), 23.5 μl DNase- and RNase-free water and 15 μl polyA RNA as template. The thermal profile of the RT program consisted of 10 min incubation at 25°C, 30 min RT at 48°C, 5 min RT inactivation at 95°C, and cooling to 4°C, and was performed in a 96-well GeneAmp PCR System 9700 (Applied Biosystems). For each polyA RNA sample, RT was carried out in duplicate, after which the cDNA was combined and diluted 1:5 in DNase- and RNase-free water and stored at −20°C.
The total volume of the SYBR Green quantitative (q)PCR mix was 20 μl per reaction, containing 10 μl SYBR Green PCR Mix (Applied Biosystems), 0.8 μl forward primer (10 μM), 0.8 μl reverse primer (10 μM), 0.25 μl Uracil-DNA Glycosylase (UDG, 5 U/μl, New England Biolabs, Ipswich, MA, USA), 3.15 μl super Q and 5 μl diluted cDNA template. The thermal profile of the SYBR Green qPCR program consisted of 10 min at 37°C, 10 min at 95°C, 40 cycles of 15 s at 95°C and 1 min at 60°C, followed by a dissociation stage from 60°C to 95°C at the end of the run, and was carried out in a 7500 Fast Real-Time PCR system (Applied Biosystems) under Standard 7500 conditions. In every qPCR run, for each time point reactions for the reference β-actin gene of European eel (Anguilla anguilla) were analysed, using the primer set described by Aroua et al..
Primers were designed for all AngHV1 ORFs, except for the newly predicted ORF57.5, ORF92A and ORF92B , using the Primer Express 3.0 program (Applied Biosystems) in the TaqMan and TaqMan MGB quantification mode, and evaluated using the Oligo Analyzer program v1.5 (Gene Link, Hawthorne, NY, USA). Primers are listed in Additional file 3: Table S3.
For all primer sets, specificity and efficiency were tested as described below. Viral DNA was extracted from purified AngHV1 virions  using the DNA blood mini kit (Qiagen) following the manufacturer’s protocol. Tenfold dilution series were prepared from AngHV1 DNA in buffer AE (Qiagen), and, for all primer sets, standard curves over four orders of magnitude were tested in triplicate. Primer sets were also checked for the formation of nonspecific reactions with host cell DNA. Primer sets were considered valid if primers did not form nonspecific products in non-template controls, and if standard curve slopes were at least −3.8. Average melting temperature (Tm-)values for each primer set were calculated from the efficiency tests. The efficiency of the β-actin reference gene primer set was determined to be 91.0% from tenfold dilution series over four orders of magnitude from cDNA from an infection trial with native VGM and VGM containing PAA or CHX at different time points post infection.
Quantitative PCR data were analysed using the Sequence Detection Software version 1.4 program (Applied Biosystems) with the Auto baseline function and a threshold of 0.05. The means of the three Ct-values for each dilution point were calculated, and the efficiency of amplification (E) of each primer set was determined from the slope of the standard curves using the Microsoft Excel 2003 program (Microsoft, Redmond, WA, USA), using the formula:
The relative expression ratio (R) was calculated for each sample using the formula modified from Pfaffl et al. by Tombácz et al.:
Esample refers to the efficiency of amplification of a particular primer set, Ct[sample max] refers to the maximal Ct-value for that particular sample during the course of infection, Ct[sample] refers to any particular sample at a given time point, Ereference refers to the efficiency of amplification of the β-actin reference gene primer set, Ct[reference max] refers to the Ct-value for the β-actin reference gene corresponding to Ct[sample max], and Ct[reference] refers to the Ct-value for the β-actin reference gene corresponding to Ct[sample]. R-values, means and standard deviations were calculated for each sample using the Microsoft Excel 2003 program. The change in relative gene expression in untreated samples was calculated by subtracting the R-value of a given time point from the previous time point:
Genes were clustered on the basis of their RΔ-values by using a complete linkage hierarchical clustering method with a centred correlation similarity metric, using the Cluster 3.0 computer program (M. Eisen, Stanford University, USA and M. de Hoon, University of Tokyo, Japan) and viewed with Alok Saldanha’s Java TreeView v1.1.6r2. RΔ-graphs of clustering genes were plotted using the Microsoft Excel program.
The inhibitory effect of CHX on gene expression (Ri-CHX) at t = 4 and t = 6 hpi and the inhibitory effect of PAA on gene expression (Ri-PAA) at t = 6 hpi were calculated using the formula of Pfaffl et al..
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The authors thank Ineke Roozenburg and Michal Voorbergen-Laarman (Central Veterinary Institute (CVI) of Wageningen UR) for technical assistance in cell and virus culture. This study received financial support from the Dutch Ministry of Economic Affairs, Agriculture and Innovation.
Steven J van Beurden
Present address: Immunology-Vaccinology (B43b), Department of Infectious and Parasitic Diseases, Faculty of Veterinary Medicine, University of Liège, Liège, 4000, Belgium
Authors and Affiliations
Central Veterinary Institute, part of Wageningen UR, P.O. Box 65, Lelystad, AB, 8200, The Netherlands
Steven J van Beurden, Ben PH Peeters & Marc Y Engelsma
Department of Infectious Diseases and Immunology, Faculty of Veterinary Medicine, Utrecht University, P.O. Box 80.165, Utrecht, TD, 3508, The Netherlands
Steven J van Beurden & Peter JM Rottier
MRC–University of Glasgow Centre for Virus Research, Glasgow, G11 5JR, UK
The authors declare that they have no competing interests.
SJvB designed the study, designed the primers, carried out the virus infections, mRNA extractions, RT, qPCR, data analyses and drafted the manuscript. BPHP and PJMR advised on the study design and manuscript. AJD provided the updated AngHV1 map (including 3’-ends), advised on results interpretation and manuscript. MYE coordinated the study, advised on the study design and manuscript. All authors read and approved the final manuscript.
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