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Molecular Microbiology
 
Mol Microbiol. 2010 September; 77(5): 1237–1245.
Published online 2010 July 22. doi:  10.1111/j.1365-2958.2010.07284.x
PMCID: PMC2941730

Histone deacetylases play distinct roles in telomeric VSG expression site silencing in African trypanosomes

Abstract

African trypanosomes evade the host immune response through antigenic variation, which is achieved by periodically expressing different variant surface glycoproteins (VSGs). VSG expression is monoallelic such that only one of approximately 15 telomeric VSG expression sites (ESs) is transcribed at a time. Epigenetic regulation is involved in VSG control but our understanding of the mechanisms involved remains incomplete. Histone deacetylases are potential drug targets for diseases caused by protozoan parasites. Here, using recombinant expression we show that the essential Trypanosoma brucei deacetylases, DAC1 (class I) and DAC3 (class II) display histone deacetylase activity. Both DAC1 and DAC3 are nuclear proteins in the bloodstream stage parasite, while only DAC3 remains concentrated in the nucleus in insect-stage cells. Consistent with developmentally regulated localization, DAC1 antagonizes SIR2rp1-dependent telomeric silencing only in the bloodstream form, indicating a conserved role in the control of silent chromatin domains. In contrast, DAC3 is specifically required for silencing at VSG ES promoters in both bloodstream and insect-stage cells. We conclude that DAC1 and DAC3 play distinct roles in subtelomeric gene silencing and that DAC3 represents the first readily druggable target linked to VSG ES control in the African trypanosome.

Introduction

Trypanosoma brucei is a mono-flagellated parasitic protozoan that causes sleeping sickness in humans and Nagana in cattle. T. brucei branched very early from the eukaryotic lineage and displays some unusual features such as polycistronic transcription of protein-coding genes (Vanhamme et al., 2001). The T. brucei bloodstream-form cell surface comprises a dense variant surface glycoprotein (VSG) coat, encoded in a polycistronically transcribed telomeric VSG expression site (ES), which can periodically change to evade host immune defences (Pays, 2005). Although there are approximately 15 different telomeric VSG ESs, only one at a time is transcriptionally active (Hertz-Fowler et al., 2008). The mechanism underlying this monoallelic VSG expression remains unknown, although the telomeric location and chromatin remodelling appear to be involved; a telomere-binding protein known as repressor/activator protein 1 and a member of the ISWI family of SWI2/SNF2-related chromatin-remodelling complexes (ISWI) are required for efficient VSG ES silencing (Hughes et al., 2007; Yang et al., 2009). In addition, a dispensable histone methyltransferase (DOT1B) has a lesser role in VSG ES silencing, and is required for rapid transcriptional switching among ESs (Figueiredo et al., 2008).

Histone post-translational modifications (PTMs), in the N-terminal tails of histones in particular, play essential roles in chromatin assembly, DNA replication, recombination and repair, and transcriptional regulation (Groth et al., 2007; Kouzarides, 2007). Although T. brucei histones are divergent compared with other eukaryotes, several residues are acetylated or methylated and the functions of these PTMs may be conserved (Horn, 2007; Figueiredo et al., 2009). These histone PTMs are dynamically regulated by pairs of histone-modifying enzymes (Kouzarides, 2007). For example, histone deacetylases (HDACs) can reverse acetylation mediated by histone acetyltransferases (Drummond et al., 2005). HDACs participate in various forms of transcription repression such as telomere position effect in the yeast, Saccharomyces cerevisiae (DeRubertis et al., 1996; Rundlett et al., 1996), position-effect variegation in Drosophila (Rundlett et al., 1996) and X-chromosome inactivation in mammals (Jeppesen and Turner, 1993). HDACs are also involved in many cancers and have emerged as drug targets for chemotherapy (Drummond et al., 2005). A large number of HDAC inhibitors have been developed, and related compounds now show potential for the treatment of diseases caused by protozoan parasites (Bougdour et al., 2009).

The roles of the T. brucei class III, Sir2-related deacetylases have been explored and it has been demonstrated that SIR2rp1, the only nuclear protein of this class in T. brucei, is required for basal telomeric silencing, but not for VSG ES silencing (Alsford et al., 2007). There are also four putative zinc-dependent, class I–II HDACs in T. brucei (Ingram and Horn, 2002), including DAC1 and DAC3, which appear to be essential for growth in the bloodstream form. In this study, we characterize these HDACs and demonstrate distinct roles in telomeric and VSG ES silencing.

Results

DAC1 and DAC3 are nuclear proteins

To determine the sites of action of the various T. brucei DACs in trypanosomes, we initially established strains conditionally expressing N-terminally tagged versions of each protein (Fig. 1A). Interestingly, because we were particularly interested in the essential DAC1 and DAC3 as potential drug targets, MYCDAC1 and GFPDAC3 both accumulate in the nucleus, while MYCDAC2 and MYCDAC4 are distributed more widely and appear to be predominantly cytoplasmic (Fig. 1B); uninduced cells were consistently negative for GFP (data not shown). Further studies therefore focused on the essential, nuclear DACs. For the purpose of monitoring protein expression during RNA interference knockdown (see below), we integrated GFP tags at the DAC1 and DAC3 chromosomal loci in bloodstream-form cells. In this case, GFPDAC1 and GFPDAC3 were expressed under the control of native transcription. Once again, both proteins accumulated in the nucleus in bloodstream-form cells (Fig. S1 and see below).

Fig. 1
DAC1 and DAC3 are nuclear proteins. A. Western blot detection of tagged DACs 1–4 (arrowheads). The DACs were conditionally expressed from an ectopic locus in bloodstream-form cells. Cells were either cultured without Tet (−) or induced ...

DAC1 and DAC3 display HDAC activity

We demonstrated above that DAC1 and DAC3 are nuclear proteins in the bloodstream form. To determine whether these DACs display HDAC activity, we expressed recombinant DAC1 and DAC3 in Escherichia coli. Active, soluble DAC1 was obtained as an N-terminal MBP-fusion protein, whereas DAC3 was obtained as an N-terminal 6xHis-fusion protein. MBPDAC1 and HISDAC3 were purified by affinity chromatography (Fig. S2) and HDAC activity was determined using an in vitro assay. Both proteins displayed HDAC activity (Fig. 2A and B), which may be relatively lower for DAC1 due to the presence of additional products in this preparation (Fig. S2A). Class I–II HDACs are zinc-dependent enzymes with conserved zinc-binding residues located at the base of the catalytic pocket; one His and two Asn residues participate in zinc-ion binding (Finnin et al., 1999). The purity and yield of the DAC3 preparation facilitated mutagenesis studies and by sequence alignment, residues Asn314, His316 and Asn582 in DAC3 were predicted to be these zinc ligands (Ingram and Horn, 2002). An H316A mutation (Figs 2C and S2C) abolished HDAC activity indicating that this residue is critical for the deacetylase activity of DAC3 (Fig. 2D).

Fig. 2
DAC1 and DAC3 display HDAC activity. A. DAC1 displayed HDAC activity that was subject to inhibition by Trichostatin A (TSA, 5 µM). Activity is expressed as OD405 per mg eluted protein. Assays were done in triplicate and error bars represent one ...

DAC1 antagonizes basal telomeric silencing

In trypanosomes, many silent VSG genes are located at the telomeric end of polycistronic ESs. These transcription units have promoters that, unusually, recruit RNA polymerase I and are often located ~50 kbp from the telomere. A small number of factors have been linked to the ES promoter silencing process (Hughes et al., 2007; Figueiredo et al., 2008; Yang et al., 2009), while distinct factors are required for basal telomeric silencing, which spreads only a few kbp from the telomere (Alsford et al., 2007; Kawahara et al., 2008). We used an RNA interference (RNAi) approach to assess the role of DAC1 and DAC3 in telomeric silencing. For this assay, hairpin RNAi knockdown constructs were engineered into a strain expressing GFPDAC1 or GFPDAC3 from one of the native alleles. Induction of RNAi against DAC1 or DAC3 leads to decreased GFPDAC1 or GFPDAC3 expression, respectively, indicating efficient protein knockdown in both cases (Fig. 3A). Each knockdown was associated with a growth defect (Fig. 3B) confirming that DAC1 and DAC3 are essential for growth in the bloodstream form.

Fig. 3
RNAi confirms that DAC1 and DAC3 are essential for growth in bloodstream-form trypanosomes. A. Expression of hairpin DAC1 or DAC3 cassettes triggers specific RNAi-mediated knockdown as reported by GFPDAC1 and GFPDAC3. The asterisk indicates a non-specific ...

RNAi knockdown was then carried out in strains with an NPT reporter gene under the control of an rRNA promoter located within 2 kbp of a telomere (see Fig. 4A). Monitoring of NPT reporter expression revealed an increase in telomeric silencing specifically associated with DAC1 knockdown (Fig. 4B) and this finding was confirmed in an independent strain (data not shown) indicating that DAC1 antagonizes basal telomeric silencing. DAC1 knockdown also coincided with a growth defect in the insect stage (Fig. 4C) but knockdown had no impact on telomeric silencing in this life-cycle stage (Fig. 4D). This developmental stage-specific function for DAC1 is consistent with failure to accumulate in the nucleus in the insect, procyclic form (Fig. 4E); while GFPDAC3 subcellular localization was not substantially altered following differentiation (Fig. S1), GFPDAC1 displayed a strikingly different localization and appeared to be predominantly cytoplasmic. Cell cycle analysis also suggested a defect in DNA replication associated with DAC1 knockdown in bloodstream-form cells (Fig. S3); these cells apparently progress through mitochondrial DNA division without DNA replication.

Fig. 4
DAC1 antagonizes basal telomeric silencing in bloodstream-form trypanosomes. A. The schematic illustrates the NPT reporter under the control of an rRNA promoter located within 2 kbp of a telomere. B. Western blots showing NPT reporter expression in bloodstream-form ...

DAC3 is required for VSG ES silencing

There are approximately 15 telomeric and polycistronic VSG ESs in T. brucei. In bloodstream-form cells, all but one are reversibly repressed and the frequency of switching is very low, typically < 10−6 per population doubling (Horn and Cross, 1997). To determine whether DAC1 or DAC3 participate in transcriptional repression at VSG ESs, we generated a strain of T. brucei cells with a GFP-tagged NPT reporter immediate downstream of a reversibly silenced VSG ES promoter (Fig. 5A). We started with cells expressing VSG2, a single copy VSG on chromosome 6a (Melville et al., 2000). A construct with a Tet operator and the NPT reporter was integrated downstream of an active VSG2 ES promoter under transcription permissive conditions. Tet removal allowed the Tet repressor to bind Tet operator and block VSG2 transcription such that only cells that switch to an alternative VSG ES survive (Glover et al., 2007); these cells retain the NPT reporter downstream of the silenced VSG2 ES promoter (Fig. 5A). VSG2 ES inactivation and the capacity for reactivation were confirmed by VSG2 Western blot and GFP-NPT fluorescence analysis (data not shown).

Fig. 5
DAC3 controls VSG ES silencing. A. The schematic illustrates the silent VSG2 ES with a Tet operator and GFP:NPT reporter adjacent to a silenced promoter. These bloodstream-form cells express a second VSG (X). B. Western blots showing reporter expression ...

Subsequently, we integrated the inducible DAC1 or DAC3 hairpin RNAi knockdown constructs into these cells. For each experiment, two independent strains were analysed and results from one of each pair are shown (Fig. 5B). Expression of the NPT reporter was specifically detected following DAC3 knockdown (Fig. 5B) and this phenotype was confirmed by detection of the GFP-tag on the NPT reporter (data not shown). Next, we determined whether DAC3 influences the silencing of VSG2 located approximately 60 kbp downstream of the VSG ES promoter (Fig. 5A). Neither VSG2 protein (Fig. 5B) nor mRNA (Fig. 5C) was detected in the samples that exhibited derepression adjacent to the promoter. These results indicated that DAC3 depletion led only to derepression at the VSG ES promoter, and that transcription was subsequently attenuated. This phenotype is similar to that reported for TbISWI knockdown (Hughes et al., 2007) and is consistent with the idea that additional factors are involved in VSG ES silencing (Horn, 2009). TbSIR2rp1 mediates basal telomeric silencing, but the effect does not extend to the VSG ES promoter (Alsford et al., 2007). To explore the possibility that DAC3 and SIR2rp1 cooperate to silence VSG ESs, we disrupted both SIR2rp1 alleles in the DAC3 RNAi strain. These sir2rp1 knockouts were confirmed by PCR (data not shown). However, expression of the NPT reporter and VSG2 (Fig. 4D) were similar after DAC3 knockdown in the SIR2rp1 wild-type and sir2rp1 null strains (compare Fig. 4B and D). Parallel knockdown of both DAC3 and DAC1 did not lead to derepression of the NPT reporter (data not shown), suggesting that the DAC1 defect dominates when both deacetylases are targeted. Thus, neither SIR2rp1 nor DAC1 appear to cooperate with DAC3 to silence VSG ESs.

To ask whether DAC3 knockdown allows derepression of the VSG2 ES in insect-stage cells, we differentiated the bloodstream-form DAC3 RNAi strains. DAC3 knockdown in these cells, once again, lead to a growth defect indicating that DAC3 expression is also essential for growth in the insect stage (Fig. 5E). Similar to the situation in bloodstream-form cells, the NPT reporter was derepressed (Fig. 5F) but VSG2 remained undetectable (Fig. 5G), indicating that attenuation of transcription occurs in both life-cycle stages.

Discussion

Previous studies revealed DAC1 and DAC3 as two putative essential deacetylases in T. brucei (Ingram and Horn, 2002) that are potential targets for chemotherapy (Horn, 2008). In this study, we report characterization of these enzymes using in vitro HDAC activity assays and functional analysis in trypanosomes. Our results indicate that both DAC1 and DAC3 display HDAC activity. We further demonstrate that DAC1 antagonizes telomeric silencing in bloodstream-form cells, and that DAC3 is required for VSG ES silencing in both bloodstream and insect-stage cells.

Based on sequence similarity, cellular localization, catalytic domain and mechanism of action, HDACs are divided into four major classes (De Ruijter et al., 2003). DAC1 and DAC2 are class I, and DAC3 and DAC4 are class II (Ingram and Horn, 2002). Trypanosomes also express three class III, Sir2-related deacetylases that are dispensable for growth; only one of these is a nuclear protein (Alsford et al., 2007). In human cells, class I HDACs are typically retained in the nucleus while class II HDACs are often able to shuttle between nucleus and cytoplasm (De Ruijter et al., 2003). We show that recombinant DAC1 and DAC3 are predominantly nuclear proteins in bloodstream-form trypanosomes, while DAC2 and DAC4 are predominantly cytoplasmic. Interestingly, DAC1 displays stage-specific subcellular localization, relocalizing to the cytoplasm in insect-stage cells.

Histone deacetylases are components of complexes that play important roles in transcription repression (Yang and Seto, 2008) and these complexes likely participate in transcription regulation in trypanosomes (Figueiredo et al., 2009). For example, histone H4K10 acetylation, mediated by the histone acetyltransferase, HAT2 (Kawahara et al., 2008), marks the transcriptional start sites for RNA polymerase II (Siegel et al., 2009). In addition, the class III deacetylase, SIR2rp1 (Alsford et al., 2007) and the histone acetyltransferase, HAT1 (Kawahara et al., 2008) are required for basal telomeric silencing in these parasites but not for VSG ES silencing. We now show that DAC1 antagonizes basal telomeric silencing in bloodstream-form trypanosomes. In support of a specific role for DAC1 in this anti-silencing effect, we see that loss of this phenotype in insect-stage cells coincides with relocalization of DAC1 to the cytoplasm in this life-cycle stage. Interestingly, the class I HDACs, Rpd3 and HDAC1 play a similar telomeric anti-silencing role in yeast (Zhou et al., 2009) and in Drosophila (Doheny et al., 2008). Rpd3 has been proposed to mediate this effect by controlling the formation of transcription boundaries, which prevent Sir2-dependent silencing from spreading into euchromatic regions (Zhou et al., 2009). Thus, HAT1 and DAC1 may cooperate to regulate SIR2rp1-mediated silencing at T. brucei telomeres and this may reflect a role for histone acetylation in boundary element formation that is conserved from trypanosomes to metazoans. In this respect, it is also interesting that bloodstream-form cells defective in either HAT1 (Kawahara et al., 2008) or DAC1 (this report) also display nuclear DNA replication defects; a proportion of cells progress inappropriately through mitochondrial DNA division or mitosis in cells depleted for DAC1 or HAT1 respectively. These results suggest that the establishment of transcription boundaries is linked to DNA replication control in trypanosomes. Developmental control of DAC1 function indicates that the telomeric boundary is specific to the bloodstream form.

A small number of factors have now been linked to the process of telomeric VSG ES silencing and it was recently reported that nucleosomes are depleted at the active ES (Figueiredo and Cross, 2010; Stanne and Rudenko, 2010), but our understanding of the silencing mechanism remains incomplete. In this study, we demonstrate that DAC3 is required for VSG ES promoter silencing, but following DAC3 knockdown, transcription is attenuated through the polycistronic ES. This phenotype is observed in both life-cycle stages examined, consistent with the nuclear accumulation of DAC3 in both of these stages. Notably, a chromatin remodelling factor, TbISWI, has been linked to similar phenotypes (Hughes et al., 2007); depletion of TbISWI leads to derepression of a silent VSG ES promoter, but no derepression of VSGs at the distal end of the ES. This is consistent with the idea that ISWI remodelers organize nucleosomes at inactive regions lacking acetylation (Corona et al., 2002) but what factors are responsible for transcription attenuation within VSG ESs in the absence of TbISWI or DAC3? Our data indicate that neither SIR2rp1 nor DAC1 are required for this attenuation in DAC3-depleted cells. In fact, the only factors linked to transcription repression throughout the ES are repressor/activator protein 1 (Yang et al., 2009) and DOT1B (Figueiredo et al., 2008). Thus, transcription attenuation in cells depleted of DAC3 or TbISWI is likely to be dependent upon the action of these factors.

Histone deacetylases have emerged as potential new drug targets in protozoan parasites. Our study reveals essential HDACs in African trypanosomes that display distinct functions in antagonizing basal telomeric silencing and facilitating telomeric VSG ES silencing. These findings provide a mechanistic basis for the development of new parasite deacetylase inhibitors.

Experimental procedures

T. brucei growth and manipulation

All cells were derived from T. brucei Lister 427 bloodstream-form MITat1.2 (clone 221a). The bloodstream-form cells were grown in HMI-11, transformed with linear DNA constructs and differentiated to the insect stage in DTM as described (Alsford et al., 2005; 2007;). Drugs were added 6 h post transfection at the following concentrations: phleomycin (CayLa), 2 µg ml−1; hygromycin (Sigma), 2.5 µg ml−1; blasticidin (Invitrogen), 10 µg ml−1; G418 (MBI Fermentas), 2 µg ml−1. Induction was carried out using tetracycline (Sigma) at 1 µg ml−1. Cell counts were carried out using a haemocytometer. Cell cycle analysis and flow cytometry were carried out as described (Kawahara et al., 2008).

Plasmid construction

Genes or gene fragments were amplified by PCR from genomic DNA clones using Fusion high fidelity DNA polymerase (NEB) and specific oligonucleotides. pMalc2x (NEB) and pTrcHis-C (Invitrogen) were used for DAC1 and DAC3 expression in E. coli respectively. pRPaTAGx, pNATGFPx and pRPaiSL were used for expression of N-terminal fusion proteins and for hairpin RNAi respectively (Alsford and Horn, 2008). piGFP:NPT was derived from piRFP:PAC (Glover et al., 2007). Briefly, PAC was replaced by NPT using digestion with NotI and ClaI, and RFP was replaced by GFP using digestion with NotI and HindIII. NPT- and BLA-targeting constructs (Alsford et al., 2007) were used for SIR2rp1 disruption. Site-directed mutagenesis was carried out using the QuikChange kit according to the manufactures' instruction (Stratagene). Briefly, 35 ng of pTrcHis-DAC3 was used as a template and 2.5 U of PfuUltra high-fidelity DNA polymerase was used for amplification. PCR was run as follows: initially 95°C for 30 s; then 16 cycles of 95°C for 30 s, 55°C for 60 s, 68°C for 6 min; and final extension 5 min at 72°C. PCR product was digested with 10 U of DpnI to remove the template. The digested mixture was cleaned with StrataClean resin (Stratagene) and transfected into XL1-Blue E. coli by electroporation. pTrcHisDAC3H316A mutant clones were confirmed by sequencing. All oligonucleotide sequences are available upon request.

Expression in E. coli and purification

For MBPDAC1 expression and purification, pMalc2x-DAC1 was transformed into the protease-deficient strain, ER2508 (NEB) and cells at an OD600 of 0.5 were induced with 0.3 mM IPTG for 4 h. Protein purification was carried out according to standard procedures (NEB). For HISDAC3 and HISDAC3H316A mutant expression and purification, pTrcHis-DAC3 and pTrcHis-DAC3H316A were transformed into the BL21 strain (Invitrogen) and cells at an OD600 of 0.6 were induced with 1 mM IPTG for 2 h. Protein purification was carried out according to standard procedures (Qiagen). Protein concentrations were determined using the BCA protein assay kit (Thermo scientific). Proteins were stored in elution buffer plus 1 mM DTT and 10% glycerol at −80°C.

HDAC activity assay

DAC1 and DAC3 activity assays were carried out by HDAC Colorimetric Assay, Drug Discovery Kit according to the manufacturer's instructions (Biomol). Briefly, 20 µl assay buffer and 5 µl purified protein were added to a 96-well plate, and then 25 µl substrate was added and mixed thoroughly (final concentration is 0.5 mM). Following incubation at 37°C for 30 min, 50 µl developer solution was added and incubated for another 10 min prior to reading the OD at 405 nm.

DNA and RNA analysis

DNA sequencing was performed using a Thermo Sequenase dye terminator Kit (Applied Biosystems), a thermal cycler and an ABI Prism 377 automated sequencer according to the manufacturer's instructions. PCR and Northern analysis were carried out according to standard protocols and signals on Northern blots were quantified using a Phosphorimager (Amersham).

Protein analysis

For Western blots, whole cell lysates were separated by SDS-PAGE and electroblotted using standard protocols. Antibodies used included rabbit polyclonal α-NPT (1:2000), mouse α-cMyc 9E10 (1:2000), mouse monoclonal α-Xpress (1:5000), rabbit polyclonal α-GFP (1:4000) and rabbit polyclonal α-VSG2 (1:20000). Western blot signals were detected using an ECL + Kit (Amersham) according to the manufacturer's instructions. Immunofluorescence microscopy was carried out as described (Alsford et al., 2007). Briefly, cells were fixed with 2% formaldehyde for at least 1 h and washed twice with PBS and once with 1% BSA (in H2O) before drying on slides for at least 3 h. Cells were then permeablized with 0.5% Triton X-100 for 10 or 20 min and blocked in 30% FBS for 5 min. Indirect detection of GFP and MYC epitopes was carried out using α-GFP (1:200) and α-cMyc 9E10 (1:500) using standard protocols. Samples were mounted in Vectashield (Vector Laboratories) containing the DNA counterstain, 4′,6-diamidino-2-phenylindole. Slides were analysed on a Nikon Eclipse E600 epifluorescence microscope. Phase and fluorescence images were captured using a Coolsnap FX (Photometrics) CCD camera and processed in Metamorph 5.0 (Universal Imaging) and Photoshop Elements 2.0 (Adobe).

Acknowledgments

We thank The China Scholarship Council for studentship support for Q-P.W. (2008638024) and the Medical Research Council for studentship support for T.K. Work in D.H's laboratory is supported by The Wellcome Trust (Project Grant: 083648). We also thank LSHTM colleagues; Sam Alsford, Lucy Glover, Eiko Matsuo, Kevin Tetteh and Martin Taylor for materials, advice and protocols and also John Kelly and Sam Alsford for comments on the draft manuscript.

Supporting information

Additional supporting information may be found in the online version of this article.

Please note: Wiley-Blackwell are not responsible for the content or functionality of any supporting materials supplied by the authors. Any queries (other than missing material) should be directed to the corresponding author for the article.

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