Genome-wide nucleosome mapping of Plasmodium falciparum reveals histone-rich coding and histone-poor intergenic regions and chromatin remodeling of core and subtelomeric genes
- Scott J Westenberger†1,
- Long Cui†2,
- Neekesh Dharia1,
- Elizabeth Winzeler1Email author and
- Liwang Cui2Email author
© Westenberger et al; licensee BioMed Central Ltd. 2009
Received: 31 August 2009
Accepted: 16 December 2009
Published: 16 December 2009
Epigenetic modifications of histones and regulation of chromatin structure have been implicated in regulation of virulence gene families in P. falciparum. To better understand chromatin-mediated gene regulation, we used a high-density oligonucleotide microarray to map the position and enrichment of nucleosomes across the entire genome of P. falciparum at three time points of the intra-erythrocytic developmental cycle (IDC) in vitro. We used an unmodified histone H4 antibody for chromatin immunoprecipitation of nucleosome-bound DNA.
We observed generally low nucleosomal occupancy of intergenic regions and higher occupancy of protein coding regions. In contract to the overall small fluctuation of nucleosomal occupancy in most coding regions throughout the IDC, subtelomeric genes encoding surface proteins such as var and rif, as well as some core chromosomal genes such as transcription factors, showed large changes in chromatin structure. Telomeres harbored a region with the highest nucleosomal occupancy of the genome and also exhibited large changes with higher nucleosomal occupancy at schizont stages. While many of these subtelomeric genes were previously shown to be modified by H3K9 trimethylation, we also identified some housekeeping genes in core chromosome regions that showed extensive changes in chromatin structure but do not contain this modification. tRNA and basal transcription factor genes showed low nucleosomal occupancy at all times, suggesting of an open chromatin structure that might be permissive for constitutively high levels of expression. Generally, nucleosomal occupancy was not correlated with the steady-state mRNA levels. Several var genes were exceptions: the var gene with the highest expression level showed the lowest nucleosomal occupancy, and selection of parasites for var2CSA expression resulted in lower nucleosomal occupancy at the var2CSA locus. We identified nucleosome-free regions in intergenic regions that may serve as transcription start sites or transcription factor binding sites. Using the nucleosomal occupancy data as the baseline, we further mapped the genome-wide enrichment of H3K9 acetylation and detected general enrichment of this mark in intergenic regions.
These data on nucleosome enrichment changes add to our understanding of the influence of chromatin structure on the regulation of gene expression. Histones are generally enriched in coding regions, and relatively poor in intergenic regions. Histone enrichment patterns allow for identification of new putative gene-coding regions. Most genes do not show correlation between chromatin structure and steady-state mRNA levels, indicating the dominant roles of other regulatory mechanisms. We present a genome-wide nucleosomal occupancy map, which can be used as a reference for future experiments of histone modification mapping.
In eukaryotes, packaging of DNA into chromatin has profound effects on cellular processes that utilize DNA as the template, including transcription, replication, recombination and repair. The basic structural repeat unit of chromatin is the nucleosome, which contains ~150 bp of DNA wrapped in about 1.75 superhelical turns around a central histone octamer. The chromatin structure is complex and dynamic, changing through both covalent and non-covalent mechanisms . Both histone tails and the globular domains are subject to a myriad of covalent modifications, including acetylation, methylation, phosphorylation, sumoylation, ubiquitylation, and ADP-ribosylation . These modifications may directly affect the physical properties of chromatin, and also serve as a "histone code" that is read by other effector molecules . Among non-covalent mechanisms, chromatin can be remodeled by ATP-dependent chromatin remodeling complexes and by incorporation of histone variants. The exchanges of histone variants such as H2A.Z and H3.3 with the canonical histones may influence the nucleosome stability and chromatin patterns [4, 5]. Moreover, there also exists significant crosstalk among these chromatin-mediated epigenetic mechanisms. The advances in high throughput technologies such as ChIP-chip (chromatin immunoprecipitation - DNA microarrays) and "deep sequencing" (e.g., Illumina/Solexa technology) have enabled genome-wide profiling of histone modifications and variant histones. These studies have shown that specific histone variants and modifications are found to be associated with different regions of the genome to define active euchromatin and silent heterochromatin. Insights provided by these studies have significantly advanced our understanding of how chromatin organization regulates genome function.
As demonstrated in model eukaryotes, nucleosome positioning can be a major factor in regulating gene expression. Since nucleosomes generally impede transcription and high nucleosome occupancy is considered repressive, extensive remodeling and histone eviction occur during gene activation [6, 7]. Consequently, nucleosome occupancy fluctuates during cell cycle or in response to environmental changes such as stress and activation [8, 9]. Large-scale mapping of nucleosome occupancy has been performed in Saccharomyces cerevisiae [10–13], Caenorhabditis elegans [14, 15], Drosophila melanogaster , and human . These studies have revealed that promoters are often depleted of nucleosomes, and gene expression is correlated inversely with nucleosome occupancy at the promoter. Further, functional transcription factor binding sequences are also nucleosome-free regions . Especially, nucleosome positioning around the active transcription start sites has a similar organization patterns in different eukaryotes [9, 13, 16]. These high-resolution nucleosome occupancy data also allowed the validation of computational models to predict nucleosome organization, which suggest the presence of intrinsic signals for nucleosome occupancy encoded across the genome [18, 19].
The malaria parasite Plasmodium falciparum causes over one million deaths each year. Over the last two decades, our knowledge of the malaria parasites at the molecular level has expanded substantially, particularly with the completion of the genome-sequencing project . Microarray analysis has revealed patterns of changes in mRNA levels throughout the intra-erythrocytic developmental cycle (IDC) of this parasite [21, 22]. While regulation of transcription in the malaria parasite is poorly understood, the conservation of many chromatin-modification factors in the genome underlines the significance of epigenetic mechanisms in this parasite . The malaria parasite genome encodes four canonical and four variant histones and nuclear DNA is organized in typical eukaryotic nucleosomes [24, 25]. Whereas Plasmodium chromosomes are not highly condensed during its cell cycle, indirect evidence suggests the existence of heterochromatin . A number of modifications such as acetylation and methylation have been found on the histones [25, 27] and their roles in transcription regulation appear to be evolutionarily conserved. For example, the H3K9 acetylation, conferred by the histone acetyltransferase (HAT) GCN5, is associated with active genes, whereas the heterochromatin marker H3K9 trimethylation (H3K9me3) is associated with silent genes [28–30]. Another prominent example of epigenetic regulation in Plasmodium is the regulation of the mutually exclusive expression of the ~60 var genes, which mediate antigenic switching . Silencing of the telomeric clusters of var genes requires the Sir2 histone deacetylase [31, 32]. While research on epigenetics in the malaria parasite is still in its infancy, there is a clear indication that chromatin remodeling represents an important mechanism of gene regulation and high throughput technologies such as ChIP-chip are also feasible for the extremely AT-rich genome.
Expanding on our previous success of mapping parasite histone marks using ChIP and low-density microarrays, we report here a high-density atlas of the nucleosome occupancy through the IDC of P. falciparum using a custom whole-genome tiling microarray.
Genome-wide nucleosomal occupancy in P. falciparum
We analyzed the genome-wide nucleosomal occupancy in synchronized in vitro cultures of P. falciparum for three time points from ring, trophozoite and schizont stages covering the IDC. Parasites were treated with formaldehyde to cross-link DNA-binding proteins to the genomic DNA and nucleosomal DNA was then immunoprecipitated using an antibody to histone H4. The purified DNA was hybridized to a custom whole-genome tiling array and compared with 3D7 genomic DNA hybridization data to determine relative enrichment of histones genome-wide.
Mean nucleosome enrichment values and Pearson correlation of nucleosome patterns between different stages.
Mean Log2 ratio of probes ≤10
Pearson Correlation Coefficient
Ring vs Trophozoite
Ring vs Schizont
Trophozoite vs Schizont
Internal var clusters
While most genes demonstrated nucleosome enrichment in the coding regions, some genes showed a divergence from this pattern. The first set of 1075 genes showed low nucleosomal occupancy throughout the coding regions, which includes most tRNAs, many (26 of 44) 40S and 60S ribosomal protein subunits, RNA polymerase II subunits and associated basal transcription factors such as TFIIS, as well as U6 snRNA and most LSM-domain containing small nuclear ribonucleoproteins (snRNPs) involved in ribosomal RNA maturation and mRNA splicing. The second set of 1104 genes appeared to cluster those genes with small 5' exons, visualized by the small red peak following the start of the gene. This set includes most var, rifin and stevor and some other subtelomeric variant surface antigens (VSAs), which have small 5' exons with secretory signals and generally show lower nucleosome enrichment in their coding regions than core chromosomal genes (Table 1). The third set of 918 genes had peak nucleosome enrichment upstream of the putative ATG, which includes some genes that are close to another upstream coding region and genes for which there are no probes in the upstream coding regions, resulting in log2 ratios of zero for missing data. The remaining sets four and five with 2559 genes include the vast majority of core chromosomal protein-coding genes.
Individual nucleosome position appeared to be fixed for most coding regions, since the nucleosome mapping pattern did not change for most genes throughout the IDC, showing that coding regions are tightly bound by closely spaced nucleosomes. In some coding regions, less distinct nucleosome peaks implied a delocalized nucleosome arrangement, but this pattern was similar throughout the IDC. Intergenic regions had some peaks of fixed nucleosome positions that also maintained their position specificity throughout the IDC, while overall nucleosome enrichment remained low.
To examine the hypothesis that nucleosome enrichment is determined by DNA sequence, we examined the distribution of log2 ratios for 25mer probes with different numbers of G or C nucleotides (GC bins 1-25) in various regions of the genome (Additional file 2). The average GC content of probes in various regions ranged from 5 to 7 GCs per 25mer oligonucleotide (Additional file 3). The highly AT-rich genome of P. falciparum, with higher AT content in the intergenic regions than coding regions, results in higher average probe GC content in coding than non-coding regions. There was a higher average log2 ratio of nucleosome enrichment in regions with higher GC content. This effect was more pronounced in intergenic regions, while coding regions showed a more equal log2 ratio distribution across GC bins. However, even GC-rich non-coding regions showed lower log2 ratios of nucleosome enrichment than highly AT-rich coding regions. Therefore, while the highly AT-rich intergenic regions may be predisposed to lower nucleosomal occupancy, DNA sequence does not appear to be the primary determinant of chromatin nucleosome enrichment, which may be specifically coordinated with the delineation of coding versus non-coding regions.
Telomeric changes in chromatin structure
Different patterns of nucleosomal occupancy dynamics
Core chromosome genes with H3K9me3 modification. H4 change is the Δlog2 ratio (H4 ChIP/gDNA) over three time points.
Conserved Plasmodium protein, unknown function
high mobility group protein
Erythrocyte membrane protein, putative
RNA binding protein, putative
Surface-associated Interspersed gene SURFIN 4.1
conserved Plasmodium protein, unknown function
conserved Plasmodium protein, unknown function
CPW-WPC family protein
Ser/Arg-rich splicing factor, putative
transcription factor with AP2 domain(s)
glycophorin-binding protein 130 precursor
Cytoadherence linked asexual protein 3.1
serine/threonine protein kinase, putative
Cytoadherence linked asexual protein, 3.2
conserved Plasmodium protein, unknown function
liver stage antigen-1
conserved Plasmodium protein, unknown function
conserved Plasmodium protein, unknown function
Transcription and chromatin-related genes with extreme changes in nucleosome enrichment, highest in trophozoites.
high mobility group protein
pre-mRNA splicing factor, putative
Transcription factor IIA, alpha/beta subunit
small nuclear ribonucleoprotein D1, putative
DNA/RNA-binding protein Alba, putative
Nifu-like protein, putative
small nuclear ribonucleoprotein, putative
arginine n-methyltransferase, putative
HORMA domain protein, putative
EF-hand domain hypothetical protein, conserved
RNA and export factor binding protein, putative
tudor domain conserved Plasmodium protein
transcription elongation factor s-ii, putative
high mobility group protein
chromosome associated protein, putative
transcription factor with AP2 domain(s)
RNA binding protein, putative
Chromodomain-helicase-DNA-binding protein 1
Histone acetyltransferase, putative
RNA-binding protein, putative
zinc finger protein, putative
transcription factor with AP2 domain(s)
RNA binding protein, putative
RNA binding protein, conserved
RNA binding protein, putative
transcription factor with AP2 domain(s)
Depending on the dynamics of nucleosome enrichment in different developmental stages, genes can be organized into distinct categories. Some genes involved in basal transcription machinery, ribosomal RNA maturation and mRNA splicing were always nucleosome-free (Additional file 6). Genes for U6 snRNA LSM protein (PF13_0142) and RNA polymerase II (PF13_0023) were confirmed to have low nucleosomal occupancy less than or similar to intergenic regions, and much lower than adjacent genes (Figure 5C and 5D). The maintenance of an open chromatin conformation may allow for high levels of constitutive expression of these genes. Numerous hypothetical genes with similarly low nucleosome enrichment may also play a role in these processes. In addition to the genes found in TARE 5 telomeric regions described above, we found several genes that displayed nucleosomal occupancy changes similar to those seen for telomeres. These genes encode the Pf11-1 protein PF10_0374, S-antigen, Liver Stage Antigen 1, interspersed repeat antigen, Maurer's cleft two transmembrane protein 1.1, Plasmodium MYXSPDY repeat protein, two glycophorin binding protein homologous proteins, a highly variable hypothetical protein PF10_0351, and several conserved hypothetical proteins (Additional file 7). All these genes displayed a very large increase in nucleosome enrichment (> 0.7 log2 ratio) from trophozoite to schizont stages and intermediate levels in rings, placing them in the top 20% of all genes ranked by nucleosomal occupancy change throughout the IDC. These genes contain highly repetitive regions, and may be regulated by the same chromatin remodeling machinery that is targeted to the highly repetitive telomere sequences. It is interesting to note that many of these genes encode highly variable surface proteins, and five of them are found in close proximity on chromosome 10. Another small group of genes including an amino transferase, leucine-rich repeat protein 2 and a PPPDE peptidase showed yet a different pattern with highest nucleosome enrichment in rings, lowest in trophozoites, and a slight increase in schizonts (Additional file 8).
Interestingly, the non-coding RNA types showed different patterns of nucleosome enrichment. tRNA genes have the lowest nucleosomal occupancy of any set of genes, lower than the average for intergenic regions, indicating that their chromatin structure is different from those of protein-coding RNAs. This nucleosome-free status of tRNAs may be due to their essential role in translation and high abundance in the cell, or may be a specific feature of RNA polymerase III (Pol III) transcribed regions. Another Pol III transcript, 5S rRNAs, had much lower nucleosome enrichment than other rRNAs throughout the IDC and showed a different pattern of enrichment changes. 5.8S rRNAs showed higher nucleosome enrichment in rings relative to 18S and 28S rRNAs, with little change in trophozoites and a large decrease in schizonts. The 18S and 28S rRNA loci showed a large increase from rings to trophozoites and decrease again in rings. This 18S and 28S rRNA pattern is similar to many subtelomeric genes. While the loci on chromosomes 1 and 5 are subtelomeric and thus might be expected to behave similarly to other subtelomeric genes, the chromosome 7 locus is not subtelomeric, and therefore this pattern may be specific to rRNA loci and not a byproduct of their subtelomeric localization.
Comparison of cDNA start sites and nucleosome free-regions
To test the hypothesis that nucleosome-free regions may exist at transcription start sites (TSS) as has been shown in other organisms, we examined the nucleosome enrichment at over 2600 putative transcription start sites annotated by the Malaria Full-Length cDNA database http://fullmal.hgc.jp/index_ajax.html . We found a large distribution of nucleosome enrichment values at these sites (Additional file 1). The median value for these regions was between -0.5 and -0.7 for the various stages (Additional file 1), which was higher than the mean for core chromosomal non-coding regions (Table 1). However, some of these TSS are predicted inside coding regions, which had median log2 ratios of around 0.2. We also predicted absolute minima of a 150 bp window running mean of the log2 ratio of nucleosome occupancy in the upstream intergenic regions of all genes (Additional file 1). Multiple, additional local minima - nucleosome-free regions were also observed in many intergenic regions. While some cDNA sequences did appear to begin at intergenic local minima of nucleosome enrichment (Additional file 1), consistent with the hypothesis, many others were found at intergenic local peaks of nucleosome enrichment. Therefore, our dataset is not completely consistent with the hypothesis that TSSs correlate with nucleosome-free intergenic regions for all genes. The caveat is that given low probe coverage for intergenic regions, their chromatin structure may not be accurately represented in our data. Besides, the cDNA sequence dataset is also incomplete, providing TSS predictions for about half of the genes and further cDNA sequencing may show better correspondence with our nucleosomal occupancy data. Furthermore, many P. falciparum genes have been shown to use multiple TSSs, which may obscure the minima of nucleosomal occupancy within the intergenic regions. Additionally, nucleosomal occupancy may differ at other points of the life cycle not represented in our dataset, during which some genes are most highly expressed. Taken together, transcription of some genes may be initiated at these nucleosome-free regions (NFRs) (Additional file 1), while others may have alternative requirements for chromatin structure at the TSS.
Correlation of nucleosome enrichment with gene expression
Overall, changes in nucleosome enrichment were not correlated with gene expression for the majority of genes in the genome. We calculated the Pearson correlation coefficients between the log2 ratios of nucleosome enrichment and gene expression values from sorbitol-synchronized in vitro P. falciparum culture analyzed previously . There was no genome-wide pattern of correlation or anti-correlation with expression throughout the IDC. This implies that for most genes, their expression is not regulated by, nor does it result in changes in the nucleosome enrichment of the gene coding regions. However, particular subsets of genes did show interesting patterns and correlations between expression and nucleosome enrichment.
We identified 851 genes with high expression (>500 units)  at some time point of the IDC, and showed minimal changes in nucleosomal occupancy (Δlog2 ratio < 0.5). The nucleosomal occupancy of these genes ranged from nucleosome-free (log2 ratio < -1.5) to highly occupied (log2 ratio >0.7). This group includes genes upregulated in merozoite and early ring stages such as merozoite-associated tryptophan-rich antigen, PTRAMP, RESA, PHISTs, and other genes involved in host cell remodeling. It also includes genes upregulated in late schizont stage involved in gliding motility and invasion of red blood cells such as RAP1, RAP3, RBP2a, RBP2b, RBP3, apical sushi protein (ASP), MSP3, MSP9, EBA-140, CLAG3.2, AMA1, and SPATR. This indicates that these genes involved in merozoite development and invasion are not regulated at the level of nucleosomal occupancy, and their high expression is not associated with large changes in nucleosomal occupancy.
In comparison, 315 genes showed large changes in nucleosomal occupancy (Δlog2 ratio >0.7, 2-fold), but are not highly expressed (<200 units) at any time point in the IDC . These include numerous subtelomeric members of multigene families of antigenic surface protein genes, such as pfemp1, surfins, rifins and stevors, of which some members are highly expressed and subject to the general nucleosomal occupancy changes regulating all subtelomeric regions. These genes showed low nucleosome enrichment in ring stages when expression of these genes is highest, and were nucleosome-enriched in trophozoites and schizonts. In contrast, most low-expressing genes in core chromosome regions (76 of 128) with large changes in nucleosomal occupancy showed the opposite pattern of high nucleosomal occupancy in rings and low in trophozoites and schizonts (Additional file 8). This set of 120 genes also includes cysteine repeat modular protein 2, transcription elongation factor S-II, leucine-rich repeat proteins LRR2 and LRR10, and UbiE-like methyltransferase. These patterns suggest the possible existence of two kinds of chromatin remodeling machinery acting with opposing results targeted to different chromosomal regions. However, chromatin remodeling at these genes did not appear to affect their mRNA levels during the IDC.
Nucleosome occupancy changes of the var genes
This pattern of nucleosome enrichment changes at var genes was also found among other VSA genes. For the 129 rifin genes, they were histone-poor in ring stages (log2 ratio = -0.64) but more histone-rich in trophozoites and schizonts (log2 ratio = 0.30 and 0.14). The nucleosome enrichment pattern for var genes was slightly different from that of rifins with average nucleosomal occupancy in rings (log2 ratio = -0.22) and much higher than average nucleosomal occupancy in trophozoites and schizonts (log2 ratio = 0.8 and 0.72). To identify genes with similar chromatin remodeling patterns, we used var and rifin genes as seeds to search for genes with highly correlated changes (>0.95 Pearson coefficient) in nucleosomal enrichment throughout the IDC. This identified a set of 226 genes with large changes in nucleosome enrichment (Δlog2 ratio > 0.6). These genes are found exclusively in subtelomeric regions or internal var gene clusters (Figure 4). Most of these genes were also previously described as enriched in the histone H3K9me3 modification, a marker of heterochromatin .
H3K9 acetylation modification pattern
The variation in nucleosomal occupancy observed using the unmodified histone H4 antibodies was also visible using histone H3K9 acetylation (H3K9ac) antibodies. Therefore, to properly determine regions enriched for H3K9 acetylation, it is necessary to normalize the data relative to the unmodified histone H4 hybridization pattern, rather than to genomic DNA. When histone H3K9ac ChIP DNA was normalized relative to genomic DNA, the pattern followed the H4 pattern of nucleosomal occupancy with slightly higher peaks (data not shown). Therefore, the distribution of H3K9ac generally followed the background distribution of nucleosomes. Normalization to the H4 ChIP pattern resulted in higher signals in the intergenic regions, perhaps due to lower, local nucleosomal occupancy. Very distinct spikes were observed in regions of the highest nucleosomal occupancy. This indicates that while the nucleosomal occupancy was generally lower in intergenic regions, the majority of the histones in the intergenic regions contained the H3K9ac modification. The H3K9ac enrichment appeared in all intergenic regions and did not appear to be correlated with changes in mRNA levels. These data confirmed the findings of Salcedo-Amaya et al. who also found that H3K9ac was enriched in all intergenic regions, and only appeared higher for very highly expressed genes in schizont stages .
The association of nucleosomes with coding regions and their relative absence from intergenic regions is distinctly different from the findings in model eukaryotes, where nucleosomes are usually absent only at promoters and intergenic regions are condensed. In P. falciparum genome, this may be the result of the extreme AT-richness in the intergenic regions. Since poly-A tracts induce bending of the DNA helix  and this bending tends to exclude nucleosomes from these regions , the high AT content (95%) of intergenic regions of P. falciparum may selectively exclude histones from these regions. While model organisms generally have small nucleosome-free regions observed at TSSs [11, 41], our analysis using the P. falciparum full-length cDNA data was inconclusive. Instead, a more extensively nucleosome-free region may be present in the intergenic regions of the parasite genome allowing easy access to RNA polymerase machinery and transcription factors. This may be partially related to the diverse transcription initiation sites found in many P. falciparum genes . Yet, in spite of the lower nucleosomal occupancy at the intergenic regions, there were spikes of modified histones in the intergenic regions, which may play additional roles in gene expression regulation. The higher nucleosomal occupancy in coding regions of most genes may provide a means to safeguard against spurious transcription initiation in the coding region of the gene.
In model eukaryotes, gene expression is positively correlated with the nucleosome occupancy at the promoter regions. In contrast, the intergenic putative promoter regions of P. falciparum showed little or no change in nucleosomal occupancy, and generally remained nucleosome-free, compared to the large changes observed in coding regions. Comparing the nucleosomal occupancy of the coding regions, we found no general correlation with steady-state mRNA levels determined by microarrays. This is not surprising, since chromatin structure only represents one mechanism of transcription regulation. In addition, transcription initiation is regulated by sequence-specific transcriptional activators and repressors. Steady-state mRNA levels are determined by the level of transcription, and post-transcriptional regulation of mRNA stability and degradation. Therefore, we would not expect chromatin structure to be the dominant determinant of steady-state mRNA levels.
The highly condensed heterochromatin that comprises most non-coding regions of higher eukaryotes represses transcription in those regions. However, in P. falciparum, a recent study found the repressive histone modification of H3K9me3 only at subtelomeric loci and not in other intergenic regions . It may be that the generally relaxed, non-condensed structure of P. falciparum intergenic chromatin in core chromosomal regions is sufficiently permissive of transcription such that further relaxation is not required to recruit transcription factors and initiate high levels of transcription. Our Q-PCR validation at promoters of selected individual genes supported such a generalization (e.g., var genes, msp2). Another study found that the transcription pre-initiation complex was pre-assembled on promoters of all erythrocytic-expressed genes, independent of any histone acetylation , supporting this hypothesis, and challenging the model that chromatin acetylation precedes transcription initiation in Plasmodium.
In human cells, regulation of transcription by RNA Pol III requires histone acetylation and changes in chromatin condensation [45, 46]. However, the consistently low nucleosomal occupancy of tRNA and 5S rRNA genes in P. falciparum may indicate a different mechanism for regulating Pol III-derived transcripts that may not involve interaction with modified histones but may instead depend on other Pol III associated transcription factors. Therefore, it may be advantageous to keep these genes in a perpetually permissive state to allow for rapid transcription of tRNAs when protein synthesis is rapidly accelerated in growing trophozoites. This same situation may apply to the RNA polymerase II transcribed genes that constitute the basal transcription machinery, which may need to be rapidly and highly expressed to initiate a general transcriptional increase in ring stage.
The expression of var genes is inversely correlated with nucleosomal occupancy. This has been confirmed from the dramatic changes in nucleosomal occupancy between active and silent var2CSA gene. The changes in nucleosomal occupancy observed at the intron of var genes supports the hypothesis that var gene regulation is based on cooperative interactions between the two promoters of each var gene . The higher nucleosome occupancy in exon 2 of most var genes may inhibit full-length gene transcription compared with the lower nucleosomal occupancy in exon 1. This may provide an explanation for the low-level production of many var transcripts that are detectable by RT-PCR, but not detectable by Northern blots. The generally permissive chromatin structure of all var genes exon 1 may allow for abortive transcripts to be formed and rapidly degraded and for the generation of antisense transcript directed by the var intron. Transcription factor genes with patterns of nucleosome enrichment similar to VSAs may be involved in regulating the expression of these genes. The subnuclear localization of the singly expressed var gene may be shared with some of these similarly regulated core chromosomal genes.
The lack of histones in intergenic regions may prevent the condensation of chromosomes during late stages of mitotic replication, which does not occur in Plasmodium parasites as it does in other eukaryotic organisms. The telomeric regions display the highest chromatin condensation of any region of the genome. In other eukaryotes where chromosomes condense upon mitotic cell division, the centromere region is responsible for binding to the kinetochore and microtubules for chromosomal segregation in daughter cells. In Plasmodium, not all chromosomes have annotated centromeres, and the chromosomes do not condense at schizogony. The telomeric regions with TAREs and Rep20 that have higher nucleosomal enrichment may play a role in chromosome segregation into daughter cells . This may also be an adaptation to the schizogony process where multiple rounds of nuclear replication precede cytokinesis in the development of merozoites. The highly repetitive genes that show telomere-like chromatin changes may be targeted by chromatin remodeling machinery that recognizes repetitive regions throughout the genome.
P. falciparum exhibits unique chromatin structure due to its highly AT-rich genome, with histone-rich coding regions and relatively histone-free intergenic regions. Chromatin dynamics differ for coding, non-coding, subtelomeric and telomeric regions of the genome. Histone enrichment patterns allow for identification of new putative gene-coding regions. Numerous genes display dynamic changes in nucleosomal occupancy, but these changes do not correlate with mRNA levels for most genes. However, nucleosome enrichment at var genes is negatively correlated with expression. Our genome-wide nucleosome occupancy data provides a framework to build our understanding of the mechanisms of chromatin-mediated regulation of RNA expression and DNA replication throughout the cell cycle. Future studies will elaborate upon the role of specific histone modifications, and the interactions of nucleosomes with DNA binding proteins and transcription machinery to produce the highly regulated cycle of gene expression in this dangerous parasite.
The P. falciparum 3D7 clone was cultured at 5% hematocrit in type O+ human red blood cells as previously described . The parasites were synchronized twice by 5% sorbitol treatments at the ring stage . To obtain parasite materials, infected erythrocytes were lysed by 0.1% saponin treatment, and parasite pellets were collected by centrifugation and washed twice with cold phosphate-buffered saline (PBS). Synchronized parasites were harvested at 12, 30 and 42 h to represent ring, trophozoite, and schizont stages, respectively.
For ChIP, 3 × 109 trophozoite and schizont stage or 9 × 109 ring stage parasites were collected. First, the parasites were treated with 2 ml of permeabilization buffer (150 mM sucrose, 15 mM Tris-HCl, pH 7.5, 15 mM NaCl, 60 mM KCl, 2 mM CaCl2, 0.15 mM spermin, and 0.5 mM spermidine) for 5 min at room temperature. Micrococcal nuclease (MNase) digestion was performed at 37°C for 10 min using 10 units of the enzyme, which were titrated to digest most chromatin into mononucleosomes. The MNase digestion was stopped by 2 ml of stop solution (40 mM Tris-HCl, pH 8.0, 40 mM EDTA, 150 mM NaCl, 2% SDS, 1.2 mg/ml proteinase K) and incubating at 50°C for 15 min. After washing the parasites twice with cold PBS, the samples were crosslinked with 1% formaldehyde at room temperature for 30 min. After quenching the crosslinker with glycine, parasites were washed twice with cold PBS and resuspended in 1.5 ml of immunoprecipitation (IP) buffer (50 mM Hepes, pH 7.5, 140 mM NaCl, 1 mM EDTA, 1% Triton X-100, 0.1% sodium deoxycholate) with a protease inhibitor cocktail (Roche). A brief sonication was performed on ice for 20 s to break the cell membranes. After removing cell debris by centrifugation, the digested chromatin was used for IP with the anti-H4 antibodies (Millipore) as previously described . Amplification of immunoprecipitated DNA was performed using a randomly primed PCR amplification method [50, 51]. Fifty micrograms of amplified DNA were digested into 50 bp fragments in a 50 ml reaction with 2 units of DNase I (Promega) at 37°C for 1 min. After inactivating the enzyme at 95°C for 10 min, the digested DNA fragments were labeled with 1 mM Bio-N6-ddATP (Enzo) using 400 U terminal deoxynucleotidyl transferase (Roche) incubated for 1 hr at 37°C, then at 70°C for 10 minutes. ChIP with the anti-H3K9ac antibodies was performed similarly as with the anti-H4 antibodies.
Hybridization and data analysis
End-labeled DNA was hybridized to the Affymetrix microarray in a hybridization mix prepared using the Affymetrix hybridization, Wash and Stain kit, following the manufacturer's instructions. Chips were washed on the Affymetrix Wash Station using a modified protocol Flex FS450_0001 with all temperatures set to 23°C. Chips were scanned on the Affymetrix scanner and data was analyzed and visualized using custom Matlab scripts available upon request. The array contains over 6.5 million probes total. 4,219,964 probes are uniquely mapped to a single location, and 4,642,958 probes mapped to 10 or fewer locations in the genome, with 91% of those uniquely mapped to a single location. Samples were normalized using median line normalization for invariant probes relative to two hybridizations of 3D7 genomic DNA (3D7-1, 3D7-2) described previously . We calculated the log2 of the ratio of hybridization intensity of the test sample divided by the 3D7 reference for each probe. Then we calculated the running mean log2 ratio for windows of 150 bp for regions that contain at least 3 probes. For highly repetitive intergenic regions with no probe coverage, we connect the running mean line between the nearest two points with average log2 ratios. We compared the hybridization intensity of the ChIP-chip data with 3D7 genomic DNA data to determine genome-wide relative enrichment of nucleosomes. We compared the results of analyses using probes that uniquely mapped to a single location versus all probes that mapped to 10 or fewer locations in the genome. We found that inclusion of the probes mapped to 10 or fewer locations did not change the average nucleosome enrichment patterns for coding regions with good unique probe coverage (Table 1). This provided informative data for many subtelomeric multigene families with similar sequences. Therefore, we used this probe-mapping cutoff for all analyses. Our results demonstrated similar patterns of nucleosome enrichment for these multigene families, implying that the average signal distribution across the multiple locations is an accurate representation of the chromatin structure for these repetitive regions. The interpretation of an average log2 ratio over 150 bp also served to diminish the contribution of signal from outlier probes. Since chromatin structure is also influenced by DNA sequence, we expect similar nucleosomal occupancy signal from genes with similar sequences, and thus the probe signal will be similar at all locations. However, these results in identical repetitive telomeric and subtelomeric regions should be considered representative of the average nucleosomal occupancy of these sequences, and not precisely representing one particular region. Gene annotation information was taken from PlasmoDB version 5.5. Microarray data were submitted NCBI Gene Expression Omnibus (GEO) website with a provisional accession number GSE18968. Nucleosomal occupancy and the H3K9ac maps for P. falciparum chromosomes have also been submitted to PlasmoDB. Running median lines of log2 ratio for ring, trophozoite, and schizont are visible as Genome Browser tracks.
Validation of the microarray data
To validate the microarray results, ChIP with anti-H4 antibodies followed by real-time PCR analysis for selected genes was performed using aliquots of the same parasite populations . The relative nucleosome enrichment level of selected genes versus input DNA was calculated using 2-ΔΔCt method with MAL8P1.36 as a reference gene which had stable nucleosome occupancy throughout IDC . To determine whether the level of nucleosome occupancy is correlated with the expression levels of var genes, RNA was extracted from aliquots of the same parasite populations. Real-time RT-PCR was used to quantify the relative expression level of var genes using a set of primers to specifically amplify individual var genes with seryl-tRNA synthetase as a reference gene . ChIP with anti-H4 antibodies followed by real-time PCR analysis was used to quantify the relative nucleosomal enrichment at var genes using the same set of primers with MAL8P1.36 as a reference. To further demonstrate that nucleosome occupancy is correlated with var gene expression, we panned the parasites with CSA to select parasites with var2CSA (PFL0030c) expression . After three rounds of CSA selection, the expression level of each var gene was determined by real time RT-PCR to confirm that var2CSA was active. To compare the nucleosome occupancy of CSA-selected versus unselected parasites, ChIP and real-time PCR were performed using previously-described primers for different regions of var2CSA .
List of Abbreviations
quantitative polymerase chain reaction
reverse-transcriptase polymerase chain reaction.
We would like to thank the staff of PlasmoDB for their help and support for genomic analysis of Plasmodium species and rapid dissemination of our results to the malaria research community. We would like to thank Rahil Sethi for preliminary analysis of histone occupancy data. We would also like to thank Selina Bopp, Stephan Meister and Taylor Bright for their reading of and helpful comments on the manuscript. SJW was supported by NIH grant 1F32AI074242-01A1. Long Cui and Liwang Cui were supported by NIH grant AI064553. EAW was supported by the Keck Foundation and NIH grant R01AI059472.
- Goldberg AD, Allis CD, Bernstein E: Epigenetics: A landscape takes shape. Cell cycle. 2007, 128: 635-638.Google Scholar
- Kouzarides T: Chromatin modifications and their function. Cell. 2007, 128 (4): 693-705. 10.1016/j.cell.2007.02.005.View ArticlePubMedGoogle Scholar
- Jenuwein T, Allis CD: Translating the histone code. Science. 293 (5532): 1074-1080. 10.1126/science.1063127.
- Raisner RM, Mahdhani HD: Patterning chromatin: form and function for H2A.Z variant nucleosomes. Cur Opin Gen Dev. 2006, 16: 119-124. 10.1016/j.gde.2006.02.005.View ArticleGoogle Scholar
- Lieb JD, Clarke ND: Control of transcription through intragenic patterns of nucleosome composition. Cell. 2005, 123 (7): 1187-1190. 10.1016/j.cell.2005.12.010.View ArticlePubMedGoogle Scholar
- Boeger H, Griesenbeck J, Strattan JS, Kornberg RD: Nucleosomes unfold completely at a transcriptionally active promoter. Mol Cell. 2003, 11 (6): 1587-1598. 10.1016/S1097-2765(03)00231-4.View ArticlePubMedGoogle Scholar
- Henikoff S: Nucleosomes at active promoters: unforgettable loss. Cancer Cell. 2007, 12: 407-409. 10.1016/j.ccr.2007.10.024.View ArticlePubMedGoogle Scholar
- Hogan GJ, Lee CK, Lieb JD: Cell cycle-specified fluctuation of nucleosome occupancy at gene promoters. PLoS Genet. 2006, 2 (9): e158-10.1371/journal.pgen.0020158.PubMed CentralView ArticlePubMedGoogle Scholar
- Schones DE, Cui K, Cuddapah S, Roh TY, Barski A, Wang Z, Wei G, Zhao K: Dynamic regulation of nucleosome positioning in the human genome. Cell. 2008, 132 (5): 887-898. 10.1016/j.cell.2008.02.022.View ArticlePubMedGoogle Scholar
- Bernstein BE, Liu CL, Humphrey EL, Perlstein EO, Schreiber SL: Global nucleosome occupancy in yeast. Genome Biol. 2004, 5 (9): R62-10.1186/gb-2004-5-9-r62.PubMed CentralView ArticlePubMedGoogle Scholar
- Lee CK, Shibata Y, Rao B, Strahl BD, Lieb JD: Evidence for nucleosome depletion at active regulatory regions genome-wide. Nature Genet. 2004, 36 (8): 900-905. 10.1038/ng1400.View ArticlePubMedGoogle Scholar
- Yuan GC, Liu YJ, Dion MF, Slack MD, Wu LF, Altschuler SJ, Rando OJ: Genome-scale identification of nucleosome positions in S. cerevisiae. Science. 2005, 309 (5734): 626-630. 10.1126/science.1112178.View ArticlePubMedGoogle Scholar
- Lee W, Tillo D, Bray N, Morse RH, Davis RW, Hughes TR, Nislow C: A high-resolution atlas of nucleosome occupancy in yeast. Nature Genet. 2007, 39 (10): 1235-1244. 10.1038/ng2117.View ArticlePubMedGoogle Scholar
- Johnson SM, Tan FJ, McCullough HL, Riordan DP, Fire AZ: Flexibility and constraint in the nucleosome core landscape of Caenorhabditis elegans chromatin. Genome research. 2006, 16 (12): 1505-1516. 10.1101/gr.5560806.PubMed CentralView ArticlePubMedGoogle Scholar
- Valouev A, Ichikawa J, Tonthat T, Stuart J, Ranade S, Peckham H, Zeng K, Malek JA, Costa G, McKernan K, et al: A high-resolution, nucleosome position map of C. elegans reveals a lack of universal sequence-dictated positioning. Genome Res. 2008, 18 (7): 1051-1063. 10.1101/gr.076463.108.PubMed CentralView ArticlePubMedGoogle Scholar
- Mavrich TN, Jiang C, Ioshikhes IP, Li X, Venters BJ, Zanton SJ, Tomsho LP, Qi J, Glaser RL, Schuster SC, et al: Nucleosome organization in the Drosophila genome. Nature. 2008, 453 (7193): 358-362. 10.1038/nature06929.PubMed CentralView ArticlePubMedGoogle Scholar
- Liu X, Lee CK, Granek JA, Clarke ND, Lieb JD: Whole-genome comparison of Leu3 binding in vitro and in vivo reveals the importance of nucleosome occupancy in target site selection. Genome Res. 2006, 16 (12): 1517-1528. 10.1101/gr.5655606.PubMed CentralView ArticlePubMedGoogle Scholar
- Segal E, Fondufe-Mittendorf Y, Chen L, Thastrom A, Field Y, Moore IK, Wang JP, Widom J: A genomic code for nucleosome positioning. Nature. 2006, 442 (7104): 772-778. 10.1038/nature04979.PubMed CentralView ArticlePubMedGoogle Scholar
- Ioshikhes IP, Albert I, Zanton SJ, Pugh BF: Nucleosome positions predicted through comparative genomics. Nature Genet. 2006, 38 (10): 1210-1215. 10.1038/ng1878.View ArticlePubMedGoogle Scholar
- Gardner MJ, Shallom SJ, Carlton JM, Salzberg SL, Nene V, Shoaibi A, Ciecko A, Lynn J, Rizzo M, Weaver B, et al: Sequence of Plasmodium falciparum chromosomes 2, 10, 11 and 14. Nature. 2002, 419 (6906): 531-534. 10.1038/nature01094.View ArticlePubMedGoogle Scholar
- Bozdech Z, Llinas M, Pulliam BL, Wong ED, Zhu J, DeRisi JL: The transcriptome of the intraerythrocytic developmental cycle of Plasmodium falciparum . PLoS Biol. 2003, 1 (1): E5-10.1371/journal.pbio.0000005.PubMed CentralView ArticlePubMedGoogle Scholar
- Le Roch KG, Zhou Y, Blair PL, Grainger M, Moch JK, Haynes JD, De La Vega P, Holder AA, Batalov S, Carucci DJ: Discovery of gene function by expression profiling of the malaria parasite life cycle. Science. 301 (5639): 1503-1508. 10.1126/science.1087025.
- Aravind L, Iyer LM, Wellems TE, Miller LH: Plasmodium biology: genomic gleanings. Cell. 2003, 115 (7): 771-785. 10.1016/S0092-8674(03)01023-7.View ArticlePubMedGoogle Scholar
- Cary C, Lamont D, Dalton JP, Doerig C: Plasmodium falciparum chromatin: nucleosomal organisation and histone-like proteins. Parasitol Res. 1994, 80 (3): 255-258. 10.1007/BF00932684.View ArticlePubMedGoogle Scholar
- Miao J, Fan Q, Cui L, Li J, Li J, Cui L: The malaria parasite Plasmodium falciparum histones: organization, expression, and acetylation. Gene. 2006, 369: 53-65. 10.1016/j.gene.2005.10.022.View ArticlePubMedGoogle Scholar
- Chookajorn T, Ponsuwanna P, Cui L: Mutually exclusive var gene expression in the malaria parasite: multiple layers of regulation. Trends Parasitol. 2008, 24 (10): 455-461. 10.1016/j.pt.2008.07.005.View ArticlePubMedGoogle Scholar
- Cui L, Fan Q, Cui L, Miao J: Histone lysine methyltransferases and demethylases in Plasmodium falciparum. Int J Parasitol. 2008, 38 (10): 1083-1097. 10.1016/j.ijpara.2008.01.002.PubMed CentralView ArticlePubMedGoogle Scholar
- Cui L, Miao J, Furuya T, Li X, Su XZ, Cui L: PfGCN5-mediated histone H3 acetylation plays a key role in gene expression in Plasmodium falciparum. Eukaryot Cell. 2007, 6 (7): 1219-1227. 10.1128/EC.00062-07.PubMed CentralView ArticlePubMedGoogle Scholar
- Chookajorn T, Dzikowski R, Frank M, Li F, Jiwani AZ, Hartl DL, Deitsch KW: Epigenetic memory at malaria virulence genes. Proc Natl Acad Scie USA. 2007, 104 (3): 899-902. 10.1073/pnas.0609084103.View ArticleGoogle Scholar
- Fan Q, An L, Cui L: Plasmodium falciparum histone acetyltransferase, a yeast GCN5 homologue involved in chromatin remodeling. Eukaryot Cell. 2004, 3 (2): 264-276. 10.1128/EC.3.2.264-276.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Duraisingh MT, Voss TS, Marty AJ, Duffy MF, Good RT, Thompson JK, Freitas-Junior LH, Scherf A, Crabb BS, Cowman AF: Heterochromatin silencing and locus repositioning linked to regulation of virulence genes in Plasmodium falciparum. Cell. 2005, 121 (1): 13-24. 10.1016/j.cell.2005.01.036.View ArticlePubMedGoogle Scholar
- Freitas-Junior LH, Hernandez-Rivas R, Ralph SA, Montiel-Condado D, Ruvalcaba-Salazar OK, Rojas-Meza AP, Mancio-Silva L, Leal-Silvestre RJ, Gontijo AM, Shorte S, et al: Telomeric heterochromatin propagation and histone acetylation control mutually exclusive expression of antigenic variation genes in malaria parasites. Cell. 2005, 121 (1): 25-36. 10.1016/j.cell.2005.01.037.View ArticlePubMedGoogle Scholar
- Corcoran LM, Thompson JK, Walliker D, Kemp DJ: Homologous recombination within subtelomeric repeat sequences generates chromosome size polymorphisms in P. falciparum. Cell. 1988, 53 (5): 807-813. 10.1016/0092-8674(88)90097-9.View ArticlePubMedGoogle Scholar
- Figueiredo LM, Pirrit LA, Scherf A: Genomic organisation and chromatin structure of Plasmodium falciparum chromosome ends. Mol Biochem Parasitol. 2000, 106 (1): 169-174. 10.1016/S0166-6851(99)00199-1.View ArticlePubMedGoogle Scholar
- O'Donnell RA, Freitas-Junior 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 J. 2002, 21 (5): 1231-1239. 10.1093/emboj/21.5.1231.PubMed CentralView ArticlePubMedGoogle Scholar
- Watanabe J, Wakaguri H, Sasaki M, Suzuki Y, Sugano S: Comparasite: a database for comparative study of transcriptomes of parasites defined by full-length cDNAs. Nucleic Acids Res. 2007, 35: D431-438. 10.1093/nar/gkl1039.PubMed CentralView ArticlePubMedGoogle Scholar
- Zhou Y, Ramachandran V, Kumar KA, Westenberger S, Refour P, Zhou B, Li F, Young JA, Chen K, Plouffe D, et al: Evidence-Based Annotation of the Malaria Parasite's Genome Using Comparative Expression Profiling. PLoS ONE. 2008, 3 (2): e1570-10.1371/journal.pone.0001570.PubMed CentralView ArticlePubMedGoogle Scholar
- Salcedo-Amaya AM, van Driel MA, Alako BT, Trelle MB, Elzen van den AM, Cohen AM, Janssen-Megens EM, Vegte-Bolmer van de M, Selzer RR, Iniguez AL, et al: Dynamic histone H3 epigenome marking during the intraerythrocytic cycle of Plasmodium falciparum. Proc Natl Acad Scie USA. 2009, 106 (24): 9655-9660. 10.1073/pnas.0902515106.View ArticleGoogle Scholar
- Haran TE, Mohanty U: The unique structure of A-tracts and intrinsic DNA bending. Q Rev Biophys. 2009, 42 (1): 41-81. 10.1017/S0033583509004752.View ArticlePubMedGoogle Scholar
- Suter B, Schnappauf G, Thoma F: Poly(dA.dT) sequences exist as rigid DNA structures in nucleosome-free yeast promoters in vivo. Nucleic Acids Res. 2000, 28 (21): 4083-4089. 10.1093/nar/28.21.4083.PubMed CentralView ArticlePubMedGoogle Scholar
- Yaragatti M, Basilico C, Dailey L: Identification of active transcriptional regulatory modules by the functional assay of DNA from nucleosome-free regions. Genome Res. 2008, 18 (6): 930-938. 10.1101/gr.073460.107.PubMed CentralView ArticlePubMedGoogle Scholar
- Watanabe J, Sasaki M, Suzuki Y, Sugano S: Analysis of transcriptomes of human malaria parasite Plasmodium falciparum using full-length enriched library: identification of novel genes and diverse transcription start sites of messenger RNAs. Gene. 2002, 291 (1-2): 105-113. 10.1016/S0378-1119(02)00552-8.View ArticlePubMedGoogle Scholar
- Lopez-Rubio JJ, Mancio-Silva L, Scherf A: Genome-wide analysis of heterochromatin associates clonally variant gene regulation with perinuclear repressive centers in malaria parasites. Cell Host Microbe. 2009, 5 (2): 179-190. 10.1016/j.chom.2008.12.012.View ArticlePubMedGoogle Scholar
- Gopalakrishnan AM, Nyindodo LA, Ross Fergus M, Lopez-Estrano C: Plasmodium falciparum: Preinitiation complex occupancy of active and inactive promoters during erythrocytic stage. Exp Parasitol. 2009, 121 (1): 46-54. 10.1016/j.exppara.2008.09.016.View ArticlePubMedGoogle Scholar
- Kenneth NS, Ramsbottom BA, Gomez-Roman N, Marshall L, Cole PA, White RJ: TRRAP and GCN5 are used by c-Myc to activate RNA polymerase III transcription. Proc Natl Acad Scie USA. 2007, 104 (38): 14917-14922. 10.1073/pnas.0702909104.View ArticleGoogle Scholar
- Tse C, Sera T, Wolffe AP, Hansen JC: Disruption of higher-order folding by core histone acetylation dramatically enhances transcription of nucleosomal arrays by RNA polymerase III. Mol Cell Biol. 1998, 18 (8): 4629-4638.PubMed CentralView ArticlePubMedGoogle Scholar
- Dzikowski R, Li F, Amulic B, Eisberg A, Frank M, Patel S, Wellems TE, Deitsch KW: Mechanisms underlying mutually exclusive expression of virulence genes by malaria parasites. EMBO Rep. 2007, 8 (10): 959-965. 10.1038/sj.embor.7401063.PubMed CentralView ArticlePubMedGoogle Scholar
- Trager W, Jensen JB: Human malaria parasites in continuous culture. Science. 1976, 193 (4254): 673-675. 10.1126/science.781840.View ArticlePubMedGoogle Scholar
- Lambros C, Vanderberg JP: Synchronization of Plasmodium falciparum erythrocytic stages in culture. J Parasitol. 1979, 65 (3): 418-420. 10.2307/3280287.View ArticlePubMedGoogle Scholar
- Lieb JD, Liu X, Botstein D, Brown PO: Promoter-specific binding of Rap1 revealed by genome-wide maps of protein-DNA association. Nat Genet. 2001, 28 (4): 327-334. 10.1038/ng569.View ArticlePubMedGoogle Scholar
- Schubeler D, Scalzo D, Kooperberg C, van Steensel B, Delrow J, Groudine M: Genome-wide DNA replication profile for Drosophila melanogaster: a link between transcription and replication timing. Nat Genet. 2002, 32 (3): 438-442. 10.1038/ng1005.View ArticlePubMedGoogle Scholar
- Dharia NV, Sidhu AB, Cassera MB, Westenberger SJ, Bopp SE, Eastman RT, Plouffe D, Batalov S, Park DJ, Volkman SK, et al: Use of high-density tiling microarrays to globally identify mutations and elucidate mechanisms of drug resistance in Plasmodium falciparum. Genome Biol. 2009, 10 (2): R21-10.1186/gb-2009-10-2-r21.PubMed CentralView ArticlePubMedGoogle Scholar
- Livak KJ, Schmittgen TD: Analysis of relative gene expression data using real-time quantitative PCR and the 2-ΔΔCt method. Methods. 2001, 25 (4): 402-408. 10.1006/meth.2001.1262.View ArticlePubMedGoogle Scholar
- Salanti A, Staalsoe T, Lavstsen T, Jensen AT, Sowa MP, 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. Mol Microbiol. 2003, 49 (1): 179-191. 10.1046/j.1365-2958.2003.03570.x.View ArticlePubMedGoogle Scholar
- Alkhalil A, Achur RN, Valiyaveettil M, Ockenhouse CF, Gowda DC: Structural requirements for the adherence of Plasmodium falciparum -infected erythrocytes to chondroitin sulfate proteoglycans of human placenta. J Biol Chem. 2000, 275 (51): 40357-40364. 10.1074/jbc.M006399200.View ArticlePubMedGoogle Scholar
- Lopez-Rubio JJ, Riviere L, Scherf A: Shared epigenetic mechanisms control virulence factors in protozoan parasites. Cur Opin Microbiol. 2007, 10 (6): 560-568. 10.1016/j.mib.2007.10.003.View ArticleGoogle Scholar
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