| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
US Department of Agriculture, Agricultural Research Service, Insect Biocontrol Laboratory, Bldg 011A, Room 214, BARC West, Beltsville, MD 20705, USA
Correspondence
D. E. Gundersen-Rindal
gundersd{at}ba.ars.usda.gov
 |
ABSTRACT |
|---|
 TOP ABSTRACT INTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
B signalling in the parasitized host. In this study, transcription of each gene was mapped by 5'- and 3'-RACE (rapid amplification of cDNA ends) and temporal and tissue-specific expression was examined in the parasitized host. For polydnavirus gene prediction in the parasitized host, no available gene prediction parameters were entirely precise. The mRNAs for each GiBV segF gene initiated between 30 and 112 bp upstream of the translation initiation codon. All were encoded in single open reading frames (ORFs), with the exception of PTP9, which was transcribed as a bicistronic message with the adjacent ank gene. RT-PCR indicated that all GiBV segF PTPs were expressed early in parasitization and, for most, expression was sustained over the course of at least 7 days after parasitization, suggesting importance in both early and sustained virus-induced immunosuppression and alteration of physiology. Tissue-specific patterns of PTP expression of GiBV segF genes were variable, suggesting differing roles in facilitating parasitism. The GenBank/EMBL/DDBJ accession number for the sequence of GiBV segment F is AY871265.
|
INTRODUCTION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
; Fleming, 1991; Gruber et al., 1996; Savary et al., 1997; Stoltz, 1990, 1993; Stoltz et al., 1986; Wyder et al., 2002). Replication from parasitoid genomic provirus DNA and packaging into virions occurs only within specialized calyx cells of the female parasitoid ovary (Theilmann & Summers, 1986; Norton & Vinson, 1983; Wyder & Lanzrein, 2003). Once injected into larval hosts as virions, PDVs infect host cells, where specific viral genes are transcribed and translated. Although the manifestations of PDV–parasitoid manipulation of host varies according to parasitoid and host insect species (Summers & Dib-Hajj, 1995), PDVs and their gene products function to regulate the larval host to favour parasitoid survival in several interrelated ways; these include suppression of host immune systems (Blissard et al., 1986; Theilmann & Summers, 1986; Asgari et al., 1997; Lavine & Beckage, 1996; Li & Webb, 1994; Cui & Webb, 1998), the inhibition of host protein synthesis (Shelby & Webb, 1994; Pennacchio et al., 1998; Vinson et al., 1998) and the regulation of host development and physiology (Lawrence & Lanzrein, 1993; Stoltz, 1993; Strand & Pech, 1995). Multiple host-regulatory functions are exerted by PDVs such that expression of PDV-encoded gene products within the pest host results ultimately in inhibition of the host immune response and development and/or alteration of physiology, enabling the parasitoid to evade encapsulation and to complete development.
The segmented genomes of both braconid and ichneumonid PDVs (BV and IV, respectively) encode genes and gene groups or families, many bearing structural resemblance to insect genes. Expression of many predicted and characterized PDV genes involves splicing of two or more exons to generate full-length mRNAs, which are then processed and translated in a fashion characteristic of their integrated eukaryotic cellular origin. Some PDV genes are encoded in single exons or open reading frames (ORFs). Numerous studies have analysed IV and BV gene transcription in parasitized lepidopteran hosts. Transcripts, genes or gene products have been identified as being involved in immunosuppression and inhibition of encapsulation (Asgari et al., 1996, 1997; Cui et al., 1997; Glatz et al., 2004; Hayakawa et al., 1994; Li & Webb, 1994; Provost et al., 2004; Strand et al., 1992; Strand, 1994; Yamanaka et al., 1996), and these gene transcripts tend to be present in largest quantities immediately upon parasitization and either decline thereafter or persist for days after parasitization. PDV genes are also involved in developmental regulation and alteration of host physiology (Béliveau et al., 2000; Johner et al., 1999; Johner & Lanzrein, 2002; Provost et al., 2004), and these gene transcripts for the most part are produced early in parasitization, although a recent study has shown certain gene transcripts from Chelonus inanitus BV (CiBV) to be present at low levels early in infection and upregulated late in parasitization (Bonvin et al., 2004). Gene transcription has also been examined for several genes of unknown function in the parasitized host (Chen et al., 2003b; Chen & Gundersen-Rindal, 2003; Volkoff et al. 2002). Transcription of viral genes from the parasitoid itself, as opposed to those within the parasitized host, has not been well studied (Bonvin et al., 2004).
Many BV genes and gene families are conserved across the BV genomes characterized to date. Our research focuses on the braconid parasitoid Glyptapanteles indiensis, a parasitoid of the lepidopteran pest Lymantria dispar (gypsy moth). The G. indiensis BV (GiBV) shares some genetic similarity with the Cotesia congregata BV (CcBV), the first BV genome to be fully sequenced (Espagne et al., 2004). Recently, a member of the GiBV protein tyrosine phosphatase family (PTP) gene family, GiBV segF PTP2 (then called PDVPTP), was identified, characterized and shown to be expressed ubiquitously in parasitized host tissues from early parasitization through to at least 8 days after parasitization (Chen et al., 2003a). Subsequently, Espagne et al. (2004) showed that PTPs comprise the largest multigene gene family in the CcBV genome, and Provost et al. (2004) characterized the family of PTPs encoded in both CcBV and Toxoneuron nigriceps (Tn) BV; these genes appear to be found in abundance in many bracoviruses. CcBV and GiBV PTPs exhibit some similarity in sequence and structure. PTPs, which are generally encoded in single ORFs in BVs, have been hypothesized to function in BVs as regulators of host signal transduction, likely having roles in alteration of host physiology (Provost et al., 2004).
Here, the focus is on GiBV genome segment F (GiBV segF), a segment predicted on the basis of nucleic and amino acid sequences to encode numerous PTPs and a single gene containing four ankyrin repeats, termed ank (Espagne et al., 2004) (also referred to as vankyrin; Kroemer & Webb, 2004). Ankyrin repeat genes have been hypothesized to have a functional role in inhibiting NF-B signalling in the parasitized host, as they have similarity to inhibitors of NF-B gene transcription factors (Kroemer & Webb, 2004). Because of our interest in analysing the roles in parasitization of existent GiBV genes versus putative or predicted GiBV genes, the validity of various gene predictors for GiBV genes was tested by analysing and mapping GiBV segF PTP and ank gene transcripts using 5'- and 3'-RACE (rapid amplification of cDNA ends) as they are transcribed early (2 h after parasitization) in the infected host. In addition, we examined temporal and tissue-specific GiBV segF gene expression by assessing transcription over time using non-quantitative RT-PCR in the parasitized host, including a time point after emergence of the parasitoid larva.
|
METHODS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
. Parasitization of gypsy moth larvae by G. indiensis was conducted by exposing an individual first instar L. dispar larva to a single G. indiensis female within a 35x10 mm Petri dish until oviposition was observed. After a single oviposition was observed, the parasitized larva was removed from the Petri dish and put into a 30 ml plastic cup with high-wheatgerm diet and incubated at room temperature. Times post-parasitization (p.p.) were calculated and recorded from the initiation of parasitization. The parasitoid embryo or larva was not removed from 2 h p.p., 24 h p.p. or 3 days p.p. individuals. The parasitoid larva was removed by dissection from 7 days p.p. individuals. The parasitoid larva had emerged from 13 days p.p. individuals. G. indiensis larvae were dissected from the parasitized host 10 days p.p. from parasitized L. dispar larvae and washed to remove host material.
Isolation and sequencing of GiBV segment DNA.
Adult female G. indiensis were dissected, reproductive tracts were isolated and fluid containing PDVs was gently released from the calyx with dissecting forceps. The fluid was collected under a dissecting microscope, avoiding eggs and ovarian tissues, and filtered through a 0·45 µm filter and PDV nucleic acid was extracted in an equal volume of extraction buffer containing 500 µg proteinase K ml–1 and 0·5 % SDS and incubated at 37 °C. Nucleic acid was gently extracted by rocking in an equal volume of phenol/chloroform according to the method of Beckage et al. (1994). GiBV segF was cloned in its entirety as described previously (Gundersen-Rindal & Dougherty, 2000). Plasmid DNA was prepared in large scale using the Quantum Prep Maxi DNA kit (Bio-Rad). Plasmid clone DNA was sequenced by a combination of primer walking and random transposon insertion using the Genome Priming System (GPS-1; New England Biolabs) followed by cycle sequencing using N, S, SP6 or T7 promoter primers and analysis on an ABI310 automatic sequencer (Applied Biosystems, Inc.). Contigs were assembled using Lasergene software (DNASTAR, Inc.). The sequence of the GiBV circular genome segment was assembled at 2x to 6x coverage and validated. The GiBV segF sequence was deposited in GenBank under accession number AY871265. GiBV segF ORFs or coding regions were predicted based on sequence analysis and genes were identified using several gene predictor programs: NCBI ORF Finder [prediction for standard genetic code, wide variety of organisms; http://www.ncbi.nlm.nih.gov/gorf/gorf.html (only large ORFs are shown)], FGENESH [ab initio gene prediction based separately on Drosophila melanogaster, Anopheles gambiae and Apis mellifera insect gene parameters; http://www.softberry.com (Salamov & Solovyev, 2000; Solovyev & Salamov, 1999)] and GENSCAN W [prediction based on human gene parameters; http://genes.mit.edu/GENSCAN.html (Burge, 1998; Burge & Karlin, 1998)] (Table 1). ORFs were searched against the sequence database (NCBI) using BLAST searches (Altschul et al., 1990, 1997) based on the amino acid sequence translations of individual ORFs.
|
5'- and 3'-RACE and cloning.
To identify 5' and 3' ends of GiBV segF genes, first-strand ‘RACE ready’ cDNAs were synthesized separately for 5'- and 3'-RACE reactions from larval RNAs 2 h p.p. using the BD SMART RACE cDNA amplification kit (BD Biosciences) with the supplied modified oligo(dT) and BD SMART II A oligonucleotide primers according to the manufacturer's instructions. Gene-specific primers were designed for 5'- and 3'-RACE second-strand cDNA synthesis reactions on the basis of NCBI ORF predictions for GiBV segF (Table 2). 5'- and 3'-RACE gene-specific products were generated with cycling conditions of 25 cycles of 94 °C for 30 s, 68 °C for 30 s and 72 °C for 3 min followed by 16 cycles of 94 °C for 30 s, 50 °C for 30 s and 72 °C for 5 min and a final elongation at 72 °C for 7 min, and examined by electrophoresis on 1 % agarose gels containing ethidium bromide. 5'-RACE products having more than one product were cloned into the pCR2.1 TOPO vector according to the protocol of the TOPO TA Cloning kit (Invitrogen). Plasmid DNA was isolated using a Quantum Prep miniprep kit (Bio-Rad) as specified by the manufacturer.
|
). Cloned products were sequenced without gel purification. Cycle-sequencing conditions were 35 cycles of 96 °C for 10 s, 50 °C for 5 s and 60 °C for 4 min. Automatic sequencing was carried out on an ABI 3100 (Applied Biosystems). 5'- and 3'-RACE product sequences were assembled (DNASTAR, SeqManII component) and compared with genomic sequences to identify features of each gene transcript.
RT-PCR.
Primers were designed to amplify the translated region of each identified GiBV segF gene (Table 2), including those predicted by insect parameters (not shown). Total RNAs from L. dispar larvae at various time points p.p. and various tissues at 7 days p.p. were treated with DNA-free (Ambion) to eliminate DNA contamination and used as templates in non-quantitative RT-PCR, which was performed according to the manufacturer's protocol using the RETROscript kit (Ambion) for two-step RT-PCR. Cycling conditions were 95 °C for 3 min, followed by 30 cycles of 94 °C for 30 s, 55 °C for 30 s and 72 °C for 2 min with a final elongation at 72 °C for 7 min. Duplicate reactions were performed using RNA templates without reverse transcription to verify the absence of contaminating viral DNA in the RNA templates. Products were separated by electrophoresis on 1 % agarose gels containing ethidium bromide and visualized on a UV transilluminator.
|
RESULTS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
; Gundersen-Rindal & Lynn, 2003). GiBV segF ORFs or coding regions were predicted based on the standard genetic code of a wide variety organisms, on D. melanogaster, Anopheles gambiae and Apis mellifera insect gene parameters and on human gene parameters (Table 1). ORFs were searched against the sequence database (NCBI) using BLAST searches (Altschul et al., 1990, 1997) based on the amino acid sequence translations of individual ORFs. All GiBV segF ORFs identified as existent had conserved sequence similarity to characterized genes, nine PTP genes and one single ankyrin repeat gene (ank) (Fig. 1). These PTPs, similarly to CcBV PTPs, were predominantly predicted to be encoded as single exons. By contrast, those based on FGENESH D. melanogaster, Anopheles gambiae and Apis mellifera were predominantly predicted to contain introns, in many cases multiple introns (Table 1). FGENESH predictions based on Drosophila suggested only three encoded genes for GiBV segF, with two containing multiple introns. FGENESH predictions based on Anopheles gambiae suggested eight genes, with seven containing at least one intron. FGENESH predictions based on Apis mellifera suggested 11 genes, with eight containing one intron. Fairly accurate gene predictions were obtained based on a wide range of organisms using standard genetic code (NCBI) or human (GENSCAN W) parameters for gene finding. GENSCAN W predictions based on human parameters predicted nine genes, two containing a single intron. A better prediction of GiBV genes, in terms of accurate gene start sites, was obtained using hymenopteran Apis mellifera parameters. However, using Apis mellifera parameters, introns were frequently predicted which did not exist in the parasitized host, as verified through RACE and RT-PCR analyses.
|
), with sequences of GiBV segF PTPs 1–9 ranging from 17·9 to 63·4 % identity at the amino acid level. GiBV genome segF was most similar in its sequence and gene organization to the characterized C1 circular genome segment of CcBV, which has been shown to encode eight PTPs and three EP1-like genes, but no ankyrin repeat genes (Espagne et al., 2004; Provost et al., 2004). At the amino acid level, GiBV segF PTP1 was most closely related to the CcBV C1 PTPB, GiBV segF PTP2 to CcBVC1 PTPQ, GiBVsegF PTP3 to CcBVC1 PTPP, GiBV segFPTP4 to CcBV C1 PTPP and PTPQ and GiBV segF PTP5 to CcBV C1 PTPM; GiBV segF PTP6 and PTP7 were both most closely related to CcBV C1 PTPI. The GiBV segF PTPs 8 and 9 were most closely related to CcBV PTPN and PTPC, respectively, which both originated from a different CcBV circular genome segment, C10.
|
). 5'-RACE products included the region from the nested 5' gene-specific primer to the gene translation start site plus the 5'-UTR or leader sequence and were of the approximate sizes expected. 3'-RACE products included the region from the nested 3' gene-specific primer to the translation stop site plus the 3'-UTR, terminating in a poly(A) tail, and were also of the approximate size expected. Occasional faint and likely non-specific products were observed in 5'-RACE reactions. 5'-RACE reactions for two predicted genes, PTP7 and ank, yielded two visible products of different sizes (Fig. 2a). 3'-RACE products yielded single amplification products for each predicted gene (Fig. 2b). All RACE products were sequenced, assembled and analysed for gene hallmarks.
|
b). For most GiBV segF genes, promoter sequences were predicted with high confidence within the 40 bp immediately upstream of the sites of transcription initiation (Neural Network promoter prediction; http://www.fruitfly.org/seq_tools/promoter), although promoter sequences were not predicted for every gene within such close proximity of the transcription initiation sites.
|
) located 12 bp downstream of the consensus poly(A) signal. Data from 5'- and 3'-RACE indicate the PTP9 and ank are transcribed together before processing. RACE data using multiple gene-specific primers indicate that the ank repeat gene is also transcribed independently (Fig. 3a, b), whereas PTP9 is transcribed only as a bicistronic message with ank. GiBV segF PTP genes 1–8 were all mapped as described, but details are shown only for PTP9. The existence of predicted gene 7 (14993–14766), a 76 amino-acid-encoding gene predicted by FGENESH based on Anopheles gambiae (and also by NCBI ORF Finder), and predicted gene 10 (15093–15116 joined to 15672–15800), a 51 amino acid-encoding gene predicted by FGENESH based on Apis mellifera, were shown to be non-existent in the parasitized host by 5'- and 3'-RACE analysis using primers specific for these regions (data not shown). Products of the incorrect size were amplified from parasitized L. dispar RNA in 3'-RACE, the sequences of which were not GiBV-related and were likely the result of non-specific amplification. Overall comparison of actually transcribed GiBV segF genes with those predicted by the various gene-finding programs showed that no predictor of GiBV genes was entirely precise. It is quite possible that predicted genes are existent but transcribed only in the parasitoid.
GiBV segF gene temporal and tissue-specific expression patterns
In a previous study (Chen et al., 2003a), we used quantitative RT-PCR to detect GiBVsegF PTP2 gene expression in tissues of parasitized L. dispar larvae within 2 h of parasitization, followed by a decline after 8 days. Here we used non-quantitative RT-PCR with gene-specific RT-PCR primers to look at expression patterns for the nine existent GiBV segF PTPs and the single ankyrin repeat gene. Using gene-specific primers designed for RT-PCR to amplify all or most of each gene identified in GiBV segF, temporal expression patterns in the parasitized host were assessed (Fig. 4). The absence of contaminating DNA in RNA samples was verified by inclusion of templates that were DNase-treated but not reverse-transcribed (shown only for 2 h p.p.). Amplified product was generated for GiBVsegF PTPs 1–9 and ank throughout parasitization, with the exception of PTP4, for which product was not detected at 7 and 13 days p.p. The presence of product 13 days p.p. and after emergence of the parasitoid suggested that GiBV gene transcripts remain at a very low level in the parasitized host even after their role has been served in parasitization. Amplification with specific L. dispar actin gene primers verified the presence of sufficient template for non-parasitized samples. Because gene predictors for GiBV segF based on Anopheles gambiae, Apis mellifera and human parameters had predicted PTP1/PTP2 and/or ank/PTP9 to be spliced genes containing two exons with an intervening intron, we used specific primers for RT-PCR in combinations ptp1F/ptp2R1 and ptp9F1/ankR to assess the presence of the larger transcripts. No product was amplified for ptp1/ptp2R1 (data not shown). The larger product was amplified using ptp9F1/ankR, indicating the presence of detectable longer transcript in the parasitized host, too large to possess the intron of 278 bp predicted using Apis mellifera parameters. No product was detected in control reactions using tissue from non-parasitized hosts or in reactions using RNA templates that were not reverse-transcribed (not shown).
|
). Only GiBV segF PTP3 and the ank gene yielded detectable product from haemocytes at 7 days p.p. GiBV segF PTPs 1, 2, 3 and 7 yielded detectable product from midgut at 7 days p.p. All GiBV segF PTPs except PTP1 and PTP4 were detected from fat body at 7 days p.p., while all but PTP4 were detected from nervous tissue.
|
|
DISCUSSION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
) found that human parameters predicted exons and introns of one CiBV gene (CiV14g1) with 100 % accuracy, but did not recognize another (CiV14g2). Collectively, the few BV gene transcripts mapped and verified to date indicate that gene-prediction and gene-calling accuracy based on currently available parameters is gene-dependent. Until PDV-trained gene predictors are available, gene existence in PDVs will need to be verified in parasitized host and parasitoid, especially since, unlike most viral genes, large percentages of PDV genes (69 % of CcBV genes reported by Espagne et al., 2004) are predicted to contain introns.
The existence of predicted genes in GiBV segF was verified by transcript mapping using 5'- and 3'-RACE, which also identified sites of transcription initiation for the ten expressed genes, nine members of the PTP gene family and one ankyrin repeat gene, and defined their parameters. The nine PTPs were diverse in sequence, as evidenced by their catalytic core amino acid sequences (Table 3). Gene transcription occurred bidirectionally from the circular segment, with PTPs 1–4 transcribed in clockwise orientation, and the remaining genes in anti-clockwise orientation relative to the segment origin. The absence of introns was confirmed for each GiBV segF PTP, with the exception of PTP9, which was transcribed as a bicistronic message with the ankyrin repeat gene, ank. Ank was also transcribed independently of PTP9. The presence of transcript for each GiBV segF gene was assessed in the parasitized host using non-quantitative RT-PCR, where amplified product was detected at 2 h p.p. and over the course of parasitization and parasitoid development for each, with the exception of PTP4, which was detected only up to 3 days p.p., indicating both early and sustained expression of these genes throughout the course of parasitism.
Tissue-specific expression of the GiBV segF PTP and ank genes in the parasitized L. dispar host was examined at 7 days p.p. CcBV tissue-specific PTP expression patterns in the parasitized host Manduca sexta at 12 or 24 h p.p. in infection and parasitization had previously been assessed, with the finding that certain CcBV PTPs were expressed ubiquitously, while others were expressed in certain host tissues (Provost et al., 2004). At 7 days p.p., much later in the course of parasitism than was assessed in the CcBV system, GiBV gene tissue-specific expression patterns were somewhat variable. Very little GiBV gene expression was detected in host haemocytes or in midgut tissue. This suggested perhaps that any involvement of these particular GiBV PTPs in signal transduction pathways controlling haemocyte immune cells and the encapsulation processes of the host immune system functions may have been required immediately and through early infection, but may not have been sustained once the parasitoid embryo reached the 7 day p.p. time point. For PDVs in general, midgut has not usually been regarded as a site for functional PDV host-impairing activity, although certain PTPs may function at some level in this host tissue. For most PTPs, early and sustained expression was expected, as had been observed in the previous study using quantitative RT-PCR to detect sustained expression of GiBVsegF PTP2 in several tissues of parasitized L. dispar larvae within 2 h p.p., which started to decline by 8 days p.p. Several GiBV segF PTP genes (PTP2, 3 and 7) were expressed ubiquitously and expression was sustained for longer than 7 days p.p. The tissue-specific expression patterns of GiBV segF PTPs were sometimes, but not always, consistent with the tissue-specific expression patterns of their most closely related CcBV PTP, although differing time points p.p. for assessment, differing methods for assessment and differing BV–host systems could easily have accounted for discrepancy. The unexpected presence of some detectable PTP RT-PCR products 13 days p.p. (a time point occurring after emergence of the parasitoid) suggested that certain GiBV gene transcripts may have remained at low levels in the parasitized host even after their physiological role(s) in parasitism had been served. It is tempting to speculate that sustained detection of GiBV segF transcripts could relate to potential integration of this genome segment in vivo, as GiBV segF DNA has previously been demonstrated by this laboratory to integrate into chromosomal DNA of cultured lepidopteran cells. It is also interesting to note that certain GiBV PTPs possessed imperfect core catalytic (HC motif) regions, for example GiBV segF PTP5, this region being essential for protein tyrosine phosphatase activity. The CcBV PTP to which GiBV PTP5 is most closely related, CcBV PTPM, is also mutated in the catalytic core region and was shown to lack phosphatase activity (Provost et al., 2004). Since in both BV systems these PTPs are expressed in host tissues during the course of parasitism, it is likely that they do serve a function in parasitism, which may be quite distinct from other BV PTP activities.
The high allocation of coding sequence of GiBV and other BVs to members of the PTP gene family is undoubtedly related to their importance in signal transduction pathways used to control cellular protein phosphorylation in the regulation of host physiological processes, protein synthesis and immunosuppressive functions that ensure parasitoid survival. These roles may be wide-ranging and variable and may occur at various regulatory levels, including gene transcription and cell division. Dephosphorylation of proteins is a common mechanism among eukaryotes for regulation of cellular processes, where PTPs play critical roles in the reversible phosphorylation of proteins involved in several biochemical and signalling pathways and regulate tyrosine phosphorylation during cellular events such as proliferation, cell signalling and oncogenic transformations (Neel & Tonks, 1997). While BV PTPs will undoubtedly be found to be critical to host regulation, no precise functional role has been assessed or demonstrated to date for any identified PTP in any BV–host system. Certainly, collective expression data suggest that BV-encoded PTP genes are important regulators for early events in parasitized hosts and may serve a role(s) throughout the course of endoparasitoid development. PTPs may be equally important in disrupting signal transduction pathways controlling immune encapsulation and other vital processes. The precise, and perhaps multiple, functional roles for BV PTPs in the alteration of host processes remain to be explored.
|
ACKNOWLEDGEMENTS |
|---|
|
REFERENCES |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
Altschul, S. F., Madden, T. L., Schäffer, A. A., Zhang, J., Zhang, Z., Miller, W. & Lipman, D. J. (1997). Gapped BLAST and PSI-BLAST: a new generation of protein database search programs. Nucleic Acids Res 25, 3389–3402.
Asgari, S., Hellers, M. & Schmidt, O. (1996). Host haemocyte inactivation by an insect parasitoid: transient expression of a polydnavirus gene. J Gen Virol 77, 2653–2662.
Asgari, S., Schmidt, O. & Theopold, U. (1997). A polydnavirus-encoded protein of an endoparasitoid wasp is an immune suppresser. J Gen Virol 78, 3061–3070.[Abstract]
Beckage, N. E., Tan, F. F., Schleifer, K. W., Lane, R. D. & Cherubin, L. (1994). Characterization and biological effects of Cotesia congregata polydnavirus on host larvae of the tobacco hornworm, Manduca sexta. Arch Insect Biochem Physiol 26, 165–195.[CrossRef]
Béliveau, C., Laforge, M., Cusson, M. & Bellemare, G. (2000). Expression of a Tranosema rostrale polydnavirus gene in the spruce budworm, Choristoneura fumiferana. J Gen Virol 81, 1871–1880.
Bell, R. A., Owens, C. D., Shapiro, M. & Tardif, J. R. (1981). Development of mass-rearing technology. In The Gypsy Moth: Research Toward Integrated Pest Management, USDA Technical Bulletin no. 1584, pp. 599–633. Edited by C. C. Doane & M. L. McManus. Washington, DC: US Department of Agriculture.
Blissard, G. W., Vinson, S. B. & Summers, M. D. (1986). Identification, mapping, and in vitro translation of Campoletis sonorensis virus mRNAs from parasitized Heliothis virescens larvae. J Virol 57, 318–327.
Bonvin, M., Kojic, D., Balnk, F., Annaheim, M., Wehrle, I., Wyder, S., Kaeslin, M. & Lanzrein, B. (2004). Stage-dependent expression of Chelonus inanitus polydnavirus genes in the host and the parasitoid. J Insect Physiol 50, 1015–1026.[Medline]
Burge, C. B. (1998). Modeling dependencies in pre-mRNA splicing signals. In Computational Methods in Molecular Biology, pp. 127–163. Edited by S. Salzberg, D. Searls & S. Kasif. Amsterdam: Elsevier Science.
Burge, C. B. & Karlin, S. (1998). Finding the genes in genomic DNA. Curr Opin Struct Biol 8, 346–354.[CrossRef][Medline]
Chen, Y. P. & Gundersen-Rindal, D. E. (2003). Morphological and molecular characterization of the polydnavirus in the parasitoid wasp Glyptapanteles indiensis (Hymenoptera: Braconidae). J Gen Virol 84, 2051–2060.
Chen, Y. P., Taylor, P. B., Shapiro, M. & Gundersen-Rindal, D. E. (2003a). Quantitative expression analysis of a Glyptapanteles indiensis polydnavirus protein tyrosine phosphatase gene in its natural lepidopteran host, Lymantria dispar. Insect Mol Biol 12, 271–280.[CrossRef][Medline]
Chen, Y. P., Higgins, J. A. & Gundersen-Rindal, D. E. (2003b). Quantification of a Glyptapanteles indiensis polydnavirus gene expressed in its parasitized host, Lymantria dispar, by real-time quantitative RT-PCR. J Virol Methods 114, 125–133.[CrossRef][Medline]
Cui, L. & Webb, B. A. (1998). Relationships between PDV genomes and viral gene expression. J Insect Physiol 44, 785–793.[CrossRef][Medline]
Cui, L., Soldevila, A. & Webb, B. A. (1997). Expression and hemocyte-targeting of a Campoletis sonorensis polydnavirus cysteine-rich gene in Heliothis virescens larvae. Arch Insect Biochem Physiol 36, 251–271.[CrossRef][Medline]
Espagne, E., Dupuy, C., Huguet, E., Cattolico, L., Provost, B., Martins, N., Poirie, M., Periquet, G. & Drezen, J.-M. (2004). Genome sequence of a polydnavirus: insights into symbiotic virus evolution. Science 306, 286–289.
Fleming, J. G. W. (1991). The integration of polydnavirus genomes in parasitoid genomes: implications for biocontrol and genetic analyses of parasitoid wasps. Biol Control 1, 127–135.
Fleming, J. G. W. & Summers, M. D. (1986). Campoletis sonorensis endoparasitic wasps contain forms of C. sonorensis virus DNA suggestive of integrated and extrachromosomal polydnavirus DNAs. J Virol 57, 552–562.
Glatz, R., Roberts, H. L., Li, D., Sarjan, M., Theopold, U. H., Asgari, S. & Schmidt, O. (2004). Lectin-induced haemocyte inactivation in insects. J Insect Physiol 50, 955–963.[Medline]
Gruber, A., Stettler, P., Heiniger, P., Schumperli, D. & Lanzrein, B. (1996). Polydnavirus DNA of the braconid wasp Chelonus inanitus is integrated in the wasp's genome and excised only in later pupal and adult stages of the female. J Gen Virol 77, 2873–2879.
Gundersen-Rindal, D. & Dougherty, E. M. (2000). Evidence for integration of Glyptapanteles indiensis polydnavirus DNA into the chromosome of Lymantria dispar in vitro. Virus Res 66, 27–37.[CrossRef][Medline]
Gundersen-Rindal, D. E. & Lynn, D. E. (2003). Polydnavirus integration in lepidopteran host cells in vitro. J Insect Physiol 49, 453–462.[CrossRef][Medline]
Hayakawa, Y., Yazaki, K., Yamanaka, A. & Tanaka, T. (1994). Expression of polydnavirus genes from the parasitoid wasp Cotesia kariyai in two noctuid hosts. Insect Mol Biol 3, 97–103.[Medline]
Johner, A. & Lanzrein, B. (2002). Characterization of two genes of the polydnavirus of Chelonus inanitus and their stage-specific expression in the host Spodoptera littoralis. J Gen Virol 83, 1075–1085.
Johner, A., Stettler, P., Gruber, A. & Lanzrein, B. (1999). Presence of polydnavirus transcripts in an egg–larval parasitoid and its lepidopterous host. J Gen Virol 80, 1847–1854.[Abstract]
Kroemer, J. A. & Webb, B. A. (2004). Polydnavirus genes and genomes: emerging gene families and new insights into polydnavirus replication. Annu Rev Entomol 49, 431–456.[CrossRef][Medline]
Lavine, M. D. & Beckage, N. E. (1996). Temporal pattern of parasitism-induced immunosuppression in Manduca sexta larvae parasitized by Cotesia congregata. J Insect Physiol 42, 41–51.
Lawrence, P. O. & Lanzrein, B. (1993). Hormonal interactions between insect endoparasites and their host insects. In Parasites and Pathogens of Insects, vol. 1, pp. 59–86. Edited by N. E. Beckage, S. N. Thompson & B. A. Federici. San Diego: Academic Press.
Li, X. & Webb, B. A. (1994). Apparent functional role for a cysteine-rich polydnavirus protein in suppression of the insect cellular immune response. J Virol 68, 7482–7489.
Neel, B. G. & Tonks, N. K. (1997). Protein tyrosine phosphatases in signal transduction. Curr Opin Cell Biol 9, 193–204.[CrossRef][Medline]
Norton, W. N. & Vinson, S. B. (1983). Correlating the initiation of virus replication with a specific pupal developmental phase of an ichneumonid parasitoid. Cell Tissue Res 231, 387–398.[Medline]
Pennacchio, F., Falabella, P. & Vinson, S. B. (1998). Regulation of Heliothis virescens prothoracic glands by Cardiochiles nigriceps polydnavirus. Arch Insect Biochem Physiol 38, 1–10.
Provost, B., Varricchio, P., Arana, E. & 10 other authors (2004). Bracoviruses contain a large multigene family coding for protein tyrosine phosphatases. J Virol 78, 13090–13103.
Salamov, A. A. & Solovyev, V. V. (2000). Ab initio gene finding in Drosophila genomic DNA. Genome Res 10, 516–522.
Savary, S., Beckage, N., Tan, F., Periquet, G. & Drezen, J.-M. (1997). Excision of the polydnavirus chromosomal integrated EP1 sequence of the parasitoid wasp Cotesia congregata (Braconidae, Microgastinae) at potential recombinase binding sites. J Gen Virol 78, 3125–3134.[Abstract]
Shelby, K. S. & Webb, B. A. (1994). Polydnavirus infection inhibits synthesis of an insect plasma protein, arylphorin. J Gen Virol 75, 2285–2292.
Solovyev, V. V. & Salamov, A. A. (1999). INFOGENE: a database of known gene structures and predicted genes and proteins in sequences of genome sequencing projects. Nucleic Acids Res 27, 248–250.
Stoltz, D. B. (1990). Evidence for chromosomal transmission of polydnavirus DNA. J Gen Virol 71, 1051–1056.
Stoltz, D. B. (1993). The polydnavirus life cycle. In Parasites and Pathogens of Insects, vol. 1, pp. 167–187. Edited by N. E. Beckage, S. N. Thompson & B. A. Federici. San Diego: Academic Press.
Stoltz, D. B., Guzo, D. & Cook, D. (1986). Studies on polydnavirus transmission. Virology 155, 120–131.[CrossRef][Medline]
Strand, M. R. (1994). Microplitis demolitor polydnavirus infects and expresses in specific morphotypes of Pseudoplusia includens haemocytes. J Gen Virol 75, 3007–3020.
Strand, M. R. & Pech, L. L. (1995). Immunological basis for compatibility in parasitoid-host relationships. Annu Rev Entomol 40, 31–56.[CrossRef][Medline]
Strand, M. R., McKenzie, D. I., Grassl, V., Dover, B. A. & Aiken, J. M. (1992). Persistence and expression of Microplitis demolitor polydnavirus in Pseudoplusia includens. J Gen Virol 73, 1627–1635.
Summers, M. D. & Dibb-Hajj, S. (1995). Polydnavirus-facilitated endoparasite protection against host immune defenses. Proc Natl Acad Sci U S A 92, 29–36.
Theilmann, D. A. & Summers, M. D. (1986). Molecular analysis of Campoletis sonorensis virus DNA in the lepidopteran host Heliothis virescens. J Gen Virol 67, 1961–1969.
Vinson, B. S., Malva, C., Varricchio, P., Sordetti, R., Falabella, P. & Pennacchio, F. (1998). Prothoracic gland inactivation in Heliothis virescens (F.) (Lepidoptera: Noctuidae) larvae parasitized by Cardiochiles nigriceps Viereck (Hymenoptera: Braconidae). J Insect Physiol 44, 845–857.[CrossRef][Medline]
Volkoff, A.-N., Béliveau, C., Rocher, J., Hilgarth, R., Levasseur, A., Duonor-Cérutti, M., Cusson, M. & Webb, B. A. (2002). Evidence for a conserved polydnavirus gene family: ichnovirus homologs of the CsIV repeat element genes. Virology 300, 316–331.[CrossRef][Medline]
Wyder, T. & Lanzrein, B. (2003). Ovary development and polydnavirus morphogenesis in the parasitic wasp Chelonus inanitus. II. Ultrastructural analysis of calyx cell development, virion formation and release. J Gen Virol 84, 1151–1163.
Wyder, S., Tschannen, A., Hochuli, A., Gruber, A., Saladin, V., Zumbach, S. & Lanzrein, B. (2002). Characterization of Chelonus inanitus polydnavirus segments: sequences and analysis, excision site and demonstration of clustering. J Gen Virol 83, 247–256.
Yamanaka, A., Hayakawa, Y., Noda, H., Nakashima, N. & Watanabe, H. (1996). Characterization of polydnavirus-encoded mRNA in parasitized armyworm larvae. Insect Biochem Mol Biol 26, 529–536.[CrossRef][Medline]
Received 8 July 2005;
accepted 1 November 2005.
This article has been cited by other articles:
|
|
 |
|
  Y.-F. Chen, M. Shi, F. Huang, and X.-x. Chen Characterization of two genes of Cotesia vestalis polydnavirus and their expression patterns in the host Plutella xylostella J. Gen. Virol., December 1, 2007; 88(12): 3317 - 3322. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 R. Lapointe, K. Tanaka, W. E. Barney, J. B. Whitfield, J. C. Banks, C. Beliveau, D. Stoltz, B. A. Webb, and M. Cusson Genomic and Morphological Features of a Banchine Polydnavirus: Comparison with Bracoviruses and Ichnoviruses J. Virol., June 15, 2007; 81(12): 6491 - 6501. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
