Plasticity of the Leishmania genome leading to gene copy number variations and drug resistance

Abstract

Leishmania has a plastic genome, and drug pressure can select for gene copy number variation (CNV). CNVs can apply either to whole chromosomes, leading to aneuploidy, or to specific genomic regions. For the latter, the amplification of chromosomal regions occurs at the level of homologous direct or inverted repeated sequences leading to extrachromosomal circular or linear amplified DNAs. This ability of Leishmania to respond to drug pressure by CNVs has led to the development of genomic screens such as Cos-Seq, which has the potential of expediting the discovery of drug targets for novel promising drug candidates.

Introduction

Leishmania are dimorphic parasites living as extracellular promastigotes in the digestive tract of Phlebotomus or Lutzomyia sandflies and as intracellular amastigotes within phagocytic cells (mainly macrophages) of the vertebrate hosts. Leishmania species cause leishmaniasis, the second largest parasite killer; there are 1.3 million new cases annually, 12 million people are affected worldwide, and 350 million people are currently at risk ¹. The Leishmania genus includes several species, among which more than 20 are pathogenic to humans ². Leishmania can be divided into two subgenera: the Leishmania Leishmania subgenus responsible for visceral and cutaneous leishmaniasis and the Leishmania Viannia subgenus often associated with either cutaneous or muco-cutaneous forms of the disease ². Visceral leishmaniasis is mainly caused by L. donovani and L. infantum and is characterized by fever, hepatosplenomegaly, and pancytopenia ³, making it the most severe and deadly form of the disease when compared with the self-healing but nonetheless debilitating skin lesions of cutaneous leishmaniasis ^{4, 5}.

No effective human vaccine is currently available against Leishmania (a canine Leishmania vaccine was recently registered in Europe ⁶), and control measures mainly involve chemotherapy ^{7– 9}. Pentavalent antimony (Sb) has been the standard drug for 70 years and remains the mainstay in many endemic regions, apart from Northern India, where antimonial formulations have been rendered obsolete because of widespread parasite resistance. Other first-line therapies include the polyene antibiotic amphotericin B (AMB) for which a single dose was shown to be 95% effective against visceral leishmaniasis in India ¹⁰. Liposomal AMB has become a standard treatment in many countries ¹¹ but requires administration by the intravenous route. Geographical differences in the response to liposomal AMB were reported, and visceral leishmaniasis cases in India were more responsive than those from East Africa or South America ¹². Clinical AMB resistance is scarce and parasites remained susceptible even after multiple rounds of treatment in the same patient ¹³. The alkyl-lysophospholipid analogue miltefosine (MTF) is the only oral drug against Leishmania ^{14, 15}. It has been successfully used for the treatment of visceral leishmaniasis since its registration in 2002 in India ¹⁶. However, relapse rates are on the rise in India ^{17, 18} and Nepal ^{19, 20}, making MTF resistance a likely problem. The aminoglycoside paromomycin (PMM) is also approved for the treatment of visceral leishmaniasis in India ^{21, 22}. So far, the scarce use of PMM has limited the emergence of resistance, but geographical variations in PMM efficacy against visceral leishmaniasis were noted between East Africa (especially Sudan) and India ^{23, 24}. Lastly, pentamidine (PTD) has been abandoned for the treatment of visceral leishmaniasis because of serious toxicities and is mainly restricted to patients with cutaneous leishmaniasis in South America ^{25– 27}.

Despite six decades of use, the mode of action (MOA) of antimonials is not known. It has been shown to lead to the production of reactive oxygen species ^{28– 31}, the depletion of trypanothione ³², and apoptosis-like death ^{33– 36}, but an exact MOA is still awaited. The same applies for MTF, AMB, PTD, and PMM, with the possible exception of AMB, which kills Leishmania by forming pores in ergosterol-containing membranes. New molecules with well-defined drug targets are clearly needed.

Leishmania and its genome

The Leishmania genome is around 32 Mb and displays over 8,300 coding genes ^{37, 38}. Within the Leishmania genus, gene synteny is conserved for more than 99% of genes between L. major, L. infantum, and L. braziliensis, and only few species-specific genes were found ³⁸. Leishmania species have between 34 and 36 chromosomes ranging in size from 0.3 to 2.8 Mb ^{37– 41}. One unique feature characterizing trypanosomatid parasites lies in their genome architecture, their protein-coding genes being organized as large polycistronic units ^{42, 43}. In the absence of defined RNA polymerase II promoters, transcription of the long polycistronic units occurs in a bidirectional fashion from transcriptional start sites located at strand switch regions ^{43, 44}. Processing into individual messenger RNAs (mRNAs) occurs by the addition through trans-splicing of a spliced leader RNA (39 nt) to the 5′ ends of each mRNA, coupled to 3′ end polyadenylation ^{45, 46}. Because of its lack of transcriptional control, Leishmania uses several adaptive mechanisms to regulate gene expression when facing changing environmental conditions during its development. 3′ untranslated regions (3′ UTRs) were shown to be major players in monitoring mRNA stability and translation rates in this parasite ^{47– 53}. To overcome stressful conditions like drug pressure, Leishmania also often relies on DNA copy number variations (CNVs) (aneuploidy, gene amplification, or gene deletion) for regulating the expression of drug targets, drug transporters, or other determinants of resistance. This is not restricted to Leishmania, however, and variations in gene dosage or chromosome copy numbers also influence drug susceptibility, adaptability, and proliferation in fungi and cancer cells ^{54– 57}. In addition to CNVs, single-nucleotide polymorphisms (SNPs) in drug targets or in transporters can lead to drug resistance without the need for altering gene expression.

Copy number variations

During the last few decades, Leishmania parasites were considered to be essentially diploid but recent data have shown that aneuploidy seems to be the norm ^{58– 64}. Within populations of Leishmania parasites, distinct aneuploidy patterns were shown to occur at the level of individual cells. This phenomenon was called mosaic aneuploidy and can translate into a seemingly average diploid population when the cumulative ploidy is derived from next-generation DNA sequencing data but in which few parasites actually share the same ploidy for individual chromosomes ^{62, 63, 65}. Interestingly, variations in the size and content of chromosomes have also been observed between different strains of the related trypanosomatid parasite Trypanosoma cruzi ^{66, 67}. In the case of Leishmania, circumstantial links between the presence of supernumerary chromosomes or chromosomal losses and drug resistance have been observed ^{58– 60, 64, 68– 71}, suggesting that a particular group of genes on the variant chromosomes may possibly act together in establishing resistance, but this has yet to be demonstrated.

Aneuploidy is generally linked to developmental abnormalities as best exemplified by the trisomy 21 syndrome in humans. However, Leishmania uses aneuploidy as a lifestyle. This is raising a number of questions about aneuploidy generation, stability, transmission, and biological significance (reviewed elsewhere ^{60, 62, 72}). In the absence of transcription initiation control, increases (or decreases) in chromosome copy number may serve as a strategy for regulating expression under environmental cues. This can happen at the level of whole chromosomes, and indeed there was a good correlation between chromosome ploidy and the level of DNA and RNA expression ⁵⁹. Increasing the copy numbers of entire chromosomes may lead to the overexpression of toxic genes, but the Leishmania genome (32 Mb) is spread in 34 to 36 chromosomes, thus reducing the co-expression of many genes. However, as explained in detail below, Leishmania also has the ability to amplify (or delete) specific smaller regions of DNA as part of extrachromosomal elements by recombination/rearrangements at the level of homologous repeated sequences (RSs). RNA levels derived from these amplifications are correlated to DNA copy number.

The genome of Leishmania is populated with repeated DNA sequences. A recent study highlighted the entire set of RSs in different Leishmania species, and it was found that the whole Leishmania genome has the potential to be rearranged at the level of those RSs for generating extrachromosomal elements ⁷³. Indeed, almost 2,000 RSs are distributed over the genome of L. infantum and these potentially support the formation of more than 3,000 extrachromosomal DNA elements ⁷³. Short interspersed degenerate retroposons (SIDERs) account for up to 65% of all RSs. SIDERs are truncated versions (~0.55 kb) of formerly active retroposons that are predominantly located in 3′ UTRs and have been associated with post-transcriptional regulation at the levels of both mRNA stability and translation ^{47, 48, 52, 53, 74, 75}. Because SIDERs are degenerated, they were found in different RS groups. Remarkably, SIDER elements would have dual roles: one functional by regulating gene expression and a second one structural, providing the backbone to facilitate gene rearrangements for changing copy number of chromosomal DNA regions.

Extrachromosomal DNA amplifications are frequently detected in Leishmania parasites challenged with drugs or other stressful conditions ^{58, 59, 64, 76– 87}. The episomes are amplified as either circular or linear extrachromosomal DNA and formed through rearrangements at the level of direct or inverted homologous RSs, respectively ( Figure 1) ^{73, 80, 88}. Interestingly, between 60% and 80% of the predicted amplicons appear to be already present in the population in the absence of selection and these pre-existing stochastic gene amplifications were shown to foster the selection of adaptive traits in response to drug pressure ⁷³. Beneficial amplicons were shown to increase in abundance upon higher drug pressure and to decrease when the drug is removed, allowing parasites to respond to a changing environment ⁷³.

Figure 1. Potential mechanisms for gene amplification in Leishmania.

( a) The RAD51 recombinase mediates homologous recombination between direct repeated sequences (DRS) and leads to (i) extrachromosomal circular amplicon or (ii) intrachromosomal tandem duplication by unequal sister chromatid exchange or RAD51-mediated break-induced replication. Black arrows represent DRS. ( b) The MRE11 nuclease processes DNA ends after single-strand break (SSB), double-strand break (DSB), or hairpin formation during replication and leads to extrachromosomal linear amplification. Black arrows represent inverted repeated sequences (IRS). The green segments represent the amplified DNA regions. dsDNA, double-stranded DNA; ssDNA, single-stranded DNA.

Since gene rearrangements through RSs are primary responses to drug pressure, a reasonable hypothesis was that identifying recombinase proteins involved in these rearrangements could lead to strategies to prevent the emergence of resistance. A first candidate was the RAD51 DNA repair protein, a key protein involved in homologous recombination (HR), a mechanism evolutionarily conserved in trypanosomatids ⁸⁹. Interestingly, the expression of RAD51 was induced in Leishmania by DNA double-strand breaks (DSBs) ^{90, 91}. Inactivating RAD51 led to viable parasites unable to generate circular extrachromosomal elements but still capable of producing linear amplicons upon drug pressure ⁷³. Leishmania has three RAD51 paralogs (RAD51-3, RAD51-4, and RAD51-6) that were shown to work as a complex in promoting HR through their capacity to stimulate RAD51 activity ⁹². Inactivation of RAD51-4 was also shown to prevent the formation of circular amplicons in L. infantum exposed to drugs, but not of linear amplicons ⁹².

Linear amplicons are formed by the annealing of RSs found in an inverted orientation ^{64, 73, 93}. MRE11 is a DNA repair nuclease that interacts with RAD50 and NBS1 to form the MRN complex ^{94, 95} and is important for DSB repair by HR ^{96, 97} or for non-homologous end joining ⁸⁹ ( Figure 1b). Inactivation of MRE11 impaired the ability of L. infantum to form linear amplicons upon drug selection at the level of inverted RSs, although the capacity to generate circular amplicons was similar to that of wild-type parasites ⁹³. Moreover, a fully functional MRE11 is important for linear amplification, as parasites expressing DNA-binding-proficient but nuclease-deficient MRE11 exclusively generated circular amplicons during drug selection ⁹³. Interestingly, inactivation of MRE11 alone or along with its partner RAD50 led to extensive chromosomal translocation in L. infantum ⁹⁸, showing that the MRE11/RAD50 complex is important for the maintenance of genome integrity in addition to its role in gene rearrangements. The number of enzymes involved in the formation of extrachromosomal elements suggests that targeting this pathway may not be a viable strategy for preventing the emergence of resistance, although this remains to be experimentally tested.

Single-nucleotide polymorphisms and small nucleotide insertions or deletions

Although CNVs are important contributors of drug resistance, SNPs and small nucleotide insertions or deletions (indels) can also contribute to resistance. This was proven with experimental drugs ^{99, 100} and was highlighted with MTF where amino acid substitutions or non-sense mutations were observed in the MTF transporter (MT) ¹⁰¹ or in its Ros3 subunit ¹⁰². This was further confirmed in additional mutants using whole genome sequencing ^{103, 104} or by deep sequencing of MT ¹⁰⁵. Mutations detected in the MT gene of L. infantum isolates serially collected from an MTF-treated patient who had multiple relapses were shown to correlate with resistance ¹⁰⁶, suggesting that MTF resistance could become a clinical reality in the near future.

Genome-wide surveys of genetic variations in L. donovani isolates from the Indian subcontinent supported the notion that resistance to antimonials emerged on several distinct occasions ^{58, 107}. Isolates could also be clustered on the basis of their genetic structure and haplotypes, with some groups being enriched for non-responsive strains ^{58, 107, 108}. Interestingly, a particular group of highly resistant isolates that clustered together were found to share genomic features associated with resistance ¹⁰⁷. Among these were a higher copy number for the H-locus, coding for the well-characterized ABC transporter MRPA ¹⁰⁹, and a homozygous two-base-pair insertion in the aquaglyceroporin 1 (AQP1) gene involved in Sb uptake and whose inactivation or downregulation is strongly correlated with resistance ^{71, 107, 110– 117}. The potential for these genomic variants in predicting treatment outcome is exciting, given the lack of molecular markers for Sb resistance, but will need to be thoroughly evaluated by using larger and geographically diversified sets of well-defined isolates.

Exploiting copy number variations for understanding drug mode of action and resistance mechanisms

Target-based assays and phenotypic whole-cell-based assays are the cornerstones of drug discovery. The current trend for anti-parasitic agents is for whole cell assays. A drawback of phenotype-based assays is the lack of knowledge about the targets of hit compounds. Although the molecules could be brought to the clinic without further knowledge about their MOA, a clear understanding of the molecular targets will facilitate the improvement of a candidate drug through lead optimization. Characterization of drug-resistant mutants, which often revealed mutations or CNVs in drug targets or in proteins responsible for drug transport, is one strategy to pinpoint drug targets. However, it is salient to point out that this strategy has not yet led to targets against the current anti-leishmanials, although amplification of gene targets was observed in mutants made resistant to experimental drugs ^{64, 99}. Since CNVs are often associated with resistance, forward genetic tools can experimentally mimic this. One such gain-of-function screen was based on functional cloning where Leishmania cosmid libraries were electroporated into Leishmania and these transfectants were selected for a specific phenotype ¹¹⁸. Selection is possible because of the high copy number (and gene expression) of the cosmids. This screen was successfully applied while selecting for drug resistance or susceptibility ^{101, 114, 119– 123}. This technique selects for cosmids conferring dominant phenotypes (leaving out less enriched cosmids) and is not easily amenable to high-throughput screening. The sensitivity of cosmid-based functional screening was enhanced by its recent coupling to next-generation sequencing in an approach termed Cos-Seq ¹²⁴. The proportion of parasites with cosmids providing a selective advantage is expected to rise with increasing drug pressure, and these can be tracked and quantified at each drug increment by Illumina sequencing ^{124, 125}. Thus, the dynamics of cosmid enrichment can be followed over the entire course of selection instead of being monitored only at endpoint. Published or ongoing Cos-Seq screens using experimental drugs with known targets (for example, methotrexate, terbinafine, and 5-fluorouracil) confirmed the recovery of the relevant target genes by Cos-Seq ¹²⁴. Interestingly, Cos-Seq supported the hypothesis that the current anti-leishmanials (MF, AMB, Sb, PMM, and PTD) may not act via specific major protein targets ¹²⁴. Indeed, although an unprecedented number of resistance genes (known and novel) were isolated using Cos-Seq, none emerged as a clear target candidate and it is conceivable that these antiquated drugs are broadly cytotoxic by disrupting multiple minor targets. Whether some of the genes are genuine drug targets remains to be established, and non-protein targets represent another possibility as these would not be detected by Cos-Seq.

The advent of high-content screening for intracellular L. donovani amastigotes ¹²⁶ is also key in the search for novel molecules having favourable anti-leishmanial properties directly on the intracellular stage of the parasite. This allowed the discovery of 192 new leads against visceral leishmaniasis from an initial set of 1.8 million compounds from GlaxoSmithKline ¹²⁷. An MOA could be hypothesized for 80 of the lead compounds using prior proprietary knowledge and bioinformatics analyses of TriTryp genomes, which revealed an over-representation of putative kinase inhibitors ¹²⁷. Cos-Seq was initially carried out with the insect form of the parasite but this could easily be adapted to intracellular parasites and this technique could be used to find the targets of these promising novel molecules or of other drugs repurposed against Leishmania ¹²⁸.

The Cos-Seq technique does not allow the isolation of loss-of-function mutations such as those found in the aquaglyceroporin AQP1 or in the MT transporter genes (see above). These require high-throughput dominant negative screening approaches, like inducible RNA interference target sequencing (RIT-Seq), which proved instrumental in elucidating mechanisms of drug uptake in trypanosomes ¹²⁹. Although RNA interference is absent from the L. Leishmania subgenus, it is active in species of the L. Viannia subgenus ¹³⁰. The lack of inducible expression in Leishmania was also a limitation of this technique, but two recent reports have shown the feasibility of inducible expression in Leishmania ^{131, 132}. Thus, it is theoretically possible to develop a technology similar to RIT-Seq in L. Viannia parasites. An alternative approach to RIT-Seq would be to rely on RNA-guided nuclease systems using clustered regularly interspaced short palindromic repeats (CRISPR) and CRISPR-associated (Cas) enzymes, as these have proven very efficient for achieving targeted genomic modifications in a wide range of genomes ^{133– 135}. In trypanosomatid parasites, the CRISPR/Cas9 system derived from Streptococcus pyogenes has been used for disrupting genes in L. major ¹³⁶, L. donovani ¹³⁷, and T. cruzi ¹³⁸ and in principle could be used for generating whole-genome Cas9-mediated gene deletion libraries.

Concluding remarks

The toolkit for drug target discovery and resistance mechanism elucidation for Leishmania is expanding. With new promising drug candidates in the pipeline and further technological developments, it should now be possible to find new targets which should further help in the control of this important neglected tropical disease.

Abbreviations

3′ UTR, 3′ untranslated region; AMB, amphotericin B; AQP1, aquaglyceroporin 1; Cas, clustered regularly interspaced short palindromic repeat-associated; CNV, copy number variation; CRISPR, clustered regularly interspaced short palindromic repeat; DSB, double-strand break; HR, homologous recombination; MOA, mode of action; mRNA, messenger RNA; MT, miltefosine transporter; MTF, miltefosine; PMM, paromomycin; PTD, pentamidine; RIT-Seq, RNA interference target sequencing; RS, repeated sequence; Sb, antimony; SIDER, short interspersed degenerate retroposon; SNP, single-nucleotide polymorphism.

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The referees who approved this article are:

• Gerald Spaeth, Unité de Parasitologie moléculaire et Signalisation, Department of Parasites and Insect Vectors, Institut Pasteur, INSERM U1201, Paris, France

• Yvon Sterkers, UMR MIVEGEC (CNRS 5290 - IRD 224 - University Montpellier), University Regional Hospital of Montpellier, Montpellier, France

• Richard McCulloch, The Wellcome Trust Centre for Molecular Parasitology, Institute of Infection, Immunity and Inflammation, University of Glasgow, Glasgow, UK

• Joachim Clos, Bernhard Nocht Institute for Tropical Medicine, Hamburg, Germany

• Francisco Gamarro, Instituto de Parasitología Lopez-Neyra, IPBLN-CSIC, Granada, Spain

Funding Statement

BP is supported by grants from the Canadian Institutes of Health Research, the Natural Sciences and Engineering Research Council of Canada, and the Ministère du Developpement Économique de l’Innovation et de l’Exportation du Québec. MO is supported by grants from the Canadian Institutes of Health Research and holds a Canada Research Chair on Antimicrobial Resistance.

The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.