Detection of virus mRNA within infected host cells using an isothermal nucleic acid amplification assay: marine cyanophage gene expression within Synechococcus sp
© Wharam et al; licensee BioMed Central Ltd. 2007
Received: 15 March 2007
Accepted: 06 June 2007
Published: 06 June 2007
Signal-Mediated Amplification of RNA Technology (SMART) is an isothermal nucleic acid amplification technology, developed for the detection of specific target sequences, either RNA (for expression) or DNA. Cyanophages are viruses that infect cyanobacteria. Marine cyanophages are ubiquitous in the surface layers of the ocean where they infect members of the globally important genus Synechococcus.
Here we report that the SMART assay allowed us to differentiate between infected and non-infected host cultures. Expression of the cyanophage strain S-PM2 portal vertex gene (g20) was detected from infected host Synechococcus sp. WH7803 cells. Using the SMART assay, we demonstrated that g20 mRNA peaked 240 – 360 minutes post-infection, allowing us to characterise this as a mid to late transcript. g20 DNA was also detected, peaking 10 hours post-infection, coinciding with the onset of host lysis.
The SMART assay is based on isothermal nucleic acid amplification, allowing the detection of specific sequences of DNA or RNA. It was shown to be suitable for differentiating between virus-infected and non-infected host cultures and for the detection of virus gene expression: the first reported use of this technology for such applications.
The Signal-Mediated Amplification of RNA Technology (SMART, developed by Cytocell Ltd., Banbury, UK), also referred to as CytAMP® (British BioCell International, Cardiff, UK) was originally developed for the medical diagnostics industry . Public Health Laboratory trials have compared CytAMP® with more conventional methods for the specific detection of MRSA (methicillin-resistant Staphylococcus aureus) . A review, outlining guidelines for the laboratory diagnosis and susceptibility testing of MRSA, reported that the sensitivity and specificity of CytAMP® was comparable to those of PCR for this purpose .
Here, we report the first application of this isothermal nucleic acid amplification assay for the detection of viral DNA and RNA within infected host cells. This is also the first report of the assay being used to detect gene expression.
The viruses chosen for this study were cyanophages. These are viruses that infect cyanobacteria, which are globally important photosynthetic microorganisms. Cyanophages have a wide spectrum of host ranges, are ubiquitous and can be easily isolated from a range of aquatic environments . Marine cyanophages are extremely numerous in surface seawater [6–9]. Their hosts, Synechococcus spp., are marine cyanobacteria, which also have a widespread distribution throughout the world's oceans and are thought to contribute up to 25% of primary productivity in the open ocean . There is great interest in marine cyanophages, as they are key components of microbial communities and influence host populations  and biogeochemical cycling [12–14], as well as primary productivity.
Much of the emphasis of research on marine cyanophages has focussed on the dynamics (or propagation strategy) between phage and host in situ and on determining their genetic diversities [15–20]. Until recently, very little had been reported about marine cyanophage gene expression, gene function or phage assembly apart from what could be deduced from sequence information [21–25]. However, following the discovery of photosynthetic genes in marine cyanophages [26–28], studies on their expression using microarrays  and quantitative real-time PCR , were used to help determine functionality (see review by Clokie et al ).
Cyanophage strain S-PM2 was originally isolated by plaque assay from coastal water off Plymouth, UK and belongs to the family Myoviridae, a group of double-stranded DNA phages with contractile tails. S-PM2 has been classified into a sub-group of phages termed the 'exo T-evens' based on a phylogenetic analysis of the structural components, encoded on a 10 kb module, from a range of T-even phages, . One of these structural components is the portal vertex protein (gp20). The g20 gene was originally identified in cyanophages in order to develop a PCR-based assay to analyze natural cyanophage populations .
Sequence analysis of g20 in S-PM2 revealed significant similarity to g20 from the enteric coliphage T4, therefore it is likely that the function of gp20 in S-PM2 is similar to that in T4 where it is involved in head assembly. T4 head assembly takes place in several phases and is reviewed extensively in Black et al. . Briefly, a prohead is assembled, starting from a membrane-bound initiation complex, the prohead then undergoes proteolysis and is detached from the membrane. The head is then packaged with DNA and final maturation steps occur. At the membrane attachment (proximal) vertex of the prohead shell, there is a dodecameric ring of gp20 protein, termed connector or portal protein. Formation of this structure is essential, and is thought to be the rate-limiting step in T4 prohead initiation. The prohead portal proteins do not undergo proteolysis (as opposed to other prohead proteins which do) and they form the site at which the tail is attached and through which DNA will eventually pass.
The g20 gene is now widely used as a marker to study the diversity and population dynamics of both marine and freshwater cyanophage [19, 20, 33–38]. Despite such wide scale exploitation of the g20 gene sequence, there have been no previous studies on cyanophage g20 gene expression.
Sequence information from cyanophage g20 was used to develop a set of probes designed for use in the SMART isothermal nucleic acid amplification technology. We have previously reported that the assay discriminated between similar g20 target DNA sequences from two different marine cyanophage strains . Earlier trials also showed the assay, as well as detecting DNA targets, could generate signals from specific RNA (using E. coli as a model target organism and a high copy number ribosomal RNA as the target sequence) . The assay conditions are identical, regardless of whether an RNA or DNA target is to be detected.
Here we report that we can detect cyanophage strain S-PM2 g20 mRNA from infected Synechococcus sp. WH7803 using a technology based on isothermal nucleic acid amplification. In addition, the SMART assay was used to monitor g20 expression and the subsequent increase in cyanophage DNA in the infected culture. This is the first use of the assay in looking at gene expression, and in detecting viral nucleic acid in an infected host. It is also the first study looking at cyanophage g20 gene expression.
Results and discussion
Detection of S-PM2 g20 mRNA from infected host cells
Oligonucleotide probe sequences used in this study.
S-PM2 g20 coding strand
S-PM2 g20 non-coding strand
A preliminary experiment was performed to determine whether SMART could detect viral RNA from an infected culture. In order to detect S-PM2 g20 mRNA from infected host cells, RNA and DNA were extracted from infected Synechococcus sp. WH7803 approximately 24 hours prior to lysis, when viral RNA was predicted to be detectable. Nucleic acid was also extracted from an uninfected culture, for use in controls.
Studying g20 gene expression during the cyanophage infection cycle
Cyanophage S-PM2 g20 expression was only detected at a low level up to the 240-minute post-infection (i.e. after addition of cyanophages to the host culture) time point. Despite variation in the data, S-PM2 g20 mRNA concentration increased sharply at 240-minutes post-infection, with maximum g20 mRNA detected at 260-minutes post infection (Fig. 3a). At 10 – 11 hours post-infection, g20 mRNA had dropped back to lower concentrations. g20 DNA started to increase 6-hours post-infection, to a maximum level 10-hours post-infection (Fig. 3b).
Data obtained using the SMART assay fit with what is already known about the kinetics of cyanophage infection. In cyanophage strain S-PM2 the onset of lysis occurs after a 9 hour latent period in infected Synechococcus sp. WH7803 cells . Maximum g20 expression was observed at 4 hours 20 minutes after infection (Fig. 3a), which is just under half way through the S-PM2 latent period. If compared to phage T4 infection, which has a latent period of 25 minutes , this would characterise S-PM2 g20 mRNA as a mid to late transcript. However, recent work by Clokie et al  demonstrated that S-PM2 only has 2 (early and late) classes of transcripts rather than the 3 (early, mid and late) observed in T4. In T4, late mRNA is known to direct the synthesis of phage T4 structural proteins as well as proteins that help with phage assembly and are involved in cell lysis. S-PM2, structural genes g18 and g23 were characterised as late transcripts  and their expression increased to maximum levels between 4 – 6 hours; this is consistent with S-PM2 g20 (another structural gene) expression data in figure 3 here.
Evidence from electron microscopy and other studies on T4 suggests that the prohead and mature head contain 960 copies of gp23, the major capsid protein, compared with only 12 copies of gp20. Indeed, gp20 is the least abundant of the prohead proteins compared to the others that have copy numbers of between 55 (gp24) and 576 (gp22) . If expression levels are similar in cyanophage S-PM2, it is encouraging that the SMART assay has the necessary sensitivity for detecting g20 gene expression. Therefore, it is likely that the assay would be highly suitable for future expression studies.
The increase in signal from S-PM2 g20 DNA (Fig. 3) is consistent with the continuous replication of cyanophage DNA for eventual packaging into proheads during the infection cycle . The peak of g20 DNA within the host cells 10 hours post-infection is consistent with previous observations that the onset of Synechococcus cell lysis occurs from 9 hours post-infection with the burst period continuing to 12 – 15 hours post-infection .
The SMART assay successfully differentiated between infected and non-infected host cultures and detected gene expression. SMART is a simple and sensitive assay, which may be a suitable alternative to more conventional techniques such as Northern analysis and RT-PCR for a range of applications. Also, since is it relatively simple to adapt the assay for the detection of other target sequences, it would be possible to use a set of different specific probes to simultaneously study the expression of different virus and host genes, or assay for different viruses. The equipment used is relatively simple and start up costs low, so for many applications (where there is interest in a relatively small number of genes) it could be developed as a simple alternative to the use of microarrays.
Interest in isothermal nucleic acid amplification is currently increasing. One possible future application of these techniques includes in situ work, for example for use in the identification and quantification of infected cells. The repeated rounds of high temperatures involved in thermal cycling can create problems with in situ PCR, due to cellular damage. In addition, isothermal amplification techniques are potentially more robust, and have lower energy requirements than methods involving thermal cycling. These are significant benefits for certain applications, such as developing assays for use in remote areas, or for autonomous systems with applications which might include environmental monitoring and assessing public health risks.
The SMART assay, based on isothermal nucleic acid amplification, allows the detection of specific sequences of DNA or RNA. It was shown to be suitable for differentiating between virus-infected and non-infected host cultures and for the detection of gene expression: the first reported use of this technology for such applications.
Cyanophages, host strain and media
Oligonucleotide probes synthesised by phosphoramidite chemistry using a model 380A synthesiser (Applied Biosystems, Foster City, CA, USA) and purified using standard HPLC or FPLC techniques were obtained from Oswel Research products (Southampton, UK).
The sequences of cyanophage-specific probes are listed in table 1. Probes for the S-PM2 g20 coding strand are identical to those used previously . A further set of probes was designed to detect the non-coding strand of g20. The sequences of targets, probes, and RNA signals were designed to minimise potential secondary structure, and their melting temperatures were determined, as described previously . The template probes include a hexaethylene glycol (HEG) linker molecule to reduce non-specific background signal. Sequences of probes for the amplification of signal RNA, capture and detection of SMART signal, and of synthetic product for ELOSA standard curve have all been published previously [1, 4].
Sampling infected host 24 hours prior to lysis
An exponentially growing culture of Synechococcus sp. WH7803 was split into 3 × 100 mL aliquots in sterile glass conical flasks and incubated at 25°C under constant illumination (5 to 36 microeinsteins m-2s-1). At time zero, cyanophage strain S-PM2 was added to flask 1 at a multiplicity of infection of approximately 0.1 (= 1 mL of fresh lysate); 24 hours later, the same volume of cyanophage lysate was added to flask 2; flask 3 remained uninfected as a control. Flask 1 lysed (indicated by clearing of the culture) 3 days after initial infection, therefore, we predicted that virus mRNA would be detectable in flask 2 at this time point (24-hours prior to culture lysis). RNA and DNA were extracted from the cultures sampled at this time point as described below.
Sampling to follow g20 gene expression during the cyanophage infection cycle
A 1 L culture of exponentially growing Synechococcus sp. WH7803 host cells was infected with cyanophage strain S-PM2 at a MOI of approximately 1 and incubated for 12 hours at 25°C under constant illumination. Duplicate 4 mL and 2 mL aliquots of infected cells (for RNA and DNA extraction respectively) were pelleted, snap frozen in liquid N2 then stored at -80°C at various time intervals over the 12 hour period. Frozen cell pellets were defrosted at 37°C and DNA and RNA were extracted as described below.
Extraction of viral nucleic acid from infected host cells
RNA was extracted from 4 mL of pelleted cells using a Qiagen RNeasy® Mini kit according to the manufacturer's instructions (Qiagen, West Sussex, UK). The protocol included a DNase treatment step. RNA was eluted in a final volume of 50 μL RNase-free sterile water. DNA was extracted from 2 mL of pelleted cells using a Qiagen DNeasy™ Tissue kit according to the manufacturer's instructions (Qiagen, West Sussex, UK). DNA was eluted in a final volume of 100 μL RNase-free sterile water. SMART assays [1, 4] were conducted on 5 μL target nucleic acid, as described below.
The SMART assay: isothermal amplification from specific target
Use of the SMART assay for the specific detection of cyanophage DNA has been described previously . Target DNA was added to a mixture containing 2 μL 10× transcription buffer (Ambion, Austin, TX, USA), extension probe (5 fmol), template probe (1 fmol), facilitator probes 1 and 2 (100 fmol each) and ultra-pure, sterile, RNase-free water to a final volume of 15 μL. Samples were mixed, heated at 90°C for 3 min on a PTC-200™ thermal cycler (MJ Research, Waltham, MA, USA), ramped down to 41°C (0.1°C/s) and held at this temperature for 1 h. A 5 μL volume of solution containing dNTPs (5 μM each), NTPs (2 mM each) (both from Amersham Biosciences, Aylesbury UK), 4 U Bst (3' to 5'exo-) DNA polymerase (New England Biolabs, Beverly, MA, USA) and 240 U T7 RNA polymerase (Ambion) was then added, and the reaction was incubated at 41°C for an additional 2 h.
To amplify the RNA signal further, the samples were brought to room temperature before the addition of 20 fmol RNA amplification probe, followed by a mixture containing 4.5 μL 10× transcription buffer, dNTPs (50 μM each dNTP), NTPs (2 mM each NTP), 4 U Bst (3' to 5'exo-) DNA polymerase, 160 U T7 RNA polymerase, and ultra-pure, sterile, RNAse-free water to give a final volume of 17 μL. The samples were mixed and then incubated at 37°C for 2 h. The samples could be stored at -20°C before the signals were quantified.
The SMART assay: capture and detection of the assay signal
The RNA signal was assayed by an Enzyme Linked OligoSorbent Assay (ELOSA). The RNA sequence includes regions for capture, via a biotinylated probe, and detection using a further probe linked to alkaline phosphatase (Fig. 1b). Biotinylated capture probe (0.9 pmol) and alkaline phosphatase-labelled probe (6 pmol) were added to each well of a streptavidin-coated Combiplate (Thermo Life Sciences, Hampshire, UK), in hybridisation buffer [50 mM Tris-HCl, pH 8.0, 1 M NaCl, 20 mM EDTA and 1% (w/v) BSA]. An aliquot (5–20 μL) of the sample to be quantified was then added, bringing the total volume to 150 μL per well. Samples were incubated at room temperature on a platform shaker at 300 rpm for 1 h. Unbound material was removed from wells by washing 4 times with 200 μL wash buffer [1× TBS/0.1% Tween-20], then once with 200 μL alkaline phosphatase substrate buffer (SCIL Diagnostics, Martinsried, Germany). Substrate (4-Nitrophenyl phosphate, Boehringer-Mannheim UK, Sussex, UK), at 5 mg/mL in substrate buffer, was then added (180 μL/well) and alkaline phosphatase activity was measured using a plate reader (Labsystems integrated EIA Management system, Thermo Life Sciences) pre-warmed at 37°C, reading absorbance at 405 nm every 2 minutes for 30 minutes. Rates of alkaline phosphatase activity for each sample were compared to a standard curve, generated using dilutions of a synthetic DNA oligonucleotide with the same sequence as the RNA product. This allowed the amount of RNA produced in each extension/transcription reaction to be calculated.
This study was partly funded by a Natural Environmental Research Council (NERC) CONNECT B grant, GR3/CO058, awarded jointly to W.H.W. and Cytocell Ltd.: CONNECT B is a scheme designed to encourage collaboration between academia and industry. The work described in this paper is the subject of various patents and patent applications (including EP-B-0,666.927; AU 672367; and WO 99/37806) originally held by Cytocell Ltd. UK. We gratefully acknowledge Cytocell Ltd. for allowing us to use the cyanophage infection system as a testing ground for their technology. Particular thanks go to Anthony Weston, who participated in the design of the study and Peter Marsh (both formerly of Cytocell Ltd., UK) for their advice and support during the development phase of the SMART assay.
- Wharam SD, Marsh P, Lloyd JS, Ray TD, Mock GA, Assenberg R, McPhee JE, Brown P, Weston A, Cardy DLN: Specific detection of DNA and RNA targets using a novel isothermal nucleic acid amplification assay based on the formation of a three-way junction structure. Nucleic Acids Research 2001, 29: e54. 10.1093/nar/29.11.e54PubMedPubMed CentralView ArticleGoogle Scholar
- Levi K, Bailey C, Bennett A, Marsh P, Cardy DL, Towner KJ: Evaluation of an Isothermal Signal Amplification Method for Rapid Detection of Methicillin-Resistant Staphylococcus aureus from Patient-Screening Swabs. Journal of Clinical Microbiology 2003, 41: 3187-3191. 10.1128/JCM.41.7.3187-3191.2003PubMedPubMed CentralView ArticleGoogle Scholar
- Brown DFJ, Edwards DI, Hawkey PM, Morrison D, Ridgway GL, Towner KJ, Wren MWD, on behalf of the Joint Working Party of the British Society for Antimicrobial Chemotherapy HISaICNA: Guidelines for the laboratory diagnosis and susceptibility testing of methicillin-resistant Staphylococcus aureus (MRSA). Journal of Antimicrobial Chemotherapy 2005, 56: 1000-1018. 10.1093/jac/dki372PubMedView ArticleGoogle Scholar
- Hall MJ, Wharam SD, Weston A, Cardy DLN, Wilson WH: Use of signal-mediated amplification of RNA technology (SMART) to detect marine cyanophage DNA. Biotechniques 2002, 32: 604-611.PubMedGoogle Scholar
- Suttle CA: Cyanophages and their role in the ecology of cyanobacteria. In The ecology of cyanobacteria: Their diversity in time and space. Edited by: Whitton BA, Potts M. Boston: Kluwer Academic Publishers, Boston; 2000:563-589.Google Scholar
- Suttle CA, Chan AM: Marine Cyanophages Infecting Oceanic and Coastal Strains of Synechococcus – Abundance, Morphology, Cross-Infectivity and Growth-Characteristics. Marine Ecology-Progress Series 1993, 92: 99-109.View ArticleGoogle Scholar
- Suttle CA, Chan AM: Dynamics and Distribution of Cyanophages and Their Effect On Marine Synechococcus spp. Applied and Environmental Microbiology 1994, 60: 3167-3174.PubMedPubMed CentralGoogle Scholar
- Waterbury JB, Valois FW: Resistance to Cooccurring Phages Enables Marine Synechococcus Communities to Coexist With Cyanophages Abundant in Seawater. Applied and Environmental Microbiology 1993, 59: 3393-3399.PubMedPubMed CentralGoogle Scholar
- Wilson WH, Joint IR, Carr NG, Mann NH: Isolation and molecular characterization of five marine cyanophages propagated on Synechococcus sp strain WH7803. Applied and Environmental Microbiology 1993, 59: 3736-3743.PubMedPubMed CentralGoogle Scholar
- Waterbury JB, Watson SW, Valois FW, Franks DG: Biological and ecological characterisation of the marine unicellular cyanobacterium Synechococcus . In Photosynthetic picoplankton. Volume 214. Edited by: Platt T, Li WKW. Canadian Bulletin of Fisheries and Aquatic Sciences; 1986:71-120.Google Scholar
- Hennes KP, Suttle CA, Chan AM: Fluorescently Labeled Virus Probes Show That Natural Virus Populations Can Control the Structure of Marine Microbial Communities. Applied and Environmental Microbiology 1995, 61: 3623-3627.PubMedPubMed CentralGoogle Scholar
- Fuhrman JA: Marine viruses and their biogeochemical and ecological effects. Nature 1999, 399: 541-548. 10.1038/21119PubMedView ArticleGoogle Scholar
- Hewson I, Govil SR, Capone DG, Carpenter EJ, Fuhrman JA: Evidence of Trichodesmium viral lysis and potential significance for biogeochemical cycling in the oligotrophic ocean. Aquatic Microbial Ecology 2004, 36: 1-8.View ArticleGoogle Scholar
- Wilhelm SW, Suttle CA: Viruses and Nutrient Cycles in the Sea – Viruses play critical roles in the structure and function of aquatic food webs. Bioscience 1999, 49: 781-788. 10.2307/1313569View ArticleGoogle Scholar
- Wilson WH, Fuller NJ, Joint IR, Mann NH: Analysis of cyanophage diversity and population structure in a south-north transect of the Atlantic Ocean. In Marine Cyanobacteria. Edited by: Charpy L, Larkum AWD. Monaco: Bulletin de l'Institut Oceanographique; 1999:209-216.
- Wilson WH, Fuller NJ, Joint IR, Mann NH: Analysis of cyanophage diversity in the marine environment using denaturing gradient gel electrophoresis. In Microbial Biosystems: New Frontiers Proceedings of the 8th International Symposium on Microbial Ecology. Atlantic Canada Society for Microbial Ecology. Edited by: Bell CR, Brylinsky M, Johnson-Green P. Halifax, Canada; 2000:565-570.Google Scholar
- McDaniel L, Houchin LA, Williamson SJ, Paul JH: Plankton blooms – Lysogeny in marine Synechococcus . Nature 2002, 415: 496-496. 10.1038/415496aPubMedView ArticleGoogle Scholar
- Ortmann AC, Lawrence JE, Suttle CA: Lysogeny and lytic viral production during a bloom of the cyanobacterium Synechococcus spp. Microbial Ecology 2002, 43: 225-231. 10.1007/s00248-001-1058-9PubMedView ArticleGoogle Scholar
- Zhong Y, Chen F, Wilhelm SW, Poorvin L, Hodson RE: Phylogenetic diversity of marine cyanophage isolates and natural virus communities as revealed by sequences of viral capsid assembly protein gene g20. Applied and Environmental Microbiology 2002, 68: 1576-1584. 10.1128/AEM.68.4.1576-1584.2002PubMedPubMed CentralView ArticleGoogle Scholar
- Muhling M, Fuller NJ, Millard A, Somerfield PJ, Marie D, Wilson WH, Scanlan DJ, Post AF, Joint I, Mann NH: Genetic diversity of marine Synechococcus and co-occurring cyanophage communities: evidence for viral control of phytoplankton. Environmental Microbiology 2005, 7: 499-508. 10.1111/j.1462-2920.2005.00713.xPubMedView ArticleGoogle Scholar
- Fuller NJ, Wilson WH, Joint IR, Mann NH: Occurrence of a sequence in marine cyanophages similar to that of T4 g20 and its application to PCR-based detection and quantification techniques. Applied and Environmental Microbiology 1998, 64: 2051-2060.PubMedPubMed CentralGoogle Scholar
- Hambly E, Tetart F, Desplats C, Wilson WH, Krisch HM, Mann NH: A conserved genetic module that encodes the major virion components in both the coliphage T4 and the marine cyanophage S-PM2. Proceedings of the National Academy of Sciences of the United States of America 2001, 98: 11411-11416. 10.1073/pnas.191174498PubMedPubMed CentralView ArticleGoogle Scholar
- Chen F, Lu JR: Genomic sequence and evolution of marine cyanophage P60: a new insight on lytic and lysogenic phages. Applied and Environmental Microbiology 2002, 68: 2589-2594. 10.1128/AEM.68.5.2589-2594.2002PubMedPubMed CentralView ArticleGoogle Scholar
- Mann NH, Clokie MRJ, Millard A, Cook A, Wilson WH, Wheatley PJ, Letarov A, Krisch HM: The genome of S-PM2, a "photosynthetic" T4-type bacteriophage that infects marine Synechococcus strains. Journal of Bacteriology 2005, 187: 3188-3200. 10.1128/JB.187.9.3188-3200.2005PubMedPubMed CentralView ArticleGoogle Scholar
- Sullivan MB, Coleman ML, Weigele P, Rohwer F, Chisholm SW: Three Prochlorococcus cyanophage genomes: Signature features and ecological interpretations. Plos Biology 2005, 3: 790-806. 10.1371/journal.pbio.0030144View ArticleGoogle Scholar
- Lindell D, Sullivan MB, Johnson ZI, Tolonen AC, Rohwer F, Chisholm SW: Transfer of photosynthesis genes to and from Prochlorococcus viruses. Proceedings of the National Academy of Sciences of the United States of America 2004, 101: 11013-11018. 10.1073/pnas.0401526101PubMedPubMed CentralView ArticleGoogle Scholar
- Mann NH, Cook A, Millard A, Bailey S, Clokie M: Marine ecosystems: Bacterial photosynthesis genes in a virus. Nature 2003, 424: 741-741. 10.1038/424741aPubMedView ArticleGoogle Scholar
- Sullivan MB, Lindell D, Lee JA, Thompson LR, Bielawski JP, Chisholm SW: Prevalence and evolution of core photosystem II genes in marine cyanobacterial viruses and their hosts. Plos Biology 2006, 4: 1344-1357. 10.1371/journal.pbio.0040234View ArticleGoogle Scholar
- Lindell D, Jaffe JD, Johnson ZI, Church GM, Chisholm SW: Photosynthesis genes in marine viruses yield proteins during host infection. Nature 2005, 438: 86-89. 10.1038/nature04111PubMedView ArticleGoogle Scholar
- Clokie MRJ, Shan JY, Bailey S, Jia Y, Krisch HM, West S, Mann NH: Transcription of a 'photosynthetic' T4-type phage during infection of a marine cyanobacterium. Environmental Microbiology 2006, 8: 827-835. 10.1111/j.1462-2920.2005.00969.xPubMedView ArticleGoogle Scholar
- Clokie MRJ, Mann NH: Marine cyanophages and light. Environmental Microbiology 2006, 8: 2074-2082. 10.1111/j.1462-2920.2006.01171.xPubMedView ArticleGoogle Scholar
- Black LW, Showe MK, Steven AC: Morphogenesis of the T4 Head. In Molecular Biology of Bacteriophage T4. Edited by: Karam JD, Drake JW, Kreuzer KN, Mosig G, Hall DH, Eiserling FA, Black LW, Spicer EK, Kutter E, Carlson K, Miller ES. Washington DC: American Society for Microbiology; 1994:218-258.Google Scholar
- Dorigo U, Jacquet S, Humbert JF: Cyanophage Diversity, Inferred from g20 Gene Analyses, in the Largest Natural Lake in France, Lake Bourget. Applied and Environmental Microbiology 2004, 70: 1017-1022. 10.1128/AEM.70.2.1017-1022.2004PubMedPubMed CentralView ArticleGoogle Scholar
- Marston MF, Sallee JL: Genetic Diversity and Temporal Variation in the Cyanophage Community Infecting Marine Synechococcus Species in Rhode Island's Coastal Waters. Applied and Environmental Microbiology 2003, 69: 4639-4647. 10.1128/AEM.69.8.4639-4647.2003PubMedPubMed CentralView ArticleGoogle Scholar
- Sandaa RA, Larsen A: Seasonal Variations in Virus-Host Populations in Norwegian Coastal Waters: Focusing on the Cyanophage Community Infecting Marine Synechococcus spp. Applied and Environmental Microbiology 2006, 72: 4610-4618. 10.1128/AEM.00168-06PubMedPubMed CentralView ArticleGoogle Scholar
- Short CM, Suttle CA: Nearly Identical Bacteriophage Structural Gene Sequences Are Widely Distributed in both Marine and Freshwater Environments. Applied and Environmental Microbiology 2005, 71: 480-486. 10.1128/AEM.71.1.480-486.2005PubMedPubMed CentralView ArticleGoogle Scholar
- Wang K, Chen F: Genetic diversity and population dynamics of cyanophage communities in the Chesapeake Bay. Aquatic Microbial Ecology 2004, 34: 105-116.View ArticleGoogle Scholar
- Wilhelm SW, Carberry MJ, Eldridge ML, Poorvin L, Saxton MA, Doblin MA: Marine and Freshwater Cyanophages in a Laurentian Great Lake: Evidence from Infectivity Assays and Molecular Analyses of g20 Genes. Applied and Environmental Microbiology 2006, 72: 4957-4963. 10.1128/AEM.00349-06PubMedPubMed CentralView ArticleGoogle Scholar
- Wilson WH, Carr NG, Mann NH: The effect of phosphate status on the kinetics of cyanophage infection in the oceanic cyanobacterium Synechococcus sp WH7803. Journal of Phycology 1996, 32: 506-516. 10.1111/j.0022-3646.1996.00506.xView ArticleGoogle Scholar
- Mathews CK: An overview of the T4 developmental program. In Molecular Biology of Bacteriophage T4. Edited by: Karam JD, Drake JW, Kreuzer KN, Mosig G, Hall DH, Eiserling FA, Black LW, Spicer EK, Kutter E, Carlson K, Miller ES. Washington DC: American Society for Microbiology; 1994:1-8.Google Scholar
- Black LW: DNA packaging in dsDNA Bacteriophages. In The Bacteriophages. Edited by: Calendar R. New York: Plenum Press; 1988:321-373.View ArticleGoogle Scholar
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