Logo of narLink to Publisher's site
Nucleic Acids Res. 2008 Aug; 36(14): 4573–4586.
Published online 2008 Jul 8. doi:  10.1093/nar/gkn406
PMCID: PMC2504296

The RNA-binding protein TbDRBD3 regulates the stability of a specific subset of mRNAs in trypanosomes


In trypanosomes, the apparent lack of regulation of RNA polymerase II-dependent transcription initiation poses a challenge to understand how these eukaryotes adjust gene expression to adapt to the contrasting environments they find during their life cycles. Evidence so far indicates that mRNA turnover and translation are the major control points in which regulation is exerted in trypanosomes. However, very little is known about which proteins are involved, and how do they regulate the abundance and translation of different mRNAs in different life stages. In this work, an RNA-binding protein, TbDRBD3, has been identified by affinity chromatography, and its function addressed using RNA interference, microarray analysis and immunoprecipitation of mRNA–protein complexes. The results obtained indicate that TbDRBD3 binds to a subset of developmentally regulated mRNAs encoding membrane proteins, and that this association promotes the stabilization of the target transcripts. These observations raise the possibility that TbDRBD3-mRNA complexes act as a post-transcriptional operon, and provide a framework to interpret how trypanosomes regulate gene expression in the absence of transcriptional control.


Messenger RNA stability and translation are emerging as important mechanisms to control gene expression (1). These processes depend largely on RNA-binding proteins (RBPs). The association of RBPs with mRNAs is determined by sequence elements located usually within the 3′-untranslated regions (3′-UTRs) of regulated transcripts, and leads to intense changes in stability and/or translation of target mRNAs (2). Many reports have shown that RBPs do not bind to individual mRNAs randomly, but they associate with specific subsets of mRNAs coding for functionally related proteins. These observations led to the hypothesis of the existence in eukaryotes of ‘post-transcriptional operons’, by which single RBPs would be able to regulate the fate of multiple mRNAs in a coordinate manner (3,4). Indeed, an increasing number of instances exist where mRNA clusters that encode components of the same macromolecular complex or cellular process have been found associated with RBPs (4). This is best exemplified by the Puf family of RBPs in yeast, where each of the five members preferentially associates to mRNAs coding for membrane-associated proteins (Puf1p and Puf2p), mitochondrial proteins (Puf3p), ribosomal RNA-processing factors (Puf4p) or components of the spindle pole body (Puf5p) (5).

Post-transcriptional regulation of gene expression is of exceptional importance in trypanosomatid protozoa. These flagellated eukaryotes branched-out very early in the eukaryotic lineage (6), and some species, like Trypanosoma brucei, Trypanosoma cruzi or Leishmania spp., pose an important problem for the economy and public health in underdeveloped countries (http://www.who.int/tdr/diseases/). These parasites exhibit complex life cycles alternating between an invertebrate and a vertebrate, and are able to undergo intense morphological and biochemical changes in response to changes in temperature, pH, nutrients and defenses they encounter within one or the other host (7). All these adaptations require major changes in the gene expression program of the parasite. However, trypanosomatids seem to have completely lost the ability to regulate transcription initiation by RNA polymerase II (8). This is due to the unusual arrangement of chromosomes, in which most protein-coding genes are found in arrays of tens to hundreds units all orientated on the same strand (9,10). A single region seems to drive the expression of the whole chromosome (11,12), producing long polycistronic pre-mRNAs that are resolved into individual, mature mRNAs by coupled trans-splicing and polyadenylation reactions (13). Thus, regulation of gene expression in these parasites needs to be exerted posttranscriptionally. Messenger RNA processing and transport seem to be unregulated in trypanosomatids; instead, evidence so far indicates that the main control points of gene expression in these organisms are at the level of mRNA degradation and translation (8,14).

Trypanosoma brucei, the causative agent of sleeping sickness in man and nagana in cattle, has several life stages within the Tse-tse fly or the mammal. The two major replicative stages are the procyclic and the bloodstream slender forms. Transcriptome analysis of these two life forms has revealed that at least 200 transcripts show developmental regulation (15), and it is assumed that the differential transcript abundance during the parasite's life cycle is due to the interaction of RBPs to specific mRNA populations (14). Indeed, various regulatory sequences have been identified in trypanosomatids that confer stage-specific mRNA destabilization, translation or cell-cycle regulation (14), and some mRNA–protein complexes with a possible role in mRNA turnover have been partially characterized (16,17). However, virtually nothing is known about the RBPs involved in the control of mRNA abundance and translation in trypanosomatids and, to date, no RBP has been found associated with a specific subset of mRNAs coding for functionally related proteins.

The present work describes the identification of several proteins in T. brucei that bind to the 3′-UTR of a developmentally regulated mRNA in vitro, and the functional characterization of one of them, TbDRBD3. The study of TbDRBD3-depleted cells by means of RNA interference in combination with microarray analysis and immunoprecipitation of mRNA–protein complexes, indicates that this protein controls the abundance of a specific subset of developmentally regulated mRNAs encoding membrane proteins.


Trypanosomes and cell culture

Procyclic-form 427 T. brucei cells were grown at 27°C in SDM-79 medium (18) containing 10% fetal bovine serum. Procyclic-form 449 trypanosomes stably expressing the Tn10 tet repressor (19) were grown in the presence of 0.5 µg/ml phleomycin. Bloodstream-form 427 cells were cultured at 37°C and 5% CO2 in HMI-9 medium (20) containing 10% fetal bovine serum.

Purification of RBPs and mass spectrometry

To obtain cytosolic extracts, procyclic 427 cells were harvested at a cell density of 5–8 × 106/ml, washed in phosphate-buffered saline, resuspended in 1 mM HEPES, pH 7.4, 1 mM DTT and EDTA-free protease inhibitor cocktail (Roche Diagnostics, Barcelona, Spain), and disrupted for 10 min in a Potter-Elvehjem homogenizer equipped with a Teflon pestle. After adding HEPES buffer (pH 7.4) and NaCl to 20 and 100 mM, respectively, the lysate was centrifuged at 3000g for 10 min. The supernatant was ultracentrifuged for 1 h at 100 000g. NP-40, EDTA and glycerol were added to the final supernatant to 0.1% (w/v), 1 mM and 10% (w/v), respectively, and the mixture was frozen at −80°C until use. The RNA baits used were the phosphoglycerate kinase B (PGK-B) 3′-UTR and a modified version thereof in which the U-rich regulatory element was deleted (21). DNA fragments corresponding to both 3′-UTRs were PCR-amplified from plasmids pHD869 or pHD1044 (21) and cloned as EcoRI–BamHI fragments into plasmid pGR24 (a pBluescript SK+ derivative containing the sequence corresponding to the T. brucei spliced-leader cloned between the KpnI and the EcoRI sites). The resulting plasmids, named pGR25 (intact 3′-UTR) and pGR26 (deleted version) were linearized at the BamHI site and in vitro transcribed by T7 RNA polymerase. Transcribed RNAs were bridged to streptavidin–agarose columns using a biotinylated deoxyoligonucleotide complementary to the spliced-leader sequence. Cytosolic extracts (30–40 mg of protein) were thawed, supplemented with 50 µg/ml tRNA and 100 U/ml of RNasin (Promega, Madrid, Spain) and split into two identical fractions; one was passed through a column containing the intact version of PGK-B 3′-UTR, and the other through a column containing the deleted version. Proteins were allowed to bind for 20 min at room temperature, followed by an incubation of 30 min at 4°C. After extensive washing in buffer K (20 mM HEPES, pH 7.4, 100 mM NaCl, 1 mM DTT, 1 mM EDTA, 0.1% NP-40, 10% glycerol), RBPs were eluted in buffer K containing 500 mM NaCl, loaded in a 12% SDS–PAGE gel and visualized by Sypro Ruby staining. Those proteins appearing only in the intact 3′-UTR chromatography eluate were excised, subjected to MALDI-TOF/TOF and identified using MASCOT software (http://www.matrixsicence.com). Mass-spectrometry analysis was performed in the Proteomic Unit of the Scientific Park/Madrid Complutense University (Madrid, Spain).

Antibody production

A fragment of the TbDRBD3 open reading frame (ORF) corresponding to the first 83 amino acids, or a fragment of TbRBP33 corresponding to the last 160 amino acids, were cloned into pHD1306 (22), expressed as His6-GST fusions, purified using glutathione- and nickel-affinity resins, and buffer exchanged into phosphate-buffered saline. Immunizations in rabbits were performed according to standard procedures (23). Polyclonal antibodies were affinity-purified using full-length versions of the proteins coupled to AffiGel-15 (Bio-Rad Laboratories, Madrid, Spain). To express full-length TbDRBD3 and TbRBP33 in Escherichia coli for antibody purification, ORFs were cloned into pGR36 (a pET24a derivative containing a DNA fragment coding for the calmodulin-binding peptide and the His6 tag cloned between the HindIII and XhoI sites). Bacteria were grown at room temperature to an OD600 of 0.2, induced with 1 mM isopropyl-β-d-thiogalactopyranoside and incubated at the same temperature to an OD600 of 1.5. Recombinant proteins were purified using both calmodulin-affinity (Stratagene, La Jolla, CA, USA) and nickel-affinity (GE Healthcare, Barcelona, Spain) resins, according to the manufacturers’ instructions. Western blots of total cell extracts were done as described (24).

Immunofluorescence assays

Immunolocalization studies in bloodstream and procyclic 427 trypanosomes were carried out in cells fixed with 4% paraformaldehyde and permeabilized with 0.2% Triton X-100 for 20 min (22), using affinity-purified anti-TbDRBD3 serum and goat anti-rabbit Alexa 488 secondary antibody (Molecular Probes, Invitrogen, Barcelona, Spain). Permeabilization with Igepal CA-630 (25), or fixation/permeabilization with methanol [using the protocol described in ref. (26), but substituting methanol for ethanol] gave similar results.

RNA interference

A stem–loop strategy was used to generate dsRNA (27). A fragment of the TbDRBD3 ORF corresponding to nucleotide positions 2–502 was PCR-amplified and cloned into pGR19 (27) as two inverted repeats flanked by an ‘stuffer’ fragment to yield pGR69. There are no other sequences in the T. brucei genome that showed significant similarity to this dsRNA. Procyclic 449 cells were transfected with pGR69 linearized with NotI and selected in the presence of 50 µg/ml hygromycin. RNAi was induced by adding tetracycline to the culture medium at a concentration of 1 µg/ml.

Microarray analysis

RNAi was induced for 48 h, and total RNA was obtained from either uninduced or TbDRBD3-depleted cells using Trizol (Invitrogen, Barcelona, Spain) and treated with DNase I (Promega). A total of 15 µg of RNA were reverse transcribed in the presence of 100 ng of oligo(dT)12–18, 0.25 mM dATP, 0.25 mM dTTP, 0.25 mM dGTP, 0.05 mM dCTP, 0.05 mM Cy3- or Cy5-dCTP, 50 mM Tris–HCl, pH 8.3, 75 mM KCl, 3 mM MgCl2, 5 mM DTT, 40 U of RNaseOUT (Invitrogen) and 400 U of Superscript III reverse transcriptase (Invitrogen). Reactions were incubated for 3 h at 50°C, stopped by heating at 70°C for 15 min and treated with 5 U of RNase H for 20 min at 37°C. cDNA was purified using the MinElute kit (Qiagen, Madrid, Spain), ethanol precipitated and resuspended in hybridization buffer. Genomic T. brucei microarray glass slides containing ca. 24 000 independent random genomic clones (15) were pre-hybridized and hybridized as described (28). Four hybridizations (two biological replicates with a dye swap each) were analyzed. Slides were scanned using a ScanArray 5000 laser-scanner (Packard BioScience, Dreieich, Germany). The resulting images were analyzed using GenePix (Axon Instruments, Sunnyvale, CA, USA) and MCHIPS software (29,30) essentially as described (15,28). Only those clones satisfying the following parameters—fitted intensities: at least 150 000; ratio: ±2; min/max-separation: 0.1—were selected. Regulated clones were sequenced from one end and identified in the T. brucei genome database (http://www.genedb.org/genedb/tryp/). Microarray data have been submitted to GEO under accession number GSE8734.

Northern analysis

A 10–15 µg of total RNA obtained from three independent RNAi experiments were electrophoresed in agarose–formaldehyde gels, transferred to Nytran membranes (Millipore, Madrid, Spain), hybridized following standard procedures (31) and analyzed using PhosphorImager screens and ImageQuant software. Transcript signals were normalized relative to a signal recognition particle (SRP) probe (32). To rule out unspecific effects on mRNA abundance due to RNAi, total RNA was also obtained from a procyclic cell line depleted of the peroxisomal protein PEX2 by means of RNAi (33) and analyzed in parallel. Table 1 shows a list of the probes used in this work.

Table 1.
Probes used in northern hybridizations

mRNA degradation experiments

Total RNA was obtained from uninduced or RNAi-induced samples (48 h in the presence of tetracycline) of 5 × 107 cells taken at different times after the addition of 10 µg/ml actinomycin D (from a stock of 5 mg/ml in DMSO). RNA extractions and analysis were performed as described above from three independent RNAi inductions. mRNA half-lives were estimated after measuring PhosphorImager signals on northern blots, normalizing to SRP signal, plotting on semilogarithmic scales and calculating the amount of time required for a transcript to decrease to 50% of the initial amount. Half-life values were compared using Student's t-tests. A P-value < 0.05 was considered statistically significant.

Luciferase constructs and assays

A modified version of plasmid pHD1437 (34), named pGR86, was constructed by replacing the CAT gene for a luciferase ORF. The 3′-UTRs of amino acid transporter 11 (AATP11), glutamine synthetase (GS) and actin (ACT) genes were cloned downstream the luciferase gene to generate pGR88, pGR98 and pGR108, respectively. These plasmids were digested with NotI and stably integrated in the tubulin locus of procyclic trypanosomes by electroporation. After selecting in the presence of 1 µg/ml puromycin, three independent clones from each transfection were selected for northern and luciferase assays. AATP11 3′-UTR was obtained from plasmid pHD1470 (35), and ACT 3′-UTR, from plasmid pHD1034 (36). GS 3′-UTR was obtained by RT–PCR using the anchored oligo(dT)18 primer CZ1584 (36) and GS gene-specific primers. Total protein extracts from 2 × 106 cells were assayed for luciferase activity in a Berthold FB 12 luminometer (Berthold Detection Systems GmbH, Pforzheim, Germany) using the Luciferase Assay System (Promega) according to the manufacturer's instructions.

Immunoprecipitation of mRNA–protein complexes

For each immunoprecipitation, 5 × 107 procyclic 427 cells were washed in serum-free SDM-79 culture medium and lyzed in 10 mM Tris–HCl, pH 7.4, 2 mM DTT, 0.1% (w/v) NP-40, 100 U/ml RNasin (Promega), 2 mM vanadyl ribonucleoside complexes (Sigma-Aldrich, Madrid, Spain) and EDTA-free protease inhibitor cocktail (Roche Diagnostics) using a Potter-Elvehjem homogenizer equipped with a Teflon pestle. After adding NaCl to 150 mM, the lysate was centrifuged at 4°C for 15 min at 14 000g. The supernatant was subjected immediately to immunoprecipitation using protein G beads and affinity-purified antibodies for 3 h at 4°C. After extensive washing in 10 mM Tris–HCl, pH 7.4, 150 mM NaCl, 0.1% (w/v) NP-40, the RNA was extracted from the immunoprecipitated material using TRI-Reagent (Sigma-Aldrich) and treated with DNase I. One half of the final RNA sample was reverse transcribed using the anchored oligo(dT)18 primer CZ1584 (36) and Superscript III reverse transcriptase (Invitrogen); the other half was treated identically, except that the reverse transcriptase was omitted (minus RT control). cDNA was amplified using mRNA-specific primers pairs and 95°C (30 s), 55°C (30 s) and 72°C (30 s) for 30 cycles, then 5 min at 72°C. Total RNA was also obtained from an equivalent amount of extract to serve as a positive control (input RNA). Control immunoprecipitations and RT–PCR experiments were performed in parallel using either anti-TbRBP33 antibodies or purified rabbit IgGs (Sigma-Aldrich). To test the effect that deletions in the 3′-UTR of AATP11 mRNA have on TbDRBD3 binding, mRNA–protein complexes were also immunoprecipitated from extracts obtained from permanent cell lines expressing CAT reporter mRNAs fused to different deletions of AATP11 3′-UTR (35). In this case, cells were disrupted by vortexing in the presence of 0.5% Igepal CA-630. PCR reactions were carried out using the sense oligonucleotide 5′-GCAAGGCGACAAGGTGCTGATGC-3′ that hybridizes close to the 3′-end of CAT ORF, and the antisense primer 5′-GCAGCTCAGTGTCTCTATAAATCAATGC-3′, which is complementary to a region present in all deletions (nucleotides 261–289, see Figure 7B).

Figure 7.
TbDRBD3 associates with target transcripts in vivo. (A) mRNA–protein complexes were immunoprecipitated from T. brucei extracts using anti-TbDRBD3 antibodies. The presence of different transcripts in the complexes was assessed by RT–PCR, ...


Identification of proteins that bind to the 3′-UTR of PGK-B mRNA

There are very few RNA cis-acting elements identified in T. brucei that determine regulation of gene expression (8,14) and that could be used as baits for RNA-affinity purification. One of them is a sequence located in the 3′-UTR of the PGK-B mRNA, which resembles mammalian regulatory AU-rich elements (21). Versions of this 3′-UTR containing or lacking the regulatory element were bound to streptavidin–agarose beads (see Materials and methods section). RBPs able to bind the intact 3′-UTR but not the version lacking the regulatory sequence were affinity-purified from procyclic cytosolic extracts, resolved in SDS–PAGE gels, stained with Sypro Ruby (Figure 1A) and identified by MALDI-TOF/TOF (Figure 1B). The protein band migrating at approximately 40 kDa consisted of a mixture of three polypeptide species, TbDRBD3, TbRBP33 and Tb927.6.4440, whereas the protein band migrating at ∼22 kDa was identified as TbUBP2. The latter is a putative homolog of TcUBP2, an RBP involved in the regulation of transcript abundance in trypanosomes (17,37). With the exception of Tb927.6.4440, all proteins contain canonical RNA recognition motifs (RRM) within their sequences (Figure 1B). This work concentrates in the characterization of one of these proteins, TbDRBD3. This RBP has two RRM motifs and a proline/glutamine-rich region near the C-terminus (Figure 1C). Work is in progress to characterize the other identified proteins following the experimental approach described in this article.

Figure 1.
Identification of proteins that bind to PGK-B 3′-UTR. (A) Procyclic cytosolic extracts were chromatographed on streptavidin–agarose columns containing the PGK-B 3′-UTR (lane 1) or a version lacking the regulatory sequence (lane ...

Subcellular localization of TbDRBD3 and effects of RNA interference on trypanosome growth

Polyclonal antibodies were raised in rabbits against TbDRBD3. The affinity-purified antiserum recognized a single band of ∼40 kDa in total cell extracts, which was similarly expressed in bloodstream and procyclic trypanosomes (Figure 2A). This protein band decreased clearly in intensity after induction of RNAi targeting TbDRBD3 mRNA (Figure 3B, see below). TbDRBD3 was found predominantly in the cytosol of wild-type bloodstream and procyclic cells, as observed by immunofluorescence microscopy, although some signal could also be observed within the nucleus (Figure 2B). TbDRBD3 fluorescence signal decreased to background levels after induction of RNAi (Supplementary Figure 1A). Different permeabilization/fixation protocols gave similar staining patterns (Supplementary Figure 1B). The localization of TbDRBD3 was also analyzed by subcellular fractionation (Figure 2C). In this case, the protein was found in both the nuclear and the cytosolic fractions. Taken together, these results indicate that TbDRBD3 can be found in both compartments, with a predominant cytosolic localization.

Figure 2.
TbDRBD3 is expressed in bloodstream and procyclic trypanosomes and localizes in both the cytosol and the nucleus. An affinity-purified anti-TbDRBD3 antiserum was used to detect the protein by (A) western blot analysis of total cell extracts or (B) immunofluorescence ...
Figure 3.
Depletion of TbDRBD3 by RNA interference and effects on growth. A cell line was generated that expressed TbDRBD3-specific dsRNA in a tetracycline-inducible manner. The levels of TbDRBD3 mRNA (A) or protein (B) were analyzed in cells incubated with tetracycline ...

To study the function of TbDRBD3 in procyclic trypanosomes, the protein was depleted in vivo using RNA interference in a tetracycline-inducible manner. A marked reduction of both mRNA and protein levels was readily observed after 48 h of tetracycline induction (Figure 3A and B). As seen in Figure 3C, depletion of TbDRBD3 resulted in a growth arrest phase followed by cell death.

TbDRBD3 regulates the abundance of a specific subset of mRNAs coding for membrane transporters and intermediate metabolism enzymes

In order to analyze whether TbDRBD3 has a role in the regulation of mRNA turnover, the transcriptome of procyclic trypanosomes depleted of TbDRBD3 was compared to that of uninduced cells using genomic microarrays. RNA samples were isolated from cells harvested after 48 h of induction with tetracycline. At this point, cell growth was barely affected (Figure 3C) and trypanosomes remained highly motile (data not shown). Thirty-four regulated spots showed reproducible regulation in TbDRBD3-depleted cells (see Supplementary Figure 2 and Materials and methods section), which already suggested that TbDRBD3 was involved in the regulation of the abundance of a small group of mRNAs. All clones were sequenced and found to encode 22 proteins, including TbDRBD3 itself (Figure 4A). Regulation was confirmed by northern analysis for all tested mRNAs (Figure 4B). With the exception of a transcript encoded by the procyclin-associated gene 4 (PAG4, see below), all regulated mRNAs decreased 2- to 5-fold in abundance upon depletion of TbDRBD3. To rule out unspecific effects on mRNA abundance due to RNAi, RNA was obtained from a control RNAi cell line depleted of the peroxisomal protein PEX2 (33) and analyzed in parallel. There was no apparent effect on the abundance of any mRNA in these cells (Figure 4B).

Figure 4.
Effect of TbDRBD3 depletion on the transcriptome of T. brucei. (A) Genomic clones showing the highest regulation in microarray hybridizations after depletion of TbDRBD3. Systematic names and predicted protein products are shown according to GeneDB T. ...

Interestingly, the majority (64%) of the regulated transcripts were found to encode membrane proteins (indicated in bold face in Figure 4A). These included the amino acid transporters AATP11 and Tb927.8.7740, transporters belonging to the major facilitator superfamily (MFS), surface protein BARP (38), a putative membrane protein with high similarity to plant generative cell-specific protein 1 (GCS1) (39), trans-sialidase TbTS (40), three receptor-type adenlyate cyclases, thimet oligopeptidase A and two different pteridine transporters. There are four genes encoding pteridine transporters in the genome of T. brucei. Three are found as nearly identical tandem repeats in chromosome I, whereas a single gene is present in chromosome X that is 57% identical to its chromosome I counterparts. The mRNAs transcribed from both loci were downregulated upon depletion of TbDRBD3 (Figure 4B). Other regulated mRNAs encoded the intermediate metabolism enzymes GS and cytosolic fumarase (cFUM).

Notably, some of these mRNAs are upregulated in procyclic forms, such as the transcripts coding for pteridin transporter Tb10.6k15.1350, AATP11, trans-sialidase TbTS, thimet oligopeptidase A, GS and cFUM [(15,40,41), see also http://www.zmbh.uni-heidelberg.de/Clayton/pc_bs_OligoArray.xls, and data not shown], which suggests that TbDRBD3 is involved, at least in part, in the developmental regulation of these transcripts during the parasite's life cycle. Although not detected in the microarray analysis, the abundance of TbNT10, a purine nucleoside transporter also known to be developmentally regulated (15,42), was checked for regulation by northern analysis and found to be decreased by 2.4-fold after depletion of TbDRBD3 in procyclic forms (Figure 4B). It is also worth mentioning that mRNAs for folate transporters, which encode proteins similar to pteridine transporters (41% identical), were barely affected by TbDRBD3 depletion (Figure 4B). Likewise, the abundance of the mRNA encoding mitochondrial fumarase (mFUM), which is also upregulated in procyclic forms (41), was not affected by TbDRBD3 RNAi (Figure 4B). The differential regulation of both fumarases was also confirmed by western blot analysis using monoclonal antibodies (41) (Figure 4C). TbDRBD3 depletion did not affect the levels of either PGK-B mRNA or protein (Figure 4B and D). Moreover, PGK-B transcript was not detected in TbDRBD3 mRNP complexes (see below). These results were unexpected, since TbDRBD3 was identified based on its ability to bind PGK-B mRNA in vitro (Figure 1A), and suggest that TbDRBD3 is not likely to be involved in the regulation of PGK-B mRNA abundance. The different behavior of TbDRBD3 in vitro and in vivo could be due to posttranslational modifications, RNA secondary structure or association to other protein factors. Differential binding abilities in vitro and in vivo have been described for other RBPs (16,43).

TbDRBD3 acts by stabilizing regulated mRNAs

A possible role of TbDRBD3 could be the stabilization of target mRNAs, given the predominant cytosolic localization of the protein and the fact that most regulated transcripts decreased in abundance in TbDRBD3-depleted cells. To test this hypothesis, the decay of four regulated transcripts coding for AATP11, GS, cFUM and GCS1, was monitored in RNAi-induced cells using actinomycin D to block transcription. Degradation kinetics of the transcript coding for mFUM and ACT mRNAs, whose abundance is not altered by TbDRBD3 ablation (Figure 4B), were also analyzed as a control. As shown in Figure 5, the decreased AATP11, GS, cFUM and GCS1 mRNA steady-state levels were due, at least in part, to the lower stability of these mRNAs in cells with reduced levels of TbDRBD3. The half-lives of mFUM, ACT mRNAs were unaffected by TbDRBD3 RNAi, as expected (Figure 5E and F).

Figure 5.
Effect of TbDRBD3 depletion on the stability of transcripts encoding (A) AATP11, (B) GS, (C) GCS1, (D) cFUM, (E) mFUM, (F) ACT and (G) PAG4. Actinomycin D was added to TbDRBD3-depleted (empty circles) or uninduced trypanosomes (filled circles). RNA samples ...

The decay of PAG4, the only transcript whose abundance increased upon TbDRBD3 ablation (Figure 4A and B), was also analyzed. As seen in Figure 5G, no apparent changes in the stability of PAG4 transcript could be detected in TbDRBD3-depleted cells. PAG4 gene is located at the end of a polycistronic unit transcribed by RNA polymerase I (in trypanosomes there are a few protein-coding genes that are transcribed by this polymerase). This unit also contains three other PAG genes, and begins with two genes coding for main surface proteins in the procyclic stage, the procyclins EP1 and EP2 (44). The steady-state levels of PAG transcripts are over two orders of magnitude lower than those of EPs (45). Depletion of TbDRBD3 in procyclic forms also resulted in an increase in the abundance of the other PAG transcripts, but EP1 and EP2 mRNA levels remained unchanged (Figure 4B and data not shown). Since EPs and PAGs genes are transcribed in the same polycistronic unit, these results suggest that TbDRBD3 depletion affects pre-mRNA processing or transcription elongation. However, PAG4 mRNA could not be detected in TbDRBD3–mRNA complexes (see below), and therefore the increase in the abundance of this transcript could be an indirect effect of TbDRBD3 depletion, for example, due to a drop in the intracellular levels of amino acids or other metabolites transported by the membrane proteins whose mRNAs are regulated by TbDRBD3 (see Discussion section).

TbDRBD3-dependent regulation is mediated through sequences localized in the 3′-UTR

Regulation of mRNA abundance is usually determined by sequences found in the 3′-UTR of target transcripts (46). To investigate whether the same is true for TbDRBD3, the 3′-UTRs of two regulated transcripts, AATP11 and GS, were placed downstream of a luciferase reporter gene and stably integrated in the TbDRBD3 RNAi cell line. As shown in Figure 6, a ca. 3-fold reduction in the steady-state abundance of luciferase mRNA could be observed upon depletion of TbDRBD3. As expected, the levels of a reporter mRNA bearing ACT 3′-UTR were unaffected by TbDRBD3 ablation. Reduction in luciferase activity, although evident, was not as marked as for mRNA levels, which could be due to the high stability of luciferase within T. brucei cells (47) or to a more efficient translation of decreased mRNA levels to sustain the overall levels of the protein. Decay kinetics of LUC-AATP11 and LUC-ACT reporter mRNAs were also analyzed (Figure 6C and D). The half-life values of both mRNAs measured in uninduced cells were lower than those observed for the respective endogenous mRNAs (i.e. compare Figure 5A with Figure 6C and Figure 5F with Figure 6D), which could be due to intrinsic instability of luciferase transcript in trypanosome cells. Importantly, the half-life of LUC-AATP11 mRNA was significantly decreased in cells with reduced levels of TbDRBD3 (Figure 6C). Decay of LUC-GS reporter mRNA could not be analyzed due to the very short half-life of this transcript (<5 min, data not shown). The half-life of LUC-ACT mRNA was unaffected by TbDRBD3 RNAi, as expected (Figure 6D).

Figure 6.
TbDRBD3 knockdown affects the abundance of reporter mRNAs bearing AATP11 and GS 3′-UTRs. Expression vectors containing a luciferase gene (LUC) fused to 3′-UTRs of AATP11, GS or ACT mRNAs were stably integrated into TbDRBD3 RNAi procyclic ...

TbDRBD3 is found in a ribonucleoprotein complex containing target mRNAs

Proteins that regulate the degradation and translation of mRNAs are found associated with their target mRNAs to form ribonucleoprotein complexes (mRNPs) (4), and indeed it was also the case for TbDRBD3, as judged by immunoprecipitation assays and RT–PCR analysis. As shown in Figure 7A, most of the downregulated mRNAs were effectively amplified from TbDRBD3 immunoprecipitated material. These include transcripts coding for AATP11, both pteridine transporters, the adenosine transporter NT10 and the GCS1 protein. cFUM mRNA was barely detectable in the TbDRBD3 sample, whereas GS mRNA) could not be amplified; therefore, the observed changes in the abundance of cFUM and GS mRNAs upon TbDRBD3 depletion could be explained by loose association to the mRNP complex or by indirect effects due to changes in cell metabolism (see Discussion section). PGK-B and PAG4 mRNAs were not detected in this assay either, indicating that TbDRBD3 does not interact with these mRNAs in vivo. Immunoprecipitation analyses using either an antiserum raised against a different RBP, TbRBP33, or purified rabbit IgGs, yielded undetectable or low-level amplification signals (Figure 7A).

No signal could be detected for transcripts encoding mFUM and ACT, two transcripts that were not regulated by TbDRBD3 (see above), underscoring the specificity of TbDRBD3–mRNA interactions. In addition, a chloramphenicol acetyl transferase (CAT) reporter mRNA could be immunoprecipitated if fused to the 3′-UTR of AATP11, but not when ACT 3′-UTR was used (Figure 7B). Most importantly, when reporter CAT mRNAs bearing different deletions of AATP11 3′-UTR were tested (35), it was observed that a region encompassing nucleotides 290–618 was required to immunoprecipitate the reporter mRNA (Figure 7B), indicating that TbDRBD3 binds specifically to sequences and/or structural elements within this particular region. Deletion of nucleotides 260–618 did not result in changes in the abundance of the mRNA [Figure 7C, (35) and data not shown]. Since the analyzed CAT reporter transcripts seem to have altered polyadenylation patterns (35), the transcription of a reporter mRNA with deletion 290–618 could result in the production of an mRNA with an aberrant 3′-UTR that makes it less prone to degradation.


There have been major advances in elucidating the mechanism of mRNA degradation in trypanosomes in vivo (36,48–51). However, information about RBPs responsible for the differential abundance of mRNAs during the parasite's life cycle is still very scarce. In this work, an RBP, TbDRBD3, was identified based on its ability to bind the 3′-UTR of PGK-B mRNA in vitro. Depletion of TbDRBD3 by means of RNAi resulted in a decrease in the steady-state abundance of a specific group of mRNAs encoding membrane proteins and intermediate metabolism enzymes, as seen by microarray and northern analysis. The small number of regulated transcripts, and the fact that the abundance of other mRNAs encoding similar proteins was not apparently affected, highlights the specificity of TbDRBD3-dependent regulation. The results obtained from reporter mRNAs bearing different 3′-UTRs, from the decay rates of several regulated transcripts, and from the immunoprecipitation analysis all suggest that TbDRBD3 binds target mRNAs and protects them from degradation. The fact that a reporter mRNA fused to the 3′-UTR of AATP11 could be efficiently immunoprecipitated using anti-TbDRBD3 antibodies (Figure 7B) suggests that TbDRBD3-binding site/s localize within the 3′-UTR of regulated transcripts. In the case of AATP11 3′-UTR, the binding region seems to be located within nucleotides 290 and 618 (Figure 7B). Interestingly, this region was shown to be important for developmental regulation of AATP11 transcript, but shorter sequence motifs could not be identified (35). All regulated mRNAs found to be associated with TbDRBD3 contain the UAUUUUUU element shown to be overrepresented among mRNAs that are more abundant in the procyclic stage (52). Since the motif is also present in the PGK-B regulatory sequence used to identify TbDRBD3 (Figure 1) (21), it is possible that this protein has affinity towards U-rich elements. Indeed, there is an UAUUUUUU motif within nucleotides 290 and 618 in AATP11 3′-UTR (35). However, this motif is also found in many other transcripts that were not detected in the microarray analysis. Moreover, two of these mRNAs, encoding GS and mFUM, contain UAUUUUUU sequences within their 3′-UTRs, and they do not bind to TbDRBD3, as shown in Figure 7A. Taken together, these observations suggest that there are additional sequence and/or secondary structure determinants that are required for TbDRBD3 to bind to its target mRNAs. This is a likely possibility, since TbDRBD3 contains two RNA-binding domains (Figure 1), and some of such RBPs are able to recognize a long binding platform or to bind simultaneously to distantly positioned sequence motifs within the same RNA molecule (53).

Due to its cytosolic localization, TbDRBD3 could inhibit deadenylation (the first step in the mRNA degradation pathway) by modulating the affinity of the poly(A)-binding protein to the poly(A) tail of regulated transcripts (1). Since TbDRBD3 was also detected in the nucleus of trypanosomes, this protein could additionally facilitate the transport of target transcripts from the nucleus to the cytoplasm, as it has been proposed for ELAV/Hu stabilizing proteins (54).

AATP11, PTX, NT10, TbTS and cFUM mRNAs are abundant in the procyclic (insect) form of the parasite and downregulated in bloodstream forms. Therefore, TbDRBD3-mediated stabilization could be responsible, at least in part, for the developmental regulation of the abundance of these transcripts during T. brucei life cycle. Interestingly, TbDRBD3 is similarly expressed in both life forms. Thus, downregulation of the aforementioned transcripts in bloodstream trypanosomes cannot be due to a drop in the levels of TbDRBD3 in the mammalian stage. Instead, TbDRBD3 binding ability could be modulated in different life forms as the result of stage-specific posttranslational modifications, differential RNA secondary structure or association with distinct protein partners.

Importantly, TbDRBD3 was found to be associated with regulated transcripts in mRNA–protein complexes in vivo, which indicates that the stability of all bound transcripts is coordinately regulated, and that TbDRBD3–mRNA particles act as an posttranscriptional operon, as it has been proposed for other RBPs in yeast and mammals (4). The presence of RNA operons in such divergent eukaryotes suggests that this kind of complexes were beneficial and ancient modules that conferred additional and advantageous flexibility in the regulation of gene expression early in the eukaryotic lineage.

Yeast Puf proteins are probably the best example of a posttranscriptional operon (4,5). Interestingly, 52–57% of the mRNAs identified in yeast Puf1p and Puf2p mRNPs complexes were found to encode membrane proteins, and over 60% of the mRNAs regulated by TbDRBD3 depletion also code for membrane proteins. Some of them are known to be involved in the transport of small molecules such as amino acids, biopterin or adenosine nucleosides. Tb927.7.5960 protein is probably involved in metabolite transport as well, since it contains the MFS motif present in a great variety of small molecule transporters (55). Protein Tb10.406.0110 is similar to plant GCS1, a membrane protein involved in pollen tube guidance and fertilization (39,56). The role of this protein in trypanosomes is unknown, but it might transduce environmental cues, as it has been proposed for plants (56). There are about sixty genes that encode putative receptor-type adenylate cyclases in the T. brucei genome. Three of them, sharing identities of 44–48%, seem to be regulated by TbDRBD3 depletion, according to microarray data. Receptor-type adenylate cyclases in trypanosomes appear to function as enzyme-linked cell surface receptors involved in cAMP signalling (57). All these observations give reason to think that TbDRBD3 regulates at the mRNA turnover level a group of membrane proteins involved in signal transduction and transport in an orchestrated and stage-specific manner. Whether or not the transported molecules converge in a common metabolic pathway is a matter of future research. The amino acid specificity of AATP11 transporter is not known. Since GS mRNA is also downregulated in procyclic TbDRBD3-depleted cells, and this enzyme catalyzes the interconversion of glutamate and glutamine, it is possible that AATP11 transports glutamine, glutamate or both. Glutamate and glutamine are the sources of all cellular nitrogen (58), and in trypanosomes they could act as precursors of pyrimidines, polyamines, folylpolyglutamates and trypanothione (a thiol equivalent to glutathione in trypanosomes). Interestingly, a proposed role for cFUM in trypanosomes is to provide fumarate for the de novo synthesis of pyrimidines (41,59), so the possibility exists that TbDRBD3 not only regulates nutrient transport but also the biosynthesis of nitrogen compounds. However, the mRNA coding for GS could not be detected in TbDRBD3–mRNA complexes, and the transcript encoding cFUM was barely detectable. Although these results can be explained by a lower affinity of TbDRBD3 towards these particular mRNAs, it is also plausible that (as in the case of PAGs transcripts described in the Results section) the reduction in the levels of both mRNAs in TbDRBD3-depleted cells is the indirect consequence of nutrient starvation due to reduced transport activities. Interestingly, the expression of GS is controlled by the intracellular concentration of glutamine in yeast (58). Alternatively, TbDRBD3 could regulate the abundance of an mRNA (not necessarily any of those shown in this work), which in turn would control GS, cFUM and PAG4 transcripts. Be what it may, regulation of the expression of GS and cFUM seems to be exerted, at least in part, at the mRNA degradation level, since the half-lives of both transcripts decreased upon depletion of TbDRBD3 (Figure 5).

The apparent absence of RNA polymerase II-dependent transcriptional regulation, the very unusual chromosomal organization and the pre-mRNA processing mechanism involving coupled trans-splicing and polyadenylation reactions all pose a challenge to understand how trypanosomes regulate gene expression. The functional characterization of TbDRBD3 described in this work illustrates how it can be achieved, and provides a framework to study posttranscriptional regulation in these parasites. Thus, trypanosome genes could be simultaneously controlled at the mRNA level by association of transcripts encoding stage-specific, functionally linked or cytotopically related proteins to regulatory RBPs, as per the posttranscriptional operon hypothesis (3,4).

The finding that TbDRBD3 is an essential protein, which associates with a specific group of mRNAs underscores the importance of this RBP in posttranscriptional regulation of gene expression in trypanosomes, and opens up the realistic possibility of discovering additional mRNA–protein complexes with a role in the control of transcript abundance and/or translation. Due to the high degree of conservation of RBPs among different organisms, the potential of these proteins as antitrypanosomal drug targets is dubious, but that might not be the case for the proteins encoded by the regulated mRNAs. In fact, pteridine transporters, trans-sialidase and cFUM, whose transcripts show TbDRBD3-dependent regulation, are known to be important in cell viability, virulence and infectivity in trypanosomatids (41,60–62). Thus, the study of RNA operons in trypanosomes should be of great help in the identification of essential proteins amenable to drug inhibition.

With over 100 predicted RBPs of unknown function in the trypanosomes genomes (14,63), new cis-acting motifs discovered (52,64–66) and the experimental approaches described in this work, the identification of RBPs acting as ‘posttranscription factors’ in trypanosomes should be a feasible task.


Supplementary Data are available at NAR Online.

[Supplementary Data]


The author is indebted to Dolores González-Pacanowska and Luis M. Ruiz-Pérez for providing laboratory facilities to carry out most of this work; to Christine Clayton for cell lines, plasmids and specially for providing bench space and reagents for microarray hybridizations; to Stefanie Brems and Jörg Hoheisel for microarray slides and to Van-Duc Luu for his assistance with microarray analysis. Stefanie Brems, Jörg Hoheisel and Christine Clayton are also thanked for making available trypanosome stage-specific gene expression microarray data. The author is also grateful to Frédéric Bringaud for anti-fumarase antibodies; to Paul A. M. Michels for anti-PGK antibodies; to Noreen Williams for anti p34/37 serum; to Keith Gull for providing a monoclonal anti-α-tubulin antibody; to Juan D. Alfonzo, José A. García-Salcedo and Asunción Delgado for critical reading of the article and to TIGR and The Wellcome Trust Sanger Institute for making the T. brucei genome sequencing project data available. This work was supported by Spanish Plan Nacional (BMC2003-05037 and BFU2006-12080); European Molecular Biology Organization (short-term fellowship ASTF109-2006 to visit Christine Clayton's laboratory, ZMBH, Heidelberg, Germany); Deutsche Forschungsgemeinschaft (SFB544 to Christine Clayton, consumables for the microrray analysis). The author is the recipient of a Ramón y Cajal research contract from Spanish Ministerio de Educación y Ciencia. Funding to pay the Open Access publication charges for this article was provided by Spanish Plan Nacional (BFU2006-12080).

Conflict of interest statement. None declared.


1. Wilusz CJ, Wormington M, Peltz SW. The cap-to-tail guide to mRNA turnover. Nat. Rev. Mol. Cell Biol. 2001;2:237–246. [PubMed]
2. Barreau C, Paillard L, Osborne HB. AU-rich elements and associated factors: are there unifying principles? Nucleic Acids Res. 2005;33:7138–7150. [PMC free article] [PubMed]
3. Keene JD, Tenenbaum SA. Eukaryotic mRNPs may represent posttranscriptional operons. Mol. Cell. 2002;9:1161–1167. [PubMed]
4. Keene JD. RNA regulons: coordination of post-transcriptional events. Nat. Rev. Genet. 2007;8:533–543. [PubMed]
5. Gerber AP, Herschlag D, Brown PO. Extensive association of functionally and cytotopically related mRNAs with Puf family RNA-binding proteins in yeast. PLoS Biol. 2004;2:342–354. [PMC free article] [PubMed]
6. Fernandes AP, Nelson K, Beverley SM. Evolution of nuclear ribosomal RNAs in kinetoplastid protozoa: perspectives on age and origins of parasitism. Proc. Natl Acad. Sci. USA. 1993;90:11608–11612. [PMC free article] [PubMed]
7. Vickerman K. Developmental cycles and biology of pathogenic trypanosomes. Br. Med. Bull. 1985;41:105–114. [PubMed]
8. Clayton CE. Life without transcriptional control? From fly to man and back again. EMBO J. 2002;21:1881–1888. [PMC free article] [PubMed]
9. Ivens AC, Peacock CS, Worthey EA, Murphy L, Aggarwal G, Berriman M, Sisk E, Rajandream MA, Adlem E, Aert R, et al. The genome of the kinetoplastid parasite, Leishmania major. Science. 2005;309:436–442. [PMC free article] [PubMed]
10. Myler PJ, Audleman L, deVos T, Hixson G, Kiser P, Lemley C, Magness C, Rickel E, Sisk E, Sunkin S, et al. Leishmania major Friedlin chromosome 1 has an unusual distribution of protein-coding genes. Proc. Natl Acad. Sci. USA. 1999;96:2902–2906. [PMC free article] [PubMed]
11. Martínez-Calvillo S, Nguyen D, Stuart K, Myler PJ. Transcription initiation and termination on Leishmania major chromosome 3. Eukaryot. Cell. 2004;3:506–517. [PMC free article] [PubMed]
12. Martínez-Calvillo S, Yan S, Nguyen D, Fox M, Stuart K, Myler PJ. Transcription of Leishmania major Friedlin chrosomose 1 initiates in both directions within a single region. Mol. Cell. 2003;11:1291–1299. [PubMed]
13. Liang XH, Haritan A, Uliel S, Michaeli S. Trans and cis splicing in trypanosomatids: mechanism, factors, and regulation. Eukaryot. Cell. 2003;2:830–840. [PMC free article] [PubMed]
14. Hendricks EF, Matthews K. Post-transcriptional control of gene expression in African trypanosomes. In: Barry D, McCulloch R, Mottram J, Acosta-Serrano A, editors. Trypanosomes: After the Genome. Norwich, UK: Horizon Bioscience; 2007. pp. 209–37.
15. Brems S, Lys Guilbride D, Gundlesdodjir-Planck D, Busold C, Luu VD, Schanne M, Hoheisel J, Clayton C. The transcriptomes of Trypanosoma brucei Lister 427 and TREU927 bloodstream and procyclic trypomastigotes. Mol. Biochem. Parasitol. 2005;139:163–172. [PubMed]
16. De Gaudenzi JG, D’Orso I, Frasch AC. RNA recognition motif-type RNA-binding proteins in Trypanosoma cruzi form a family involved in the interaction with specific transcripts in vivo. J. Biol. Chem. 2003;278:18884–18894. [PubMed]
17. Hartmann C, Benz C, Brems S, Ellis L, Luu VD, Stewart M, D’Orso I, Busold C, Fellenberg K, Frasch AC, et al. The small trypanosome RNA-binding proteins TbUBP1 and TbUBP2 influence expression of F-box protein mRNAs in bloodstream trypanosomes. Eukaryot. Cell. 2007;6:1964–1978. [PMC free article] [PubMed]
18. Brun R, Schönenberger M. Cultivation and in vitro cloning of procyclic culture forms of Trypanosoma brucei in a semi-defined medium. J. Protozool. 1979;36:289–292. [PubMed]
19. Biebinger S, Wirtz LE, Lorenz P, Clayton C. Vectors for inducible expression of toxic gene products in bloodstream and procyclic Trypanosoma brucei. Mol. Biochem. Parasitol. 1997;85:99–112. [PubMed]
20. Hirumi H, Hirumi K. Continuous cultivation of Trypanosoma brucei bloodstream forms in a medium containing a low concentration of serum protein without feeder cell layers. J. Parasitol. 1989;75:985–989. [PubMed]
21. Quijada L, Guerra-Giraldez C, Drozdz M, Hartmann C, Irmer H, Ben-Dov C, Cristodero M, Ding M, Clayton C. Expression of the human RNA-binding protein HuR in Trypanosoma brucei increases the abundance of mRNAs containing AU-rich regulatory elements. Nucleic Acids Res. 2002;30:4414–4424. [PMC free article] [PubMed]
22. Haile S, Cristodero M, Clayton C, Estevez AM. The subcellular localisation of trypanosome RRP6 and its association with the exosome. Mol. Biochem. Parasitol. 2007;151:52–58. [PubMed]
23. Harlow E, Lane D. Antibodies. A Laboratory Manual. New York: Cold Spring Harbor Laboratory; 1988.
24. Estevez AM, Lehner B, Sanderson CM, Ruppert T, Clayton C. The roles of intersubunit interactions in exosome stability. J. Biol. Chem. 2003;278:34943–34951. [PubMed]
25. Landeira D, Navarro M. Nuclear repositioning of the VSG promoter during developmental silencing in Trypanosoma brucei. J. Cell Biol. 2007;176:133–139. [PMC free article] [PubMed]
26. Tu X, Wang CC. Coupling of posterior cytoskeletal morphogenesis to the G1/S transition in the Trypanosoma brucei cell cycle. Mol. Biol. Cell. 2005;16:97–105. [PMC free article] [PubMed]
27. Clayton C, Estevez AM, Hartmann C, Alibu VP, Field MC, Horn D. Down-regulating gene expression by RNA intereference in Trypanosoma brucei. Methods Mol. Biol. 2005;309:39–60. [PubMed]
28. Diehl S, Diehl F, El-Sayed NM, Clayton C, Hoheisel JD. Analysis of stage-specific gene expression in the bloodstream and the procyclic form of Trypanosoma brucei using a genomic DNA-microarray. Mol. Biochem. Parasitol. 2002;123:115–123. [PubMed]
29. Fellenberg K, Hauser NC, Brors B, Neutzner A, Hoheisel JD, Vingron M. Correspondence analysis applied to microarray data. Proc. Natl Acad. Sci. USA. 2001;98:10781–10786. [PMC free article] [PubMed]
30. Fellenberg K, Hauser NC, Brors B, Hoheisel JD, Vingron M. Microarray data warehouse allowing for inclusion of experiment annotations in statistical analysis. Bioinformatics. 2002;18:423–433. [PubMed]
31. Ausubel FM, Brent R, Kingston RE, Moore DD, Seidman JG, Smith JA, Struhl K, editors. Current Protocols in Molecular Biology. New York: John Wiley & Sons, Inc; 1997.
32. Michaeli S, Podell D, Agabian N, Ullu E. The 7SL RNA homologue of Trypanosoma brucei is closely related to mammalian 7SL RNA. Mol. Biochem. Parasitol. 1992;51:55–64. [PubMed]
33. Guerra-Giraldez C, Quijada L, Clayton CE. Compartmentation of enzymes in a microbody, the glycosome, is essential in Trypanosoma brucei. J. Cell Sci. 2002;115:2651–2658. [PubMed]
34. Colasante C, Robles A, Li CH, Schwede A, Benz C, Voncken F, Guilbride DL, Clayton C. Regulated expression of glycosomal phosphoglycerate kinase in Trypanosoma brucei. Mol. Biochem. Parasitol. 2007;151:193–204. [PubMed]
35. Robles A, Clayton C. Regulation of an amino acid transporter mRNA in Trypanosoma brucei. Mol. Biochem. Parasitol. 2008;157:102–106. [PubMed]
36. Haile S, Estevez AM, Clayton C. A role for the exosome in the in vivo degradation of unstable mRNAs. RNA. 2003;9:1491–1501. [PMC free article] [PubMed]
37. D’Orso I, Frasch AC. TcUBP-1, a mRNA destabilizing factor from trypanosomes, homodimerizes and interacts with a novel ARE- and poly(A)-binding proteins forming a ribonucleoprotein complex. J. Biol. Chem. 2002;277:50520–50528. [PubMed]
38. Urwyler S, Studer E, Renggli CK, Roditi I. A family of stage-specific alanine-rich proteins on the surface of epimastigote forms of Trypanosoma brucei. Mol. Microbiol. 2007;63:218–228. [PubMed]
39. Mori T, Kuroiwa H, Higashiyama T, Kuroiwa T. Generative cell specific 1 is essential for angiosperm fertilization. Nat. Cell Biol. 2006;8:64–71. [PubMed]
40. Engstler M, Reuter G, Schauer R. The developmentally regulated trans-sialidase from Trypanosoma brucei sialylates the procyclic acidic repetitive protein. Mol. Biochem. Parasitol. 1993;61:1–13. [PubMed]
41. Coustou V, Biran M, Besteiro S, Riviere L, Baltz T, Franconi JM, Bringaud F. Fumarate is an essential intermediary metabolite produced by the procyclic Trypanosoma brucei. J. Biol. Chem. 2006;281:26832–26846. [PubMed]
42. Sanchez MA, Drutman S, van Ampting M, Matthews K, Landfear SM. A novel purine nucleoside transporter whose expression is up-regulated in the short stumpy form of the Trypanosoma brucei life cycle. Mol. Biochem. Parasitol. 2004;136:265–272. [PubMed]
43. Chen CY, Xu N, Shuy AB. Highly selective actions of HuR in antagonizing AU-rich element-mediated mRNA destabilization. Mol. Cell Biol. 2002;22:7268–7278. [PMC free article] [PubMed]
44. Haenni S, Renggli CK, Fragoso CM, Oberle M, Roditi I. The procyclin-associated genes of Trypanosoma brucei are not essential for cyclical transmission by tsetse. Mol. Biochem. Parasitol. 2006;150:144–156. [PubMed]
45. Vassella E, Braun R, Roditi I. Control of polyadenylation and alternative splicing of transcripts from adjacent genes in a procyclin expression site: a dual role for polypyrimidine tracts in trypanosomes? Nucleic Acids Res. 1994;22:1359–1364. [PMC free article] [PubMed]
46. Bevilacqua A, Ceriani MC, Capaccioli S, Nicolin A. Post-transcriptional regulation of gene expression by degradation of messenger RNAs. J. Cell Physiol. 2003;195:356–372. [PubMed]
47. Sommer JM, Cheng Q.-L, Keller G.-A, Wang CC. In vivo import of firefly luciferase into the glycosomes of Trypanosoma brucei and mutational analysis of the C-terminal targeting signal. Mol. Biol. Cell. 1992;3:749–759. [PMC free article] [PubMed]
48. Irmer H, Clayton C. Degradation of the unstable EP1 mRNA in Trypanosoma brucei involves initial destruction of the 3′-untranslated region. Nucleic Acids Res. 2001;29:4707–4715. [PMC free article] [PubMed]
49. Li CH, Irmer H, Gudjonsdottir-Planck D, Freese S, Salm H, Haile S, Estevez AM, Clayton C. Roles of a Trypanosoma brucei 5'-3' exoribonuclease homolog in mRNA degradation. RNA. 2006;12:2171–2186. [PMC free article] [PubMed]
50. Schwede A, Ellis L, Luther J, Carrington M, Stoecklin G, Clayton C. A role for Caf1 in mRNA deadenylation and decay in trypanosomes and human cells. Nucleic Acids Res. 2008;36:3374–3388. [PMC free article] [PubMed]
51. Haile S, Dupe A, Papadopoulou B. Deadenylation-independent stage-specific mRNA degradation in Leishmania. Nucleic Acids Res. 2008;36:1634–1644. [PMC free article] [PubMed]
52. Mayho M, Fenn K, Craddy P, Crosthwaite S, Matthews K. Post-transcriptional control of nuclear-encoded cytochrome oxidase subunits in Trypanosoma brucei: evidence for genome-wide conservation of life-cycle stage-specific regulatory elements. Nucleic Acids Res. 2006;34:5312–5324. [PMC free article] [PubMed]
53. Maris C, Dominguez C, Allain FH. The RNA recognition motif, a plastic RNA-binding platform to regulate post-transcriptional gene expression. FEBS J. 2005;272:2118–2131. [PubMed]
54. Keene JD. Why is Hu where? Shuttling of early-response-gene messenger RNA subsets. Proc. Natl Acad. Sci. USA. 1999;96:5–7. [PMC free article] [PubMed]
55. Pao SS, Paulsen IT, Saier M.H., Jr Major facilitator superfamily. Microbiol. Mol. Biol. Rev. 1998;62:1–34. [PMC free article] [PubMed]
56. von Besser K, Frank AC, Johnson MA, Preuss D. Arabidopsis HAP2 (GCS1) is a sperm-specific gene required for pollen tube guidance and fertilization. Development. 2006;133:4761–4769. [PubMed]
57. Seebeck T, Schaub R, Johner A. cAMP signalling in the kinetoplastid protozoa. Curr. Mol. Med. 2004;4:585–599. [PubMed]
58. Magasanik B, Kaiser CA. Nitrogen regulation in Saccharomyces cerevisiae. Gene. 2002;290:1–18. [PubMed]
59. Takashima E, Inaoka DK, Osanai A, Nara T, Odaka M, Aoki T, Inaka K, Harada S, Kita K. Characterization of the dihydroorotate dehydrogenase as a soluble fumarate reductase in Trypanosoma cruzi. Mol. Biochem. Parasitol. 2002;122:189–200. [PubMed]
60. Papadopoulou B, Roy G, Breton M, Kundig C, Dumas C, Fillion I, Singh AK, Olivier M, Ouellette M. Reduced infectivity of a Leishmania donovani biopterin transporter genetic mutant and its use as an attenuated strain for vaccination. Infect Immun. 2002;70:62–68. [PMC free article] [PubMed]
61. Belen Carrillo M, Gao W, Herrera M, Alroy J, Moore JB, Beverley SM, Pereira MA. Heterologous expression of Trypanosoma cruzi trans-sialidase in Leishmania major enhances virulence. Infect. Immun. 2000;68:2728–2734. [PMC free article] [PubMed]
62. Chuenkova M, Pereira ME. Trypanosoma cruzi trans-sialidase: enhancement of virulence in a murine model of Chagas’ disease. J. Exp. Med. 1995;181:1693–1703. [PMC free article] [PubMed]
63. De Gaudenzi J, Frasch AC, Clayton C. RNA-binding domain proteins in kinetoplastids: a comparative analysis. Eukaryot. Cell. 2005;4:2106–2114. [PMC free article] [PubMed]
64. Boucher N, Wu Y, Dumas C, Dube M, Sereno D, Breton M, Papadopoulou B. A common mechanism of stage-regulated gene expression in Leishmania mediated by a conserved 3′-untranslated region element. J. Biol. Chem. 2002;277:19511–19520. [PubMed]
65. D’Orso I, Frasch AC. Functionally different AU- and G-rich cis-elements confer developmentally regulated mRNA stability in Trypanosoma cruzi by interaction with specific RNA-binding proteins. J. Biol. Chem. 2001;276:15783–15793. [PubMed]
66. Bringaud F, Muller M, Cerqueira GC, Smith M, Rochette A, El-Sayed NM, Papadopoulou B, Ghedin E. Members of a large retroposon family are determinants of post-transcriptional gene expression in Leishmania. PLoS Pathog. 2007;3:1291–1307. [PMC free article] [PubMed]
67. Zhang J, Ruyechan W, Williams N. Developmental regulation of two nuclear RNA binding proteins, p34 and p37, from Trypanosoma brucei. Mol. Biochem. Parasitol. 1998;92:79–88. [PubMed]

Articles from Nucleic Acids Research are provided here courtesy of Oxford University Press
PubReader format: click here to try


Save items

Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


  • BioProject
    BioProject links
  • Cited in Books
    Cited in Books
    NCBI Bookshelf books that cite the current articles.
  • GEO DataSets
    GEO DataSets
    Gene expression and molecular abundance data reported in the current articles that are also included in the curated Gene Expression Omnibus (GEO) DataSets.
  • MedGen
    Related information in MedGen
  • Pathways + GO
    Pathways + GO
    Pathways and biological systems (BioSystems) that cite the current articles. Citations are from the BioSystems source databases (KEGG and BioCyc).
  • PubMed
    PubMed citations for these articles
  • Substance
    PubChem chemical substance records that cite the current articles. These references are taken from those provided on submitted PubChem chemical substance records.

Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...