A regulatable transgene expression system for cultured Plasmodium falciparum parasites
© Epp et al; licensee BioMed Central Ltd. 2008
Received: 25 February 2008
Accepted: 20 May 2008
Published: 20 May 2008
The ability to transfect and create transgenic cultured malaria parasites has transformed the study of Plasmodium falciparum over the last decade. With the completion of the annotated genome sequence, the process of gene discovery now routinely includes gene knockouts, over-expression and complementation analysis. However, while this technology has proven extremely valuable, significant limitations exist. In particular, P. falciparum DNA is often unstable and difficult to clone because of its AT-rich, repetitive nature. As a result, transgene expression constructs can be difficult to assemble due to the need to include two expression cassettes on a single plasmid, one to drive expression of the transgene of interest and a second for expression of the selectable marker. In addition, transgene expression levels are usually not regulatable, making it difficult to assess phenotypes that are sensitive to the amount of protein expressed.
A plasmid based system for transgene expression is described that uses a single, bidirectional promoter to drive expression of both the transgene and the selectable marker, thus greatly reducing the size of the construct and enhancing stability. Further, by altering the concentration of drug used for selection, it is possible to modulate the copy number of the concatameric episomes and thereby regulate the expression level of the transgene through a range greater than 10 fold.
The transgene expression system described here should prove useful for both routine protein over-expression and complementation experiments as well as for experiments in which precisely manipulating the expression level of candidate proteins is desirable. This should provide an additional level of precision to the tools used to study the molecular biology of malaria parasites.
Over a decade ago, the first transfections and genetic manipulations of malaria parasites were accomplished [1–3], ushering in a new era in the study of the molecular biology and biochemistry of both human and rodent parasites. Since then, numerous studies have been published utilizing transfection to both knockout various genes as well as to over-express modified transgenes to investigate such aspects of parasite biology as mechanisms of drug resistance and protein trafficking[4, 5]. Combined with the release of the annotated genome sequences of numerous parasite species as well as several different isolates of Plasmodium falciparum, there have been unprecedented recent advances in gene discovery in malaria parasites. Thus the development of the current tools used to genetically manipulate parasites continues to contribute substantially to the understanding of the basic biology of malaria.
While the ability to genetically manipulate cultured P. falciparum parasites has proven to be extremely useful, the tools that are currently used have several limitations. For example, all systems for transfecting cultured parasites are based on circular plasmids that are initially created and produced using transformed Escherichia coli. These plasmids are then introducing into cultured parasites. The requirement that all constructs must first transition through E. coli necessitates that the parasite DNA sequences included on the plasmids be stably replicated by the bacteria, a property that many sequences lack due to the extremely AT-rich, repetitive nature of the P. falciparum genome, particularly in non-coding regions. This difficulty is especially pronounced when trying to over-express transgenes from episomal constructs which require two separate cassettes, the first containing the transgene to be expressed, the second containing the selectable marker, and both requiring separate promoter and terminator elements. Such constructs must, therefore, contain several lengthy stretches of P. falciparum DNA and stability in E. coli can be a significant issue.
A second limitation for parasite transgene expression regards the inability to control and manipulate the expression level of the gene of interest. Currently, the level of expression is a result of the copy number of the episomal plasmid as well as the strength of the promoter driving transcription of the transgene. These two parameters are determined by the DNA sequences included in the plasmid and therefore can only be changed by making substantial alterations to the construct and repeating the transfection. The ability to regulate expression levels directly within transfected parasites would provide an additional layer of control and allow researchers to investigate phenotypes resulting from different amounts of expressed protein. Recently, several systems have been described which allow the regulation of gene expression, e.g. via Atc-inducible system, the use of a protein destabilization domain or ribozymes. However, due to the complexity of these systems their utility for widespread use in malaria research remains to be proven.
A new system for transgene expression is described here that addresses some of the limitations mentioned above. By utilizing DNA sequences that contain bidirectional promoter activity, expression constructs were created that use a single stretch of P. falciparum intergenic sequence to drive expression of both a transgene as well as a selectable marker, resulting in a smaller, more stable plasmid. Second, by using the blasticin-S-deaminase selectable marker and altering the concentration of blasticidin used for selection, it is possible to tightly control and manipulate the copy number of episomes carried by the parasites. In turn this leads to controlled levels of transgene expression, thus providing a novel manipulatable expression system for cultured P. falciparum parasites. This system should prove valuable for studies that employ over-expression to determine protein function or localization, as well as in complementation experiments used to validate knockout phenotypes.
Plasmodium falciparum culture and transfection
All experiments utilized the P. falciparum NF54 line cultivated at 5% haematocrit in RPMI 1640 medium, 0.5% Albumax II (Invitrogen, Carlsbad, California, United States), 0.25% sodium bicarbonate, and 0.1 mg/ml gentamicin. Parasites were incubated at 37°C in an atmosphere of 5% oxygen, 5% carbon dioxide, and 90% nitrogen. Parasites were transfected by using "DNA loaded" red blood cells as previously described. Briefly, 0.2 cm electroporation cuvettes were loaded with 0.175 ml of erythrocytes and 50 μg of plasmid DNA in incomplete cytomix solution. Electroporation conditions were 0.31 kV and 960 mFD. For stable transfections, parasites were cultured in media containing either 40 ng/ml WR99210 or the designated concentration of blasticidin.
Construction of pHLIDH constructs: Plasmids pVLH and pVLHIDH were described previously. The luciferase coding region and hrp2 3'UTR of pVLH were amplified by PCR introducing restriction sites for Pst I (5') and Kpn I (3') using the primers FflucPstI: 5'-AACTGCAGGCATGGAAGACGCCAAAAAC-3' and hrp3'downKpnI: 5'-GGGGTACCCGCCTCTCCCCGCGCGTTGG-3'. Subsequently, this fragment was ligated into Pst I/Kpn I digested pVLHIDH to replace the VLH portion (var promoter, luciferase and hrp2 3'UTR) to yield plasmid pHLIDH. In the resulting plasmid, the PFB1055c intron acts as a promoter for both the reporter and drug resistance genes. Additional intron sequences were first amplified from genomic DNA with the following primers, thereby adding the restriction sites BamH I and Sal I to the 5' and 3'ends, respectively, and inserted into BamH I/Sal I digested pHLIRH. Gene specific primers for var introns: PFC0005w: 5'-CGGGATCCGAAGGTAAAAGAGAATATATATGTG-3'/5'-GCGTCGACTTCTAAAATAATAAAAGAGG-3'; PFF0845c: 5'-CGGGATCCCTAAAGGTATTATATATG-3'/5'-GCGTCGACGATCAATAGTAGATTTGG-3'; PFD0020c: 5'-CGGGATCCGCGCTTTTATTTTTGAAGG-3'/5'-GCGTCGACGGTCCACAGGAGATTTAGG-3'. For the construction of pHLsti/CamDH, the intron in pHLIDH (Sma I and Sal I) was replaced with the PfCam promoter from pHH-Tati2 construct (Hpa I and Sal I) (gift of M. Meissner).
Contruction of pHBIRH vectors: Luciferase gene was cut out pHLIRH with Hind III and Sma I and replaced with the blasticidin S deaminase gene obtained by restriction digestion of pVcBB/IDH with Hind III and Hpa I. Restriction sites BamH I and Sal I were used to exchange bidirectional promoters between plasmids pHLIDH, pHLIRH and pHBIRH.
Renilla and firefly luciferase assays
Parasites were synchronized by magnetic cell separation using MACS CS columns (Miltenyi Biotech) and confirmed by light microscopy. Parasitaemias were counted for 1000 RBCs. For luciferase assays, parasites were obtained from 200 μl of culture by centrifugation and subsequent lysis in 100 μl of Glo Lysis Buffer (Promega). To determine firefly luciferase expression, 100 μl of Bright-Glo Luciferase reagent was added to the lysate and luminescence was measured immediately in a TD-20/20 luminometer. For Renilla luciferase expression, 100 μl Renilla assay reagent (Promega) was added to the lysate and luminescence determined using the TD-20/20 luminometer. For both Renilla and firefly luciferase, luminescence was expressed per 1% parasitaemia.
Quantitative Realtime PCR assays
RNA was extracted from synchronized ring stage parasites 16–18 h or late trophozoites 40–42 h post-invasion. RNA extraction was performed with the TRIZOL LS Reagent (Invitrogen) as previously described. RNA to be used for cDNA synthesis was purified on PureLink column (Invitrogen) according to manufacturer's protocol. Isolated RNA was then treated with Deoxyribonuclease I (Invitrogen) to degrade contaminating gDNA. cDNA synthesis was performed with Superscript II Rnase H reverse transcriptase (Invitrogen) as described by the manufacturer. cDNA was synthesized from 800 ng total RNA in a reaction volume of 20 μl. For each cDNA synthesis reaction, a control reaction without reverse transcriptase was performed with identical amounts of template and primers. Realtime PCR was carried out as described previously. All reactions were performed at a final primer concentration of 0.5 μM using Bio-Rad ITAQ SYBR SUPERMIX® in 20 μl reactions on an ABI Prism® 7900HT real-time PCR machine.
All reactions included primers for the control genes seryl-tRNA synthetase (PF07_0073), fructose biphosphate aldolase (PF14_0425) and actin (PFL2215w), as described by Salanti et al, as well as arginyl-tRNA synthetase (PFL0900c) and glutaminyl-tRNA synthetase (PF13_0170), as described by Dzikowski et al. The ΔCT for each individual primer pair was determined by substracting the individual CT value from the CT value of the control the seryl-tRNA synthetase. ΔCTs were then converted to relative copy numbers with the formula 2ΔCt. Primers for luciferase and blasticidin were previously described. Additional gene-specific primer pairs were designed using primer 3 software: Renilla luciferase: 5'-TTCGAAAGTTTATGATCCAG-3'/5'-AACATGTCGCCATAAATAAG-3'
msp 1: 5'-TACAAGTCCATCATCTCGTT-3'/5'-TGGTTAAATCAAAGAGTTCG-3'
sbp 1: 5'-AATCCACAACTGATTTGGTA-3'/5'-GAATAGGGGACATAGATTCG-3'.
Episomal expression of luciferase and dhfr in stably transformed parasites
To determine the efficiency of transgene expression from the different constructs, the three parasite lines were synchronized and luciferase and dhfr expression were analysed at different stages of the intraerythrocytic cell cycle (Figure 1). The construct with var intron PFC0005w produced the highest level of luciferase expression, although all three transformed lines were well above background. luciferase expression of all three parasite lines was significantly higher in late stages than in ring stages (Figure 1B). For the two intron promoters this was expected and corresponds to the previously reported activity of var intron promoters and synthesis of non-coding var RNAs. The Psti/cam promoter is active in a more constitutive manner and shows a lower degree of stage specificity. Compared to var intron PFB1055c, the Psti/cam promoter becomes active earlier in the cell cycle with luciferase levels ~10 fold higher in ring stage. Its activity shows a slower increase over the course of the cell cycle to finally achieve maximum expression in schizonts with luciferase activity similar to that produced by the construct with the PFB1055c var intron.
To quantitatively analyse expression of the dhfr gene in the transfected lines, realtime RT-PCR was used to measure steady state mRNA levels. This analysis showed that dhfr and luciferase expression correlated in all constructs, consistently showing stronger expression in late stages (Figure 1C). This indicates that the promoter activities in the forward and reverse orientations are not regulated independently, but are strictly linked. This is particularly interesting for the promoter region of Psti/cam as it contains two promoters for different genes that might have been expected to be regulated separately. It has been hypothesized that the Psti upstream regulatory region does not contain a constitutive promoter, but rather might be inducible only in response to cellular stress. An induction of Psti promoter activity was not observed under temperature stress (data not shown) and it is assumed that the promoter activity measured in this assay corresponds to the "normal" promoter activity of the Psti gene. However, the possibility that the Psti promoter is inducible under different conditions and that in this assay a low "stand-by" activity was measured cannot be excluded.
Transcription levels of luciferase and dhfr were compared to two single copy P. falciparum genes, skeleton binding protein 1 (sbp1) and merozoite surface protein 1 (msp1). The sbp1 gene is expressed early in the cell cycle, therefore, sbp1 RNA levels in ring stages are much higher than for luciferase, while in late stages, sbp1 expression is low compared to luciferase. Thus the expression of luciferase and sbp1 are inversely correlated. As a consequence the expression constructs described here would not be expected to be suitable for the expression of ring-specific genes. In contrast, msp1 is expressed later in the cell cycle. Although msp1 transcription is not exclusively restricted to trophozoites, but starts already in late ring stages, msp1 expression increases over the course of the cell cycle and RNA levels peak in late trophozoites[21, 22]. Due to the late-stage specific activity of the intron promoters, the expression pattern of luciferase corresponds more closely to that of msp-1. In schizont stage the expression levels of luciferase produced by the construct with the stronger intron promoter (var PFC0005w) are very similar to those of msp1. Therefore, the pHLIDH constructs might be suitable vectors for the expression of late stage genes such as msp1.
Episomal co-expression of luciferase and blasticidin-S-deaminase in stably transformed parasites
Regulation of Renilla luciferase expression by altering blasticidin concentration
To investigate if the increase in Renilla luciferase expression resulted from an increase in promoter activity or rather reflected an increase in the copy number of the expression construct, DNA was extracted from the different parasite lines and the copy numbers of the bsd and Renilla luciferase genes were determined by quantitative PCR and compared to several single-copy genes of P. falciparum. There was a 10 to 20-fold difference in copy numbers between cultures grown in the presence of 2 μg/ml and 20 μg/ml blasticidin. In all four cultures, the copy numbers of the expression constructs displayed a linear correlation with both blasticidin concentration and Renilla luciferase activity (Figure 3B), indicating that the increase in bsd and Renilla luciferase expression was not due to changes in promoter activity but rather to a change in copy number of the expression construct. Thus the plasmid copy number can be regulated over a 10-fold range by altering the drug concentration used for selection and in this way the expression of the transgene (in this case Renilla luciferase) can be co-regulated. Episomal plasmids are usually present as concatemeres of up to 15 copies[23, 24] suggesting that changes in concatemer size are the most likely mechanism for copy number variation, however, it is also possible that an increase in copy number is caused by presence of multiple episomes per parasite.
Manipulating episome copy number to "fine-tune" transgene expression levels
A possible application of these constructs could be the expression of a gene of interest in place of Renilla luciferase to investigate its putative biological function. As the effect of over-expressing genes in Plasmodium depends on the timing and the strength of expression, the expression levels of Renilla luciferase and bsd were compared to the expression levels of several endogenous P. falciparum genes. cDNA was prepared from trophozoites and subsequently analysed by quantitative PCR. As expression from intron promoters is restricted to late stages, we compared the expression levels to that of msp1, a gene that is similarly primarily expressed in late stages. The relative amount of bsd and Renilla luciferase RNA directly correlated with blasticidin concentration, corroborating the results of the Renilla luciferase activity measurement (Figure 3C). RNA levels of Renilla luciferase were lower than msp1 for blasticidin concentrations of 2 and 5 μg/ml, however parasites growing in the presence of 10 μg/ml showed nearly equal expression levels of Renilla luciferase and msp-1 (Renilla luciferase 92% of msp1). In parasites growing in the presence of 20 μg/ml, Renilla luciferase RNA levels were ~40% higher than msp1 RNA. Other genes that are ring-stage specific (kahrp and sbp1) were expressed at lower levels in late trophozoites and served as controls. These results show that with the novel expression constructs described here, gene expression can be regulated over an approximately 10-fold range and, as was exemplified with msp1, expression levels can be achieved that correspond to endogenous transcription levels. In addition, the effect of a co-expressed gene (or a truncated version thereof) can be analysed by choosing concentrations that result in mRNA amounts above or below the "normal" expression level.
The regulatable expression system described here appears to rely on the flexibility in copy number of episomal plasmid concatamers. It, therefore, seems unlikely that this system will work with constructs that have integrated into the parasite's genome. It is probably best that experiments in which alterations in transgene expression are desired be performed on parasites shortly after stably transformed lines have been obtained in order to avoid the chromosomal integrations that are typical after long-term culture of transfected parasites. In addition, the plasmid constructs described here all utilize bidirectional promoters that are primarily active late in the cell cycle. In theory, similar plasmids could be constructed that utilize a ring stage specific promoter and thus allow regulated expression early in the cell cycle. A similar system was previously described that utilized the constitutively active bi-directional promoter of the ef-1α gene of Plasmodium berghei, which might provide expression through a broader range of the parasite cell cycle.
The blasticidin resistance gene is the ideal selectable marker for the type of manipulatable system described here. Unlike the dhfr selectable markers, which encode proteins that are resistant to the drug used for selection, bsd instead encodes a protein that inactivates blasticidin. Thus, the addition of increasing amounts of blasticidin requires corresponding increases in blasticidin-S-deaminase encoded by bsd in order to detoxify the compound and maintain parasite viability. By driving expression of the transgene of interest with the same promoter that drives bsd expression, increased bsd expression necessitates increased transgene expression, giving the regulatable expression that is desired. Removal of blasticidin from the media results in rapid loss of the transfecting plasmid (data not shown), suggesting that transgene expression levels can be lowered by reducing blasticidin selection pressure. In addition, since blasticidin is not an anti-malaria drug commonly used in the field, all parasite isolates typically used for molecular genetic studies are sensitive to this drug, and therefore the constructs described here should work in all of these laboratory lines. It is not clear if this type of system will work with rodent parasites like Plasmodium berghei. These parasites must be reared in their mammalian hosts, and the effect of blasticidin on host viability has prevented it from being developed as a selection tool for generating transgenic parasites in these systems. The development of new selectable markers for rodent parasites might negate this problem and allow a similar expression system to be developed.
Other systems have been described recently that allow the conditional activation of a transgene, however these systems are more complex and hence more difficult to establish. For instance, the Atc-regulatable system requires two different components that either need to be inserted in two different selection cycles or are provided on one very large construct. The utility of the FKBP12 system is dependent on the confirmation of the protein of interest fused to the protein destabilization domain and the efficacy of the system might vary largely between different proteins investigated. The system described here is not an inducible system and there is no possibility to switch it off completely. It rather provides the possibility to adjust the level of gene expression by selection for transgene copy number. Therefore, gene regulation is not possible within hours but, depending on the desired expression level, up to 2–3 weeks of selection are needed. The significant advantage is the simplicity and hence stability of the bidirectional constructs. Manipulation by DNA cloning is relatively easy and the initial generation of stable transformants is straightforward. During cloning of the several constructs described here not a single deletion or truncation event was observed. While the use of the same 3' UTR sequence for both transgenes could potentially lead to deletion of the intervening sequence during propagation in E. coli, such deletions were never detected in any of our small or large scale plasmid DNA preparations, suggesting that the constructs are quite stable. In addition, the identical 3'UTR sequences are oriented in opposite directions and therefore homologous recombination would be expected to produce an inversion of the entire expression cassette rather than a deletion.
The ability to genetically manipulate cultured malaria parasites has made a tremendous impact on the understanding of the molecular biology of these organisms. As knowledge of these pathogens becomes more advanced, the ability to perform more precisely regulated experiments will be needed. By using the adjustable transgene expression system described here, it should be possible to control the expression level of a gene of interest, thus allowing a researcher to determine the effect of normal expression, under-expression or over-expression on parasite growth, metabolism or viability. This type of "fine-tuning" of expression levels will be particularly important for the study of protein localization, where mis-timing or over-expression can lead to incorrect localization of a protein. Similarly, manipulating the level of transgene expression can be useful in complementation studies where the chromosomal copy of a gene has been knocked out, or in cases where expression of a dominant negative version of a protein requires particularly high expression levels to cause a phenotype. For dominant negatives, the expression level of the transgene could potentially be adjusted to a level that displays a phenotype but remains sub-lethal. The ability to control transgene expression therefore has added an additional tool to the repertoire of molecular techniques and provides a relatively simple and robust alternative for the specific analysis of gene function in Plasmodium falciparum.
This work was supported National Institutes of Health Grant AI 52390 and by a fellowship from the Deutsche Forschungsgemeinschaft (DFG) to Christian Epp. Plasmid pHH-Tati2 was kindly provided by Dr. M. Meissner, University of Heidelberg. The Department of Microbiology and Immunology at Weill Medical College of Cornell University acknowledges the support of the William Randolph Hearst Foundation. KWD is a Stavros S. Niarchos Scholar.
- Wu Y, Sifri CD, Lei HH, Su X, Wellems TE: Transfection of Plasmodium falciparum within human red blood cells. Proceedings of the National Academy of Sciences USA. 1995, 92: 973-977. 10.1073/pnas.92.4.973.View ArticleGoogle Scholar
- Wu Y, Kirkman L, Wellems TE: Transformation of Plasmodium falciparum malaria parasites by homologous integration of plasmids that confer resistance to pyrimethamine. Proc Natl Acad Sci U S A. 1996, 93 (3): 1130-1134. 10.1073/pnas.93.3.1130.PubMed CentralView ArticlePubMedGoogle Scholar
- Crabb BS, Cowman AF: Characterization of promoters and stable transfection by homologous and nonhomologous recombination in Plasmodium falciparum. Proc Natl Acad Sci U S A. 1996, 93 (14): 7289-7294. 10.1073/pnas.93.14.7289.PubMed CentralView ArticlePubMedGoogle Scholar
- Koning-Ward TF, Janse CJ, Waters AP: The development of genetic tools for dissecting the biology of malaria parasites. Annu Rev Microbiol. 2000, 54: 157-185. 10.1146/annurev.micro.54.1.157.View ArticlePubMedGoogle Scholar
- Balu B, Adams JH: Advancements in transfection technologies for Plasmodium. Int J Parasitol. 2007, 37: 1-10. 10.1016/j.ijpara.2006.10.001.View ArticlePubMedGoogle Scholar
- Aravind L, Iyer LM, Wellems TE, Miller LH: Plasmodium biology: Genomic gleanings. Cell. 2003, 115: 771-785. 10.1016/S0092-8674(03)01023-7.View ArticlePubMedGoogle Scholar
- Gardner MJ, Hall N, Fung E, White O, Berriman M, Hyman RW, Carlton JM, Pain A, Nelson KE, Bowman S, Paulsen IT, James K, Eisen JA, Rutherford K, Salzberg SL, Craig A, Kyes S, Chan MS, Nene V, Shallom SJ, Suh B, Peterson J, Angiuoli S, Pertea M, Allen J, Selengut J, Haft D, Mather MW, Vaidya AB, Martin DM, Fairlamb AH, Fraunholz MJ, Roos DS, Ralph SA, McFadden GI, Cummings LM, Subramanian GM, Mungall C, Venter JC, Carucci DJ, Hoffman SL, Newbold C, Davis RW, Fraser CM, Barrell B: Genome sequence of the human malaria parasite Plasmodium falciparum. Nature. 2002, 419: 498-511. 10.1038/nature01097.View ArticlePubMedGoogle Scholar
- Meissner M, Krejany E, Gilson PR, Koning-Ward TF, Soldati D, Crabb BS: Tetracycline analogue-regulated transgene expression in Plasmodium falciparum blood stages using Toxoplasma gondii transactivators. Proc Natl Acad Sci U S A. 2005, 102: 2980-2985. 10.1073/pnas.0500112102.PubMed CentralView ArticlePubMedGoogle Scholar
- Armstrong CM, Goldberg DE: An FKBP destabilization domain modulates protein levels in Plasmodium falciparum. Nat Methods. 2007, 4: 1007-1009. 10.1038/nmeth1132.View ArticlePubMedGoogle Scholar
- Agop-Nersesian C, Pfahler J, Lanzer M, Meissner M: Functional expression of ribozymes in Apicomplexa: Towards exogenous control of gene expression by inducible RNA-cleavage. Int J Parasitol. 2007Google Scholar
- Meissner M, Breinich MS, Gilson PR, Crabb BS: Molecular genetic tools in Toxoplasma and Plasmodium: achievements and future needs. Curr Opin Microbiol. 2007, 10: 349-356. 10.1016/j.mib.2007.07.006.View ArticlePubMedGoogle Scholar
- Deitsch KW, Driskill CL, Wellems TE: Transformation of malaria parasites by the spontaneous uptake and expression of DNA from human erythrocytes. Nucleic Acids Research. 2001, 29: 850-853. 10.1093/nar/29.3.850.PubMed CentralView ArticlePubMedGoogle Scholar
- Calderwood MS, Gannoun-Zaki L, Wellems TE, Deitsch KW: Plasmodium falciparum var genes are regulated by two regions with separate promoters, one upstream of the coding region and a second within the intron. Journal of Biological Chemistry. 2003, 278: 34125-34132. 10.1074/jbc.M213065200.View ArticlePubMedGoogle Scholar
- Dzikowski R, Frank M, Deitsch K: Mutually Exclusive Expression of Virulence Genes by Malaria Parasites Is Regulated Independently of Antigen Production. PLoS Pathog. 2006, 2: e22-10.1371/journal.ppat.0020022.PubMed CentralView ArticlePubMedGoogle Scholar
- Kyes S, Pinches R, Newbold C: A simple RNA analysis method shows var and rif multigene family expression patterns in Plasmodium falciparum. Mol Biochem Parasitol. 2000, 105: 311-315. 10.1016/S0166-6851(99)00193-0.View ArticlePubMedGoogle Scholar
- Salanti A, Staalsoe T, Lavstsen T, Jensen ATR, Sowa MPK, Arnot DE, Hviid L, Theander TG: Selective upregulation of a single distinctly structured var gene in chondroitin sulphate A-adhering Plasmodium falciparum involved in pregnancy-associated malaria. Molecular Microbiology. 2003, 49: 179-191. 10.1046/j.1365-2958.2003.03570.x.View ArticleGoogle Scholar
- Frank M, Dzikowski R, Constantini D, Amulic B, Burdougo E, Deitsch K: Strict pairing of var promoters and introns is required for var gene silencing in the malaria parasite plasmodium falciparum. J Biol Chem. 2006, 281: 9942-9952. 10.1074/jbc.M513067200.PubMed CentralView ArticlePubMedGoogle Scholar
- Rozen S, Skaletsky H: Primer3 on the WWW for general users and for biologist programmers. Methods Mol Biol. 2000, 132: 365-386.PubMedGoogle Scholar
- Polson HE, Blackman MJ: A role for poly(dA)poly(dT) tracts in directing activity of the Plasmodium falciparum calmodulin gene promoter. Mol Biochem Parasitol. 2005, 141: 179-189. 10.1016/j.molbiopara.2005.02.008.View ArticlePubMedGoogle Scholar
- Kyes SA, Christodoulou Z, Raza A, Horrocks P, Pinches R, Rowe JA, Newbold CI: A well-conserved Plasmodium falciparum var gene shows an unusual stage-specific transcript pattern. Molecular Microbiology. 2003, 48: 1339-1348. 10.1046/j.1365-2958.2003.03505.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Le Roch KG, Zhou YY, Blair PL, Grainger M, Moch JK, Haynes JD, De la Vega P, Holder AA, Batalov S, Carucci DJ, Winzeler EA: Discovery of gene function by expression profiling of the malaria parasite life cycle. Science. 2003, 301: 1503-1508. 10.1126/science.1087025.View ArticlePubMedGoogle Scholar
- Bozdech Z, Llinas M, Pulliam BL, Wong ED, Zhu JC, Derisi JL: The transcriptome of the intraerythrocytic developmental cycle of Plasmodium falciparum. Plos Biology. 2003, 1: 85-100. 10.1371/journal.pbio.0000005.View ArticleGoogle Scholar
- O'Donnell RA, Freitas LH, Preiser PR, Williamson DH, Duraisingh M, McElwain TF, Scherf A, Cowman AF, Crabb BS: A genetic screen for improved plasmid segregation reveals a role for Rep20 in the interaction of Plasmodium falciparum chromosomes. Embo Journal. 2002, 21: 1231-1239. 10.1093/emboj/21.5.1231.PubMed CentralView ArticleGoogle Scholar
- Williamson DH, Janse CJ, Moore PW, Waters AP, Preiser PR: Topology and replication of a nuclear episomal plasmid in the rodent malaria Plasmodium berghei. Nucleic Acids Research. 2002, 30: 726-731. 10.1093/nar/30.3.726.PubMed CentralView ArticlePubMedGoogle Scholar
- Kocken CH, van der Wel AM, Dubbeld MA, Narum DL, van de Rijke FM, van Gemert GJ, van L, Bannister LH, Janse C, Waters AP, Thomas AW: Precise timing of expression of a Plasmodium falciparum-derived transgene in Plasmodium berghei is a critical determinant of subsequent subcellular localization. J Biol Chem. 1998, 273: 15119-15124. 10.1074/jbc.273.24.15119.View ArticlePubMedGoogle Scholar
- Fernandez-Becerra C, de Azevedo MF, Yamamoto MM, del Portillo HA: Plasmodium falciparum: new vector with bi-directional promoter activity to stably express transgenes. Exp Parasitol. 2003, 103: 88-91. 10.1016/S0014-4894(03)00065-1.View ArticlePubMedGoogle Scholar
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