Involvement of Leishmania Phosphatases in Parasite Biology and Pathogeny
Anita Leocadio Freitas-Mesquita1,2* 
André Luiz Araújo Dos-Santos1,2 
José Roberto Meyer-Fernandes1,2*- 1Instituto de Bioquímica Médica Leopoldo De Meis, Universidade Federal do Rio de Janeiro, Rio de Janeiro, Brazil
- 2Instituto Nacional de Ciência e Tecnologia em Biologia Estrutural e Bioimagem, Universidade Federal do Rio de Janeiro, Rio de Janeiro, Brazil
In the Leishmania lifecycle, the motile promastigote form is transmitted from the sand fly vector to a mammalian host during a blood meal. Inside vertebrate host macrophages, the parasites can differentiate into the amastigote form and multiply, causing leishmaniasis, one of the most significant neglected tropical diseases. Leishmania parasites face different conditions throughout their development inside sand flies. Once in the mammalian host, the parasites have to overcome the microbicide repertoire of the cells of the immune system to successfully establish the infection. In this context, the expression of protein phosphatases is of particular interest. Several members of the serine/threonine-specific protein phosphatase (STP), protein tyrosine phosphatase (PTP), and histidine acid phosphatase (HAcP) families have been described in different Leishmania species. Although their physiological roles have not been fully elucidated, many studies suggest they have an involvement with parasite biology and pathogeny. Phosphatases play a role in adaptation to nutrient starvation during parasite passage through the sand fly midgut. They are also important to parasite virulence, mainly due to the modulation of host cytokine production and impairment of the microbiocidal potential of macrophages. Furthermore, recent whole-genome expression analyses have shown that different phosphatases are upregulated in metacyclic promastigotes, the infective form of the mammalian host. Leishmania phosphatases are also upregulated in drug-resistant strains, probably due to the increase in drug efflux related to the activation of ABC transporters. Throughout this review, we will describe the physiological roles that have been attributed to Leishmania endogenous phosphatases, including their involvement in the adaptation, survival, and proliferation of the parasites inside their hosts.
Introduction
Leishmania spp. are trypanosomatid parasites that infect humans and other mammals (Chang, 1983). Leishmaniasis may be asymptomatic or it may manifest as cutaneous or mucocutaneous disease or even as a visceral form that can be lethal if untreated. The course of infection depends on the complex interaction between the infecting species and the host immune response (Pace, 2014). In the Leishmania lifecycle, promastigote forms are transmitted from the sand fly vector to the mammalian host during a blood meal. Inside the host macrophages, the parasites differentiate into the amastigote form (Chang, 1983). During their lifecycle, Leishmania parasites are exposed to diverse environmental stimuli. Protein phosphorylation and dephosphorylation are crucial events in cell recognition of external and internal signals, leading to specific responses (Cosentino-Gomes and Meyer-Fernandes, 2011; Freitas-Mesquita and Meyer-Fernandes, 2014).
The majority of eukaryotic proteins (96-99%) are phosphorylated at serine and threonine residues. Thus, serine/threonine-specific protein phosphatases (STPs) are of great importance for crucial dephosphorylation events. STPs are divided into three groups: phosphoprotein phosphatases (PPPs), metallo-dependent protein phosphatases (PPM/PP2C), and aspartate-based phosphatases (FCP/SCP) (Cohen, 1997; Szöör, 2010; Soulat and Bogdan, 2017). PPP and PPM depend on metal ions for catalysis through the activation of a water molecule for the dephosphorylation reaction, while FCPs/SCPs use an aspartate-based (DxDxT/V) catalytic core to dephosphorylate phospho Ser/Thr residues (Szöör, 2010).
Different STPs expressed by Leishmania parasites have been identified and characterized by biochemical and molecular means, including protein phosphatase 5 (PP5) (Norris-Mullins et al., 2018), protein phosphatase 1 (PP1) (Qureshi et al., 2019), protein phosphatase 2C (PP2C) (Jakkula et al., 2018), and protein phosphatase 2B (PP2B) (Banerjee et al., 1999) of Leishmania donovani; PP2B (Naderer et al., 2011), protein phosphatase with EF-Hand (PPEF) (Mills et al., 2007), and arsenate reductase 2 (ACR2) (Zhou et al., 2004; Zhou et al., 2006) of Leishmania major; PP2C (Escalona-Montaño et al., 2016) of Leishmania mexicana; and PP2C (Burns et al., 1993) of Leishmania chagasi.
Although phosphorylation on tyrosine residues comprises a small fraction of all protein phosphorylation events, it plays an important role in signaling involved in cell cycle control and differentiation (Andreeva and Kutuzov, 2008). Protein tyrosine phosphatases (PTPs) share a consensus sequence motif, and their catalytic site is surrounded by cysteine and arginine (CX5R) (Soulat and Bogdan, 2017). Based on their catalytic domains and substrate specificity, PTPs are classified as Class I, Class II, Class III, or Class IV (Alonso et al., 2004). The great majority of Leishmania PTPs belong to the Class I group, which is subdivided into classical and dual-specificity PTPs (Szöör, 2010). Classical PTPs include phosphatases homologous to human protein tyrosine phosphatase 1B (PTP1B). Contrary to those found in higher eukaryotes, in Leishmania and other kinetoplastid parasites, this group does not contain any PTP-receptors (Soulat and Bogdan, 2017). Dual-specificity phosphatases (DUSPs) are able to dephosphorylate a wide variety of phospho-substrates in addition to phospho-tyrosine (Soulat and Bogdan, 2017).
PTP1B homologs were identified and characterized in L. mexicana (Escalona-Montaño et al., 2010), L. infantum (Nascimento et al., 2006), L. major (Nascimento et al., 2006), and L. donovani (Nascimento et al., 2006). Phosphatase activity assays performed with living cells revealed the presence of a phosphohydrolase ectoenzyme with phosphotyrosine phosphatase activity in L. amazonensis (de Almeida-Amaral et al., 2006).
The histidine acid phosphatase (HAcP) superfamily is a large family of proteins with a conserved catalytic histidine residue in the motif RHG present at the N-terminus, which becomes phosphorylated during the reaction (Rigden, 2008; Coker et al., 2013). Their substrate specificity has not been ascertained; therefore, they do not belong to the classical STP or PTP families (Soulat and Bogdan, 2017). Recently, in silico analysis of the genome of different Leishmania species revealed the presence of several genes encoding HAcP, including membrane-bound acid phosphatases (also known as ectophosphatases) and secreted acid phosphatases (Soulat and Bogdan, 2017). The most studied Leishmania HAcPs are the membrane-bound acid phosphatases of L. donovani (LdMAcP) (Shakarian et al., 2002) and L. mexicana (LmxMBAP) (Wiese, 1996) and the secreted acid phosphatases of L. donovani (LdSAcP-1 and LdSAcP-2) (Shakarian et al., 1997) and L. mexicana (LmxSAP-1 and LmxSAP-2) (Wiese et al., 1995).
The present review aims to describe the occurrence of STPs, PTPs, and HAcPs in Leishmania species, highlighting their physiological roles. In the following sections, we will discuss in detail the information available in the literature concerning the involvement of Leishmania phosphatases during parasite infection. We will also provide an overview of the differential expression of phosphatases throughout the Leishmania lifecycle, particularly in response to stress conditions.
Involvement of Phosphatases in Leishmania Pathogeny
The success of Leishmania infection in mammalian hosts is related to its prompt adaptation to new and hostile environments, in addition to its ability to impair the main microbicidal functions of macrophages (Shio et al., 2012; Soulat and Bogdan, 2017). Through the secretion of virulence factors, parasites interfere in host signaling pathways, modulating the production of cytokines and inhibiting the generation of nitric oxide (NO) and reactive oxygen species (ROS) (Remaley et al., 1984; Remaley et al., 1985; Forget et al., 2006; Soulat and Bogdan, 2017). The involvement of kinase and phosphatase proteins is crucial for the tight control of phosphorylation events that govern these signaling pathways (Soulat and Bogdan, 2017). It is well known that Leishmania parasites can activate host PTPs such as src homology 2 domain-containing tyrosine phosphatase 1 (SHP-1), impairing the microbicidal capacity of macrophages (Blanchette et al., 1999; Shio et al., 2012). However, the participation of Leishmania phosphatases is also relevant during the infection process. Throughout this section, we will describe studies reporting the occurrence of STP, PTP, and HAcP in different Leishmania species and their involvement in the adaptation, survival, and proliferation of the parasites inside the host cells. Figure 1 presents a schematic summary of the physiological roles that have been attributed to Leishmania endogenous phosphatases so far.
Figure 1 Physiological roles described for Leishmania endogenous phosphatases. Phosphatases may contribute to the ability of parasites to adapt properly during stress conditions, favoring the differentiation process (Martin et al., 2014; Inbar et al., 2017; Norris-Mullins et al., 2018). Whole-genome expression analyses revealed that several Leishmania phosphatases are upregulated in nectomonad and metacyclic promastigotes (Saxena et al., 2003; Alcolea et al., 2009; Dillon et al., 2015; Inbar et al., 2017). Once inside the mammalian host, Leishmania parasites can subvert the host immune response to allow for infection of macrophages and survival inside the PV. Endogenous phosphatases may favor parasite infection and survival through modulation of cytokine production and impairment of the microbicidal potential of macrophages (Remaley et al., 1984, Remaley et al., 1985; Nascimento et al., 2006; Naderer et al., 2011; Escalona-Montaño et al., 2016; Leitherer et al., 2017; Jakkula et al., 2018). PV, parasitophorous vacuole; N, nucleus; K, kinetoplast.; ROS, reactive oxygen species.
Serine/Threonine Specific Protein Phosphatases (STPs)
PP5 is a unique member of the PPP family due to the presence of an N-terminal tetratricopeptide repeat (TPR) domain that is involved in protein-protein interactions (Borthwick et al., 2001). Recently, it was observed that PP5 plays a role in the metacyclogenesis and virulence of Leishmania parasites (Norris-Mullins et al., 2018). L. donovani axenic metacyclic promastigotes present an increase in PP5 expression when compared to procyclic promastigote and amastigote stages. Further analyses, performed using PP5-overexpressing and PP5 null mutants (ΔPP5), revealed that the absence of PP5 impairs the ability of the parasites to adapt properly during stress conditions. Although ΔPP5 promastigotes retain the ability to differentiate, a significant increase in premature cell death was observed. The relevance of PP5 during the differentiation process seems to be related to its interaction with the heat-shock protein HSP83 (Norris-Mullins et al., 2018). To investigate the potential consequences of the abolishment of PP5 on the pathobiology of Leishmania, in vitro and in vivo assays were performed with L. donovani and L. major, respectively. Although ΔPP5 L. donovani parasites have been able to successfully invade murine macrophages, an attenuation in the virulence of ΔPP5 L. major parasites was demonstrated through a well-established cutaneous leishmaniasis model system (Norris-Mullins et al., 2018).
Recently, a PP1 of L. donovani (LdPP1) was purified to study its structural properties as well as its effectiveness as an immunomodulator (Qureshi et al., 2019). Sequence analysis showed great similarity between LdPP1 and the PP1 of other trypanosomatids and even with human PP1. Such conservation during the course of evolution may be related to its indispensable involvement in vital functions (Qureshi et al., 2019). Cultured macrophages were treated with the purified LdPP1 protein to investigate possible immunomodulatory effects by ELISA and qRT-PCR analyses. LdPP1 was found to upregulate the Th1-type immune response due to the increase in the proinflammatory cytokines TNF-α and IL-6 and the levels of NO and NF-кB in macrophages (Qureshi et al., 2019).
Calcineurin (PP2B) is a Ca2+ and calmodulin-activated protein phosphatase that is comprised of a catalytic (CnA) and regulatory (CnB) subunit. The catalytic site of calcineurin, usually autoinhibited, is released by calmodulin binding, which occurs due to the increase in intracellular levels of Ca2+ (Rodríguez et al., 2009). The requirement of calcium uptake for parasite thermotolerance at 34–37°C has motivated the investigation of the role played by calcineurin in this process (Naderer et al., 2011). Through the generation of an L. major mutant lacking the essential CbN subunit (Δcnb), it was observed that calcineurin plays a role in both early and long-term adaptive parasite responses to environmental stresses faced during their lifecycle in the mammalian host (Naderer et al., 2011). Although Δcnb mutants have been internalized by macrophages, their differentiation into heat-adapted amastigotes was impaired, and consequently, they failed to proliferate. To investigate the role of calcineurin during infection in vivo, susceptible BALB/c mice were subcutaneously infected with wild-type, Δcnb mutant or complemented (Δcnb + CnB) L. major promastigotes. Δcnb parasites were completely cleared by the susceptible BALB/c mice; however, complementation with CnB restored virulence almost to wild-type levels, confirming that calcineurin signaling is essential for the survival of L. major (Naderer et al., 2011).
The involvement of secreted proteins in the evasion of the host immune response has been described in different microorganisms. Proteins with phosphatase activities were identified in the secretion medium of both promastigote (PSM) and amastigote (ASM) L. mexicana parasites. The occurrence of a PP2C in both secretion media was confirmed through recognition by an antibody against PP2C of L. major. The incubation of human macrophages with PSM and ASM led to an increase in the production of several inflammatory cytokines, including TNF-α, IL-1β, IL-12p70, and IL-10 (Escalona-Montaño et al., 2016). In L. donovani, a PP2C (LdPP2C) was also shown to elicit innate immune functions through upregulation of proinflammatory cytokines (TNF-α and IL-6) as well as NO generation by macrophages (Jakkula et al., 2018). The full-length ORF of LdPP2C was cloned into an expression vector to obtain the purified protein. In addition to an analysis of its immunomodulation, its biochemical and structural parameters were evaluated. The amino acid sequence of LdPP2C showed high conservation to its counterparts in other Leishmania species, such as L. infantum, L. major, and L. mexicana (Jakkula et al., 2018).
Protein Tyrosine Phosphatases (PTPs)
In higher eukaryotic cells, a large number of studies have demonstrated that PTPs are involved in the regulation of multiple cell processes, including proliferation and differentiation (Tonks, 2003). The involvement of PTPs in inducing differentiation and increasing virulence was first demonstrated through the heterologous expression of a prototype human protein-tyrosine phosphatase 1B (hPTP1B) in L. donovani (Nascimento et al., 2003). Genes encoding PTP were identified in L. major (LmPTP1), L. infantum (LiPTP1), and L. donovani (LdPTP1) due to their homology with hPTP1B (Nascimento et al., 2006). In silico structural analysis confirmed that LiPTP1 and hPTP1B share remarkable conservation, mainly in their active sites. The generation of LdPTP1 null mutants showed that PTP1 is dispensable for the growth and development of the parasite in culture, in contrast with previous observations that suggested the participation of PTP in the differentiation process. However, the deletion of the gene severely impaired the survival of amastigotes in BALB/c mice (Nascimento et al., 2006).
Another PTP was recently identified in L. major parasites and named Lm-PRL-1 due to its strong similarity to the human phosphatases of regenerating liver (PRL), as confirmed by structural analysis and a similar profile of their biochemical parameters (Leitherer et al., 2017). The presence of LmPRL-1 was detected in exosomes released by L. major promastigotes. Exosomes are vesicles secreted by parasites that are loaded with cytoplasmic and membrane-bound proteins, including virulence factors. To investigate the fate of the LmPRL-1 released during infection, further analyses were performed using L. major parasites that ectopically expressed hemagglutinin (HA3)-tagged LmPRL-1 (Leitherer et al., 2017). HA3-LmPRL-1 was detected not only in the amastigotes but also in the cytoplasm of the infected macrophages. Colocalization with the late phagosomal marker LAMP-1 confirmed its occurrence on the surface of parasitophorous vacuoles (PVs), where it is prone to modulate host cell signaling pathways that may favor parasite survival. In vitro interaction assays have confirmed that the expression of HA3-LmPRL-1 significantly increased parasite survival after 72 h of infection (Leitherer et al., 2017).
A dual specificity protein/lipid phosphatase of L. mexicana (LmDUSP1) has also been recently identified as a virulence factor (Kraeva et al., 2019). The LmDUSP1-encoding gene (LmxM.22.0250), acquired from bacteria via horizontal gene transfer, presents orthologs that have been implicated in virulence (Beresford et al., 2010; Soulat and Bogdan, 2017). To investigate the role of LmDUSP1 in parasite infection, knockout of LmxM.22.0250 (LmDUSP1 KO) was obtained using the CRISPR-Cas9 approach. The ablation of LmxM.22.0250 leads to a significant decrease in the parasite’s ability to infect or develop in primary murine macrophages in vitro (Kraeva et al., 2019).
Histidine Acid Phosphatase (HAcPs)
The passage of L. donovani promastigotes through susceptible Balb/c mice increased the levels of parasite HAcP activities. This was the first evidence that acid phosphatase could be considered a marker of virulence (Katakura and Kobayashi, 1988). A few years later, a study tested seven isolates of L. donovani and showed a correlation between the degree of virulence and the membrane-bound acid phosphatase activity of the parasites (Singla, 1992).
Preincubation of neutrophils stimulated by the chemoattractant peptide N-formyl-methionyl-leucyl-phenylalanine with a purified preparation of the tartrate-resistant membrane-bound HAcP of L. donovani decreased oxygen consumption and the generation of superoxide and hydrogen peroxide. These effects were abolished by the incorporation of an HAcP inhibitor in the preincubation medium, indicating that they are related to the catalytic activity of the enzyme (Remaley et al., 1984; Remaley et al., 1985). Both the membrane-bound and the secreted acid phosphatases were resistant to exposure to the toxic oxygen metabolites (e.g., superoxide anions, hydrogen peroxide, and hypochlorite) generated by the phagocytic cells. The stability of their catalytic activity enables HAcPs to compromise other host cell functions during the course of infection (Saha et al., 1985).
The association between murine peritoneal macrophages and L. amazonensis parasites in the presence of protein kinase C (PKC) agonists suggests that PKC activation may modulate the parasite-macrophage association via secreted HAcP in the early stage of a 60-min interaction (Vannier-Santos et al., 1995). By extending the analysis over a total period of 24 h postinfection, it was observed that L. amazonensis-secreted HAcP also mediates the maturation of PVs (Fernandes et al., 2013). Previous studies using bacteria as models suggested the involvement of microorganism-secreted phosphatases in both PV biogenesis and bacterial growth via an unknown mechanism (Hussain et al., 2010). Indeed, it has also been shown in L. donovani and L. major that secreted HAcP leaves the PV and becomes concentrated in compartments distributed in the cytoplasm of infected macrophages (McCall and Matlashewski, 2010).
A recent study promoted the overexpression of LdMAcP in L. donovani promastigotes and showed an increase in transgenic parasite survival during in vitro infection of macrophages (Papadaki et al., 2015). These data suggest a possible similar role for endogenous LdMAcP, consistent with previous observations indicating that this enzyme may play a role in parasite virulence (Katakura and Kobayashi, 1988; Singla, 1992; Papadaki et al., 2015; Soulat and Bogdan, 2017). On the other hand, the deletion of the membrane-bound HAcP gene of L. mexicana did not affect the virulence of these parasites (Benzel et al., 2000). Comparing wild-type and LmxMBAP-deficient parasites, no significant differences were observed in survival during in vitro infection in macrophages or in vivo infection of susceptible BALB/c mice (Benzel et al., 2000). Although this result may rule out the involvement of the membrane-bound HAcP in L. mexicana virulence, a definitive statement is not possible because of potential compensatory mechanisms, as Leishmania parasites carry a minimum of four genes encoding HAcPs (Soulat and Bogdan, 2017).
The unique tartrate-resistant membrane-bound acid phosphatase seems to be specifically expressed in the L. donovani complex, responsible for viscerilization, the most severe manifestation of leishmaniasis. It is possible that this enzyme modulates the secretion of cytokines by macrophages, thereby affecting the pathophysiology of the disease. Further studies are needed to deepen the knowledge in this area. If this hypothesis is confirmed, LdMAcP could be proven useful in diagnosis or epidemiological studies (Papadaki et al., 2015).
Transcriptome and Proteomic Analyses Revealed the Differential Expression of Several Leishmania Phosphatases
Recent advances in sequencing techniques have shown the global changes in gene expression during the lifecycle of Leishmania parasites. The following section presents several whole-genomic analyses showing the differential expression of Leishmania phosphatases according to parasite stage of life or in drug-resistant strains, as summarized in Table 1.
Table 1 Differential expression of Leishmania endogenous phosphatases during their lifecycle and in drug-resistant strains.
Differential Expression of Phosphatases During the Leishmania Lifecycle
Leishmania parasites shift their lifecycle between the PV of their mammalian host mononuclear phagocytes and the alimentary tract of their sand fly vector. Briefly, when a sand fly takes a blood meal from an infected mammalian host, the acquired amastigotes differentiate into promastigotes and colonize the insect midgut. The Leishmania promastigotes are subjected to several microenvironments with different conditions, such as a lack of nutrient availability (Inbar et al., 2017). In response to these specific conditions, the parasite can differentiate into several distinct forms. Beyond the proliferative procyclic and infective metacyclic forms, there are also intermediate forms of promastigotes, such as nectomonads, leptomonads and haptomonads. This adaptation ability has motivated several studies comparing the global variations in gene expression of the different parasite stages during their lifecycle (Inbar et al., 2017).
The first genome-scale quantitative analysis of gene expression during the differentiation from promastigotes to amastigotes was performed with L. donovani in a host-free system that mimics this process. Microarray-based expression profiling revealed that several hundred genes were transiently or permanently up- and downregulated during differentiation, including protein phosphatases that may be important in signal transduction (Saxena et al., 2007). Four morphological phases can be distinguished until 120 hours after the exposure of promastigotes to the differentiation signal: signal perception (phase I); movement cessation and aggregation (phase II); amastigote morphogenesis (phase III) and maturation (phase IV) (Barak et al., 2005). Shotgun phosphopeptide analysis has revealed that in axenic L. donovani, there is more stage-specific than constitutive protein phosphorylation (Tsigankov et al., 2013). To investigate the protein phosphorylation dynamics during promastigote to amastigote differentiation, a proteomic analysis was performed employing isobaric tags for relative and absolute quantitation (iTRAQ). Several proteins, including kinases and phosphatases, change their phosphorylation profiles during differentiation. The increase in phosphorylation predominated during phases I and III, whereas phases II and IV were characterized by greater dephosphorylation (Tsigankov et al., 2014).
Transcriptome analysis of different stages of L. infantum revealed that the upregulation rate is lower in intracellular amastigotes after infection of the U937 cell line compared to promastigotes of axenic cultures or metacyclic promastigotes anterior to the stomodeal valves (Pro-Pper) isolated from sand flies (Alcolea et al., 2010; Alcolea et al., 2016). This profile corroborates the hypothesis of preadaptation from promastigote forms toward life in the intracellular environment. However, the set of differentially regulated genes is notably different with respect to promastigotes from Pro-Pper instead of axenic cultures (Alcolea et al., 2016). In both cases, the upregulation of several phosphatases was described. Comparing amastigotes with logarithmic-phase culture promastigotes, putative PP2C (LinJ32_V3.1770) and membrane-bound acid phosphatase 2 (MBAP2) (LinJ23_V3.1430) were upregulated in promastigotes by 5.08- and 2.20-fold, respectively (Alcolea et al., 2010). With respect to Pro-Pper, an upregulation of 2.72-fold of a PP2C (LinJ.36.0560) and of 7.23-fold of a STP (LinJ.22.134) was observed (Alcolea et al., 2014).
The final development phase of Leishmania parasites found in sand flies is metacyclic promastigotes. The differentiation process named metacyclogenesis naturally occurs at the stomodeal valve of the insect; however, it is possible to mimic this process in vitro to obtain metacyclic promastigotes in axenic culture (Sacks et al., 1985; McConville et al., 1992). Studies with L. major have evaluated the global changes in gene expression during the maturation of axenic promastigotes from procyclic to metacyclic forms. DNA microarray analysis revealed an upregulation of a membrane-bound HAcP (lm26a07; 1.6-fold) and two STPs (lm34d12 and lm74g05; 1.2- and 2.2-fold, respectively) (Saxena et al., 2003). Posterior RNA-seq analysis showed that a PP2C-like protein (LmjF.34.2500) was 2.49-fold upregulated in L. major metacyclic promastigotes (Dillon et al., 2015).
The usual method to isolate metacyclic promastigotes from stationary phase cultures is negative selection with Arachis hypogaea lectin (peanut agglutinin, PNA). Using this approach, both fractions of procyclic (PNA+) and metacyclic (PNA−) L. infantum promastigotes can be simultaneously isolated from the same population to compare their expression profiles by whole-genome shotgun DNA microarrays. It was observed that a PP2C (LinJ15_V3.0170) was upregulated in PNA− metacyclic promastigotes (Alcolea et al., 2009). Notably, several genes previously related to infectivity are upregulated in PNA− metacyclic promastigotes, which is consistent with their increased infection rate confirmed by U937 human cell line infection experiments (Alcolea et al., 2009).
Although the promastigote culture model is stable, reproducible, and widely used for various purposes, some parasite properties are affected by culture passaging, such as infectivity and virulence. The difficulty of studying promastigotes in their natural environment is mainly related to the reduced amount of available biomass; however, it is possible to overcome this limitation by mRNA amplification for transcriptome analysis (Alcolea et al., 2014). Studies with L. infantum have revealed significant differences when comparing metacyclic promastigotes isolated from the sand fly midgut (Pro-Pper) to metacyclic promastigotes obtained in axenic culture by negative selection with PNA (Pro-PNA−) (Alcolea et al., 2016). The genes encoding a PP1 (LinJ.34.0840), a PP2B catalytic subunit A2 and a DUSP are upregulated in Pro-Pper (Alcolea et al., 2016). Consistent with the increase in in vitro infectivity, phosphoglycan β-1,3-galactosyltransferase (PG β1, 3GalT), which is involved in the biosynthesis of lipophosphoglycan (LPG) and proteophosphoglycans (PPG), is also upregulated in Pro-Pper. These glycoconjugates, which include membrane-bound and secreted HAcP, are abundant on the parasite’s surface (Alcolea et al., 2016).
Recently, global changes in gene expression were evaluated based on RNASeq from distinct insect stages of L. major during their cyclical development in vivo. The upregulation of membrane-bound HAcPs (LmjF.28.2650, LmjF.23.1170) was observed in nectomonad promastigotes. Together with the increase in autophagy-related genes, these observations suggest that differentiation to nectomonads and to metacyclic promastigotes involves a response to stress conditions, which triggers protein recycling (Inbar et al., 2017). Indeed, putative membrane-bound acid phosphatase 2-36 (MAP2-36; LinJ.36.2720) was one of the first and most significantly upregulated proteins in response to purine starvation, as described by proteome and transcriptome analysis in L. donovani axenic promastigotes (Martin et al., 2014).
Differential Expression of Phosphatases in Drug-Resistant Parasites
There are currently no effective vaccines to prevent leishmaniasis; thus, the control of this disease relies essentially on chemotherapy (Singh and Sundar, 2012). Although several different drugs are available, pentavalent antimony-containing compounds, including sodium stibogluconate (Pentostam®), are used as standard treatments against all forms of leishmaniasis, especially in Latin America (Herwaldt and Berman, 1992; Berman, 1997; Ashutosh et al., 2007). However, in the last decade, the emergence of parasites resistant to antimonials has led to an increase in therapeutic failure (Croft and Olliaro, 2011). Understanding drug resistance is essential to guarantee the efficacy of the available treatments and the development of new treatments (Hefnawy et al., 2017). In this context, several studies have been performed to elucidate the mechanisms of resistance and parasite biology in response to different drugs.
By using high-throughput RNA sequencing to analyze the transcriptome profiles, significant differences were identified between wild-type and potassium antimonyl tartrate (SbIII)-resistant L. infantum lines (abbreviated as LiWTS and LiSbR, respectively) (Andrade et al., 2020). The LiSbR line showed an upregulation of thirty-seven transcripts belonging to the protein phosphorylation category, which includes a DUSP that was 8.93-fold upregulated. In addition, a PPP and a PP2C were 2.28- to 17.52-fold upregulated, respectively (Andrade et al., 2020). This is consistent with a previous proteomic analysis that found a major abundance of both enzymes in the SbIII-resistant line (Matrangolo et al., 2013).
Similar analyses were performed using SbIII-resistant and SbIII-sensitive L. amazonensis promastigotes (La-SbIII-R and La-SbIII-S, respectively). Global transcriptomic changes point to an upregulation of genes encoding autophagy proteins in La-SbIII-R cells, suggesting a possible strategy of survival or induced cell death (Patino et al., 2019). The autophagy protein ATG9 is involved in cytoplasm-to-vacuole transport vesicle formation (Patino et al., 2019), while MBAP2 plays a role in endosomal trafficking (Inbar et al., 2017; Patino et al., 2019). Transcripts encoding APG9 (LmxM.27.0390) and MBAP2 (LmxM.23.1170) were both upregulated in La-SbIII-R (Patino et al., 2019).
Paromomycin (PMM) is an aminoglycoside antibiotic that has already been approved for the treatment of visceral leishmaniasis in Southeast Asia (Coser et al., 2021). Antimony-resistant and sensitive isolates of L. donovani are equally susceptible to PMM, making it a valid alternative treatment (Kulshrestha et al., 2011). To elucidate the mechanisms of resistance and parasite biology, a PMM-resistant strain was generated in the laboratory, and the expression of genes encoding the proteins of interest was determined by real-time PCR (Bhandari et al., 2014). A marked increase in the levels of the ATP-binding cassette (ABC) transporters MDR1 (6.83 ± 3.01-fold) and MRPA (11.47± 0.22-fold) and of PP2A (4.47 ± 0.71-fold) was observed in PMM-resistant L. donovani promastigotes. PP2A seems to be involved in activating the expression of those transporters, culminating in increased drug efflux (Bhandari et al., 2014). Comparing the genes differentially modulated in PMM-resistant and PMM-sensitive L. donovani promastigotes by transcriptome analysis, a PP2C-like protein (LinJ14_V3.0960) and a putative STP (LinJ30_V3.3330) were upregulated 3.02- and 2.97-fold, respectively, in the PMM-resistant parasites (Verma et al., 2017).
Concluding Remarks
The successful establishment of parasite infection depends on many factors. Leishmania parasites have evolved different features that allow them to survive and proliferate within their host cells. To impair the microbicidal function of macrophages, parasites can interfere with host signaling pathways. In this context, protein phosphatases play an important role. It is well known that the activation of host phosphatases is crucial for parasite survival (Shio et al., 2012). The participation of endogenous Leishmania phosphatases in the infection process has been an object of study for many years. Although their roles have not been fully elucidated, many studies suggest their involvement not only in parasite virulence but also in resistance to stress conditions during the Leishmania lifecycle.
Since the 1980s, phosphatases have been considered possible virulence factors. Previously, it was demonstrated that L. donovani HAcP was able to decrease ROS production by host immune cells (Remaley et al., 1984; Remaley et al., 1985). Furthermore, studies with L. amazonensis showed that HAcP was related to an increase in the parasite-macrophage association index (Vannier-Santos et al., 1995) and the survival of the amastigote form inside PVs (Fernandes et al., 2013).
More recently, several studies performed with L. donovani, L. major, and L. mexicana have confirmed the involvement of different phosphatases in parasite survival through the ablation and/or overexpression of specific genes (Nascimento et al., 2006; Naderer et al., 2011; Papadaki et al., 2015; Leitherer et al., 2017; Norris-Mullins et al., 2018; Kraeva et al., 2019). These endogenous phosphatases are able to favor infection mainly due to the modulation of cytokine production by macrophages (Leitherer et al., 2017; Kraeva et al., 2019). STPs seem to be particularly relevant for the ability of parasites to adapt properly during stress conditions (Naderer et al., 2011; Norris-Mullins et al., 2018). These physiological roles that have been attributed to Leishmania phosphatases are summarized in Figure 1.
Whole-genome expression analyses performed throughout the lifecycle of different Leishmania species revealed that phosphatases are generally upregulated in metacyclic promastigotes, the infective form of the mammalian host (Saxena et al., 2003; Alcolea et al., 2009; Dillon et al., 2015). While STPs and PTPs are related to cell signaling (Saxena et al., 2007; Dillon et al., 2015; Alcolea et al., 2016), membrane-bound HAcPs seem to play a role in the response to protein recycling during stress conditions, such as nutrient starvation (Martin et al., 2014; Inbar et al., 2017). Leishmania phosphatases are also upregulated in drug-resistant strains (Matrangolo et al., 2013; Bhandari et al., 2014; Verma et al., 2017; Patino et al., 2019; Andrade et al., 2020). STPs may contribute to parasite resistance by activating ABC transporters, leading to an increase in drug efflux (Bhandari et al., 2014; Verma et al., 2017). Table 1 presents the main findings related to the differential expression of Leishmania endogenous phosphatases during their lifecycle and in drug-resistant strains.
Additional studies are required to completely elucidate the signaling pathways by which the different phosphatases contribute to Leishmania infection. However, based on the data so far, it is possible to be sure that endogenous phosphatases are in fact relevant to parasite virulence and may reflect a possible target for the diagnosis or treatment of leishmaniasis.
Author Contributions
AF-M, AD-S, and JM-F wrote the manuscript. AF-M prepared the figure. All authors contributed to the article and approved the submitted version.
Funding
This work was supported by grants from the Brazilian agencies Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq - Grant Number: 401134/2014–8), Coordenação de Aperfeiçoamento de Pessoal de Nível superior (CAPES - Grant Number: 0012017), and Fundação Carlos Chagas Filho de Amparo à Pesquisa do Estado do Rio de Janeiro (FAPERJ - Grant Number: e-26/201.300/2014) to JM-F. AD-S was supported by Fundação Carlos Chagas Filho de Amparo à Pesquisa do Estado do Rio de Janeiro (FAPERJ - Grant Number: 202.378/2017).
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
References
Alcolea P. J., Alonso A., Degayón M. A., Moreno-Paz M., Jiménez M., Molina R., et al. (2016). In Vitro Infectivity and Differential Gene Expression of Leishmania Infantum Metacyclic Promastigotes: Negative Selection With Peanut Agglutinin in Culture Versus Isolation From the Stomodeal Valve of Phlebotomus Perniciosus. BMC Genomics 17, 1–14. doi: 10.1186/s12864-016-2672-8
Alcolea P. J., Alonso A., Gómez M. J., Moreno I., Domínguez M., Parro V., et al. (2010). Transcriptomics Throughout the Life Cycle of Leishmania Infantum: High Down-Regulation Rate in the Amastigote Stage. Int. J. Parasitol. 40, 1497–1516. doi: 10.1016/j.ijpara.2010.05.013
Alcolea P. J., Alonso A., Gómez M. J., Postigo M., Molina R., Jiménez M., et al. (2014). Stage-Specific Differential Gene Expression in Leishmania Infantum: From the Foregut of Phlebotomus Perniciosus to the Human Phagocyte. BMC Genomics 15, 1–16. doi: 10.1186/1471-2164-15-849
Alcolea P. J., Alonso A., Sánchez-Gorostiaga A., Moreno-Paz M., Gómez M. J., Ramos I., et al. (2009). Genome-Wide Analysis Reveals Increased Levels of Transcripts Related With Infectivity in Peanut Lectin Non-Agglutinated Promastigotes of Leishmania Infantum. Genomics 93, 551–564. doi: 10.1016/j.ygeno.2009.01.007
Alonso A., Sasin J., Bottini N., Friedberg I., Friedberg I., Osterman A., et al. (2004). Protein Tyrosine Phosphatases in the Human Genome. Cell 117, 699–711. doi: 10.1016/j.cell.2004.05.018
Andrade J. M., Gonçalves L. O., Liarte D. B., Lima D. A., Guimarães F. G., de Melo Resende D., et al. (2020). Comparative Transcriptomic Analysis of Antimony Resistant and Susceptible Leishmania Infantum Lines. Parasites. Vectors. 13, 1–15. doi: 10.1186/s13071-020-04486-4
Andreeva A. V., Kutuzov M. A. (2008). Protozoan Protein Tyrosine Phosphatases. Int. J. Parasitol. 38, 1279–1295. doi: 10.1016/j.ijpara.2008.04.003
Ashutosh S., Sundar, Goyal N. (2007). Molecular Mechanisms of Antimony Resistance in Leishmania. J. Med. Microbiol. 56, 143–153. doi: 10.1099/jmm.0.46841-0
Banerjee C., Sarkar D., Bhaduri A. (1999). Ca 2+ and Calmodulin-Dependent Protein Phosphatase From Leishmania Donovani. Parasitology 118, 567–573. doi: 10.1017/S0031182099004308
Barak E., Amin-Spector S., Gerliak E., Goyard S., Holland N., Zilberstein D. (2005). Differentiation of Leishmania Donovani in Host-Free System: Analysis of Signal Perception and Response. Mol. Biochem. Parasitol. 141, 99–108. doi: 10.1016/j.molbiopara.2005.02.004
Benzel I., Weise F., Wiese M. (2000). Deletion of the Gene for the Membrane-Bound Acid Phosphatase of Leishmania Mexicana. Mol. Biochem. Parasitol. 111, 77–86. doi: 10.1016/S0166-6851(00)00306-6
Beresford N. J., Saville C., Bennett H. J., Roberts I. S., Tabernero L. (2010). A New Family of Phosphoinositide Phosphatases in Microorganisms: Identification and Biochemical Analysis. BMC Genomics 11, 1–12. doi: 10.1186/1471-2164-11-457
Berman J. D. (1997). Human Leishmaniasis: Clinical, Diagnostic, and Chemotherapeutic Developments in the Last 10 Years. Clin. Infect. Dis. 24, 684–703. doi: 10.1093/clind/24.4.684
Bhandari V., Sundar S., Dujardin J. C., Salotra P. (2014). Elucidation of Cellular Mechanisms Involved in Experimental Paromomycin Resistance in Leishmania Donovani. Antimicrob. Agents Chemother. 58, 2580–2585. doi: 10.1128/AAC.01574-13
Blanchette J., Racette N., Faure R., Siminovitch K. A., Olivier M. (1999). Leishmania-Induced Increases in Activation of Macrophage SHP-1 Tyrosine Phosphatase are Associated With Impaired IFN-Γ-Triggered JAK2 Activation. Eur. J. Immunol. 29, 3737–3744. doi: 10.1002/(SICI)1521-4141(199911)29:11<3737::AID-IMMU3737>3.0.CO;2-S
Borthwick E. B., Zeke T., Prescott A. R., Cohen P. T. (2001). Nuclear Localization of Protein Phosphatase 5 is Dependent on the Carboxy-Terminal Region. FEBS Lett. 491, 279–284. doi: 10.1016/S0014-5793(01)02177-9
Burns J. M., Parsons M., Rosman D. E., Reed S. G. (1993). Molecular Cloning and Characterization of a 42-Kda Protein Phosphatase of Leishmania Chagasi. J. Biol. Chem. 268, 17155–17161.
Chang K. P. (1983). Cellular and Molecular Mechanisms of Intracellular Symbiosis in Leishmaniasis. Int. Rev. Cytol. Suppl. 14, 267–305.
Cohen P. T. W. (1997). Novel Protein Serine/Threonine Phosphatases: Variety is the Spice of Life. Trends Biochem. Sci. 22, 245–251. doi: 10.1016/S0968-0004(97)01060-8
Coker O., Warit S., Rukseree K., Summpunn P., Prammananan T., Palittapongarnpim P. (2013). Functional Characterization of Two Members of Histidine Phosphatase Superfamily in Mycobacterium Tuberculosis. BMC Microbiol. 13, 292. doi: 10.1186/1471-2180-13-292
Cosentino-Gomes D., Meyer-Fernandes J. R. (2011). Ecto-Phosphatases in Protozoan Parasites: Possible Roles in Nutrition, Growth and ROS Sensing. J. Bioenerg. Biomembr. 43, 89–92. doi: 10.1007/s10863-011-9334-y
Coser E. M., Ferreira B. A., Yamashiro-Kanashiro E. H., Lindoso J. A. L., Coelho A. C. (2021). Susceptibility to Paromomycin in Clinical Isolates and Reference Strains of Leishmania Species Responsible for Tegumentary Leishmaniasis in Brazil. Acta Trop. 215, 105806. doi: 10.1016/j.actatropica.2020.105806
Croft S. L., Olliaro P. (2011). Leishmaniasis Chemotherapy—Challenges and Opportunities. Clin. Microbiol. Infect. 17, 1478–1483. doi: 10.1111/j.1469-0691.2011.03630.x
de Almeida-Amaral E. E., Belmont-Firpo R., Vannier-Santos M. A., Meyer-Fernandes J. R. (2006). Leishmania Amazonensis: Characterization of an Ecto-Phosphatase Activity. Exp. Parasitol. 114, 334–340. doi: 10.1016/j.exppara.2006.04.011
Dillon L. A. L., Okrah K., Hughitt K. V., Suresh R., Li Y., Fernandes M. C., et al. (2015). Transcriptomic Profiling of Gene Expression and RNA Processing During Leishmania Major Differentiation. Nucleic Acids Res. 43, 6799–6813. doi: 10.1093/nar/gkv656
Escalona-Montaño A. R., Ortiz-Lozano D. M., Rojas-Bernabé A., Wilkins-Rodriguez A. A., Torres-Guerrero H., Mondragón-Flores R., et al. (2016). Leishmania Mexicana: Promastigotes and Amastigotes Secrete Protein Phosphatases and This Correlates With the Production of Inflammatory Cytokines in Macrophages. Parasitology 143, 1409–1420. doi: 10.1017/S0031182016000949
Escalona-Montaño A. R., Pardavé-Alejandre D., Cervantes-Sarabia R., García-López P., Gutiérrez-Quiroz M., Gutiérrez-Kobeh L., et al. (2010). Leishmania Mexicana Promastigotes Secrete a Protein Tyrosine Phosphatase. Parasitol. Res. 107, 309–315. doi: 10.1007/s00436-010-1863-5
Fernandes A. C. S., Soares D. C., Saraiva E. M., Meyer-Fernandes J. R., Souto-Padrón T. (2013). Different Secreted Phosphatase Activities in Leishmania Amazonensis. FEMS Microbiol. Lett. 340, 117–128. doi: 10.1111/1574-6968.12080
Forget G., Gregory D. J., Whitcombe L. A., Olivier M. (2006). Role of Host Protein Tyrosine Phosphatase SHP-1 in Leishmania Donovani-Induced Inhibition of Nitric Oxide Production. Infect. Immun. 74, 6272–6279. doi: 10.1128/IAI.00853-05
Freitas-Mesquita A. L., Meyer-Fernandes J. R. (2014). Ecto-Nucleotidases and Ecto-Phosphatases From Leishmania and Trypanosoma Parasites. Subcell. Biochem. 74, 217–252. doi: 10.1007/978-94-007-7305-9_10
Hefnawy A., Berg M., Dujardin J.-C., De Muylder G. (2017). Exploiting Knowledge on Leishmania Drug Resistance to Support the Quest for New Drugs. Trends Parasitol. 33, 162–174. doi: 10.1016/j.pt.2016.11.003
Herwaldt B. L., Berman J. D. (1992). Recommendations for Treating Leishmaniasis With Sodium Stibogluconate (Pentostam) and Review of Pertinent Clinical Studies. Am. J. Trop. Med. Hyg. 46, 296–306. doi: 10.4269/ajtmh.1992.46.296
Hussain S. K., Broederdorf L. J., Sharma U. M., Voth D. E. (2010). Host Kinase Activity is Required for Coxiella Burnetii Parasitophorous Vacuole Formation. Front. Microbiol. 1, 1–10. doi: 10.3389/fmicb.2010.00137
Inbar E., Hughitt V. K., Dillon L. A. L., Ghosh K., El-Sayed N. M., Sacks D. L. (2017). The Transcriptome of Leishmania Major Developmental Stages in Their Natural Sand Fly Vector. MBio 8, 1–18. doi: 10.1128/mBio.00029-17
Jakkula P., Qureshi R., Iqbal A., Sagurthi S. R., Qureshi I. A. (2018). Leishmania Donovani PP2C: Kinetics, Structural Attributes and in Vitro Immune Response. Mol. Biochem. Parasitol. 223, 37–49. doi: 10.1016/j.molbiopara.2018.06.005
Katakura K., Kobayashi A. (1988). Acid Phosphatase Activity of Virulent and Avirulent Clones of Leishmania Donovani Promastigotes. Infect. Immun. 56, 2856–2860. doi: 10.1128/IAI.56.11.2856-2860.1988
Kraeva N., Leštinová T., Ishemgulova A., Majerová K., Butenko A., Vaselek S., et al. (2019). Lmxm.22.0250-Encoded Dual Specificity Protein/Lipid Phosphatase Impairs Leishmania Mexicana Virulence in Vitro. Pathogens 8, 1–14. doi: 10.3390/pathogens8040241
Kulshrestha A., Singh R., Kumar D., Negi N. S., Salotra P. (2011). Antimony-Resistant Clinical Isolates of Leishmania Donovani are Susceptible to Paromomycin and Sitamaquine. Antimicrob. Agents Chemother. 55, 2916–2921. doi: 10.1128/AAC.00812-10
Leitherer S., Clos J., Liebler-Tenorio E. M., Schleicher U., Bogdan C., Soulat D. (2017). Characterization of the Protein Tyrosine Phosphatase Lmprl-1 Secreted by Leishmania Major Via the Exosome Pathway. Infect. Immun. 85, 1–19. doi: 10.1128/IAI.00084-17
Martin J. L., Yates P. A., Soysa R., Alfaro J. F., Yang F., Burnum-Johnson K. E., et al. (2014). Metabolic Reprogramming During Purine Stress in the Protozoan Pathogen Leishmania Donovani. PloS Pathog. 10, 1–21. doi: 10.1371/journal.ppat.1003938
Matrangolo F. S. V., Liarte D. B., Andrade L. C., de Melo M. F., Andrade J. M., Ferreira R. F., et al. (2013). Comparative Proteomic Analysis of Antimony-Resistant and -Susceptible Leishmania Braziliensis and Leishmania Infantum Chagasi Lines. Mol. Biochem. Parasitol. 190, 63–75. doi: 10.1016/j.molbiopara.2013.06.006
McCall L.-I., Matlashewski G. (2010). Localization and Induction of the A2 Virulence Factor in Leishmania: Evidence That A2 is a Stress Response Protein. Mol. Microbiol. 77, 518–530. doi: 10.1111/j.1365-2958.2010.07229.x
McConville M. J., Turco S. J., Ferguson M. A., Sacks D. L. (1992). Developmental Modification of Lipophosphoglycan During the Differentiation of Leishmania Major Promastigotes to an Infectious Stage. EMBO J. 11, 3593–3600.
Mills E., Price H. P., Johner A., Emerson J. E., Smith D. F. (2007). Kinetoplastid PPEF Phosphatases: Dual Acylated Proteins Expressed in the Endomembrane System of Leishmania. Mol. Biochem. Parasitol. 152, 22–34. doi: 10.1016/j.molbiopara.2006.11.008
Naderer T., Dandash O., Mcconville M. J. (2011). Calcineurin is Required for Leishmania Major Stress Response Pathways and for Virulence in the Mammalian Host. Mol. Microbiol. 80, 471–480. doi: 10.1111/j.1365-2958.2011.07584.x
Nascimento M., Abourjeily N., Ghosh A., Zhang W. W., Matlashewski G. (2003). Heterologous Expression of a Mammalian Protein Tyrosine Phosphatase Gene in Leishmania: Effect on Differentiation. Mol. Microbiol. 50, 1517–1526. doi: 10.1046/j.1365-2958.2003.03811.x
Nascimento M., Zhang W., Ghosh A., Houston D. R., Berghuis A. M., Olivier M., et al. (2006). Identification and Characterization of a Protein-Tyrosine Phosphatase in. Leishmania 281, 36257–36268. doi: 10.1074/jbc.M606256200
Norris-Mullins B., Krivda J. S., Smith K. L., Ferrell M. J., Morales M. A. (2018). Leishmania Phosphatase PP5 is a Regulator of HSP83 Phosphorylation and Essential for Parasite Pathogenicity. Parasitol. Res. 117, 2971–2985. doi: 10.1007/s00436-018-5994-4
Papadaki A., Politou A. S., Smirlis D., Kotini M. P., Kourou K., Papamarcaki T., et al. (2015). The Leishmania Donovani Histidine Acid Ecto-Phosphatase Ldmacp: Insight Into Its Structure and Function. Biochem. J. 467, 473–486. doi: 10.1042/BJ20141371
Patino L. H., Muskus C., Ramírez J. D. (2019). Transcriptional Responses of Leishmania (Leishmania) Amazonensis in the Presence of Trivalent Sodium Stibogluconate. Parasites. Vectors. 12, 1–15. doi: 10.1186/s13071-019-3603-8
Qureshi R., Jakkula P., Sagurthi S. R., Qureshi I. A. (2019). Protein Phosphatase 1 of Leishmania Donovani Exhibits Conserved Catalytic Residues and Pro-Inflammatory Response. Biochem. Biophys. Res. Commun. 516, 770–776. doi: 10.1016/j.bbrc.2019.06.085
Remaley A. T., Glew R., Kuhns D. B., Basford R. E., Waggoner A., Ernst A., et al. (1985). Leishmania Donovani: Surface Membrane Acid Phosphatase Oxidative Metabolite Production. Exp. Parasitol. 60, 331–341. doi: 10.1016/0014-4894(85)90039-6
Remaley A. T., Kuhns D. B., Basford R. E., Glew R. H., Kaplan S. S. (1984). Leishmanial Phosphatase Blocks Neutrophil O2- Production. J. Biol. Chem. 259, 11173–11175.
Rigden D. J. (2008). The Histidine Phosphatase Superfamily: Structure and Function. Biochem. J. 409, 333–348. doi: 10.1042/BJ20071097
Rodríguez A., Roy J., Martínez-Martínez S., López-Maderuelo M. D., Niño-Moreno P., Ortí L., et al. (2009). A Conserved Docking Surface on Calcineurin Mediates Interaction With Substrates and Immunosuppressants. Mol. Cell. 33, 616–626. doi: 10.1016/j.molcel.2009.01.030
Sacks D. L., Hieny S., Sher A. (1985). Identification of Cell Surface Carbohydrate and Antigenic Changes Between Noninfective and Infective Developmental Stages of Leishmania Major Promastigotes. J. Immunol. 135, 564–569.
Saha A. K., Das S., Glew R. H., Gottlieb M. (1985). Resistance of Leishmanial Phosphatases to Inactivation by Oxygen Metabolites. J. Clin. Microbiol. 22, 329–332. doi: 10.1128/jcm.22.3.329-332.1985
Saxena A., Lahav T., Holland N., Aggarwal G., Anupama A., Huang Y., et al. (2007). Analysis of the Leishmania Donovani Transcriptome Reveals an Ordered Progression of Transient and Permanent Changes in Gene Expression During Differentiation. Mol. Biochem. Parasitol. 152, 53–65. doi: 10.1016/j.molbiopara.2006.11.011
Saxena A., Worthey E. A., Yan S., Leland A., Stuart K. D., Myler P. J. (2003). Evaluation of Differential Gene Expression in Leishmania Major Friedlin Procyclics and Metacyclics Using DNA Microarray Analysis. Mol. Biochem. Parasitol. 129, 103–114. doi: 10.1016/S0166-6851(03)00100-2
Shakarian A. M., Ellis S. L., Mallinson D. J., Olafson R. W., Dwyer D. M. (1997). Two Tandemly Arrayed Genes Encode the (Histidine) Secretory Acid Phosphatases of Leishmania Donovani. Gene 196, 127–137. doi: 10.1016/S0378-1119(97)00218-7
Shakarian A. M., Joshi M. B., Ghedin E., Dwyer D. M. (2002). Molecular Dissection of the Functional Domains of a Unique, Tartrate-Resistant, Surface Membrane Acid Phosphatase in the Primitive Human Pathogen Leishmania Donovani. J. Biol. Chem. 277, 17994–18001. doi: 10.1074/jbc.M200114200
Shio M. T., Hassani K., Isnard A., Ralph B., Contreras I., Gomez M. A., et al. (2012). Host Cell Signalling and Leishmania Mechanisms of Evasion. J. Trop. Med. 2012, 1–14. doi: 10.1155/2012/819512
Singh B., Sundar S. (2012). Leishmaniasis: Vaccine Candidates and Perspectives. Vaccine 30, 3834–3842. doi: 10.1016/j.vaccine.2012.03.068
Singla N. (1992). Acid Phosphatase Activity of Promastigotes of Leishmania Donovani: A Marker of Virulence. FEMS Microbiol. Lett. 94, 221–225. doi: 10.1016/0378-1097(92)90634-Z
Soulat D., Bogdan C. (2017). Function of Macrophage and Parasite Phosphatases in Leishmaniasis, Front. Immunol 8, 1–21. doi: 10.3389/fimmu.2017.01838
Szöör B. (2010). Trypanosomatid Protein Phosphatases, Mol. Biochem. Parasitol. 173, 53–63. doi: 10.1016/j.molbiopara.2010.05.017
Tonks N. K. (2003). PTP1B: From the Sidelines to the Front Lines! FEBS Lett. 546, 140–148. doi: 10.1016/S0014-5793(03)00603-3
Tsigankov P., Gherardini P. F., Helmer-Citterich M., Späth G. F., Myler P. J., Zilberstein D. (2014). Regulation Dynamics of Leishmania Differentiation: Deconvoluting Signals and Identifying Phosphorylation Trends. Mol. Cell. Proteomics. 13, 1787–1799. doi: 10.1074/mcp.M114.037705
Tsigankov P., Gherardini P. F., Helmer-Citterich M., Späth G. F., Zilberstein D. (2013). Phosphoproteomic Analysis of Differentiating Leishmania Parasites Reveals a Unique Stage-Specific Phosphorylation Motif. J. Proteome Res. 12, 3405–3412. doi: 10.1021/pr4002492
Vannier-Santos M. A., Martiny A., Meyer-Fernandes J. R., de Souza W. (1995). Leishmanial Protein Kinase C Modulates Host Cell Infection Via Secreted Acid Phosphatase. Eur. J. Cell Biol. 67, 112–119.
Verma A., Bhandari V., Deep D. K., Sundar S., Dujardin J. C., Singh R., et al. (2017). Transcriptome Profiling Identifies Genes/Pathways Associated With Experimental Resistance to Paromomycin in Leishmania Donovani. Int. J. Parasitol. Drugs Drug Resist. 7, 370–377. doi: 10.1016/j.ijpddr.2017.10.004
Wiese M. (1996). Gene Cloning and Cellular Localization of a Membrane-Bound Acid Phosphatase of Leishmania Mexicana. Mol. Biochem. Parasitol. 82, 153–165. doi: 10.1016/0166-6851(96)02729-6
Wiese M., Ilg T., Lottspeich F., Overath P. (1995). Ser/Thr-Rich Repetitive Motifs as Targets for Phosphoglycan Modifications in Leishmania Mexicana Secreted Acid Phosphatase. EMBO J. 14, 1067–1074.
Zhou Y., Bhattacharjee H., Mukhopadhyay R. (2006). Bifunctional Role of the Leishmanial Antimonate Reductase Lmacr2 as a Protein Tyrosine Phosphatase, Mol. Biochem. Parasitol. 148, 161–168. doi: 10.1016/j.molbiopara.2006.03.009
Keywords: Leishmania spp, phosphatases, phosphate metabolism, parasite virulence, parasite infection
Citation: Freitas-Mesquita AL, Dos-Santos ALA and Meyer-Fernandes JR (2021) Involvement of Leishmania Phosphatases in Parasite Biology and Pathogeny. Front. Cell. Infect. Microbiol. 11:633146. doi: 10.3389/fcimb.2021.633146
Received: 24 November 2020; Accepted: 06 April 2021;
Published: 22 April 2021.
Edited by:
Juan David Ramírez, Rosario University, ColombiaReviewed by:
Juliana Ide Aoki, University of São Paulo, BrazilMaria Aguirre-Garcia, Universidad Nacional Autónoma de México, Mexico
Copyright © 2021 Freitas-Mesquita, Dos-Santos and Meyer-Fernandes. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Anita Leocadio Freitas-Mesquita, anitaleocadio2@gmail.com; José Roberto Meyer-Fernandes, meyer@bioqmed.ufrj.br