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Let it glow: genetically encoded fluorescent reporters in Plasmodium

Malaria Journal volume 23, Article number: 114 (2024) Cite this article

Abstract

The use of fluorescent proteins (FPs) in Plasmodium parasites has been key to understand the biology of this obligate intracellular protozoon. FPs like the green fluorescent protein (GFP) enabled to explore protein localization, promoter activity as well as dynamic processes like protein export and endocytosis. Furthermore, FP biosensors have provided detailed information on physiological parameters at the subcellular level, and fluorescent reporter lines greatly extended the malariology toolbox. Still, in order to achieve optimal results, it is crucial to know exactly the properties of the FP of choice and the genetic scenario in which it will be used. This review highlights advantages and disadvantages of available landing sites and promoters that have been successfully applied for the ectopic expression of FPs in Plasmodium berghei and Plasmodium falciparum. Furthermore, the properties of newly developed FPs beyond DsRed and EGFP, in the visualization of cells and cellular structures as well as in the sensing of small molecules are discussed.

Graphical Abstract

Fluorescent proteins driving Plasmodium discoveries

Plasmodium parasites, the causative agents of malaria, have evolved a unique parasitic life style, which requires switching between a vertebrate and an insect host, oscillating from motile to immotile forms, as well as between protist-like, sessile, intracellular and facultative intracellular stages (Fig. 1). Each of these stages is equipped with its own set of proteins, many of them functioning at the host-parasite interface, being either secreted towards the plasma membrane to ensure motility and recognition of tissues or scavenging nutrients and remodeling host cells. Imaging of different Plasmodium stages on different scales has significantly contributed to a better understanding of the function of individual proteins and of parasite-specific structures (reviewed in detail in [1]). To gain insights into the biology of Plasmodium and other organisms, genetically encoded fluorescent proteins (FPs) have made a historical contribution as they allow the localization of compartments and proteins in vivo and in vitro thus also the visualization of dynamic processes. Although FPs fused to proteins can cause mis-trafficking or impair protein function, the possibility to visualize processes in living cells gives FPs decisive advantages over immunofluorescence-based methods, which require fixation and subsequent staining.

Fig. 1
figure 1

Stage-specific and constitutive expression of FPs along the Plasmodium life cycle. Human and mosquito outlines displayed in the center illustrate the division of the parasite cycle in insect-specific and vertebrate-specific stages. Fluorescent P. berghei and P. falciparum reporter lines driving expression of the respective FP from classical genomic loci used for ectopic gene expression are shown. Reporter lines are classified in constitutive, oocyst- and sporozoite-specific, zoite-specific, sporozoite- and/or liver stage-specific as well as gametocyte-specific. The colour code highlighting the different expression groups matches with that of the life cycle sections the respective lines express the fluorescent reporter. Images of the P. berghei fluo line are shown as an example of a reporter line with both constitutive (GFP driven by the ef1a promoter) and stage-specific FP expression (mCherry driven by the CSP promoter in late oocysts, sporozoites and early liver stages). Merged images showing GFP and mCherry expression in combination with nuclear staining are shown for all stages. The scale bar for all images is 10 µm except for midgut and salivary gland where it represents 100 µm. Please note that P. falciparum reporter lines making use of the etramp10.3./peg4 promoter also display FP expression in gametocytes, although not shown here. Also, the P. berghei reporter line PbGFP103464 is fluorescent in late liver stages only, while the reporter line PbANKA-Cherry 2204cl5 is fluorescent in sporozoites and liver stages

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An extremely important dynamic process with significant implications for malaria pathology is the uptake of haemoglobin by the parasite when developing within a red blood cell (RBC). While the parasite grows within human RBCs, it develops from a ring stage into a trophozoite that subsequently matures into a schizont. The latter divides into a number of merozoites that upon release, invade new RBCs and continue asexual replication. During its development inside RBCs, Plasmodium main source of amino acids is haemoglobin. However, the parasite is separated from the RBC cytoplasm by a parasitophorous vacuole membrane impeding haemoglobin uptake. A recent study shed light on the pathway that initiates endocytosis of haemoglobin by using FPs to tag the Kelch propeller protein K13, a protein involved in artemisinin resistance, and its interactome [2]. It also demonstrated that reduced expression of K13 can slow down endocytosis, making anti-malarials, such as artemisinin, less effective [2]. While the majority of merozoites that invade RBCs replicate asexually, a minority commits to become gametocytes, the only form that is infectious to mosquitoes. How sexual commitment is regulated and how individual parasites decide their developmental path remained elusive for a long time. The protein gametocyte development 1 (GDV1) was recently discovered to be a key regulator in this process. By fusing GDV1 with a reporter consisting of GFP and a destabilization domain, gametocyte conversion was shown to be highly dependent on the expression level of GDV1, which acts as a transcriptional activator of silenced gametocyte specific genes [3].

Mature male and female gametocytes, when ingested by a female Anopheles mosquito during a blood meal, become activated and subsequently fuse to form a zygote. The zygote develops into a motile stage, called ookinete, which crosses the midgut epithelium. Once the ookinete reaches the basal lamina, it transforms into a sessile oocyst which, after growing for up to two weeks, divides into thousands of motile sporozoites. During all these stage transitions, gametocyte to gamete(s), zygote to ookinete and oocyst to sporozoite(s), chromosomal rearrangements play an important role in DNA replication and distribution. Recently, the C-terminal fusion of kinsesin-8X to GFP enabled the representation of mitotic and meiotic parasitic stages in vivo with unprecedented accuracy [4]. Similarly, the production of interdomain GFP fusion proteins with the circumsporozoite protein, an important vaccine candidate for malaria prophylaxis, allowed new insights into the transport and processing of this important protein as well as into the formation of sporozoites during oocyst development [5]. Sporozoites emerging from oocysts, are released into the haemolymph and cross the salivary gland epithelium to reach the lumen from which they will be deposited with the saliva in the dermis of hosts upon blood feeding. Transmitted sporozoites actively move to enter the bloodstream, which transports them to the liver.

Using parasite lines expressing FPs at the sporozoite stage and software-based analysis to quantify movement patterns, it could be shown that sporozoites sense environmental elasticity to discriminate between different tissues [6] and that sporozoites of human and rodent infecting malaria species require no species-specific adaptations to traverse the skin of different hosts [7]. In the liver parasites invade hepatocytes and develop as exoerythrocytic forms (EEFs) until they undergo schizogony to form thousands of merozoites. In order to be efficiently released from infected hepatocytes, the parasites must disrupt the parasitophorous vacuole in a phospholipase-mediated process that subsequently leads to the death of the host cell and the detachment of merozoite-filled vesicles, the merosomes [8, 9]. Merozoites released from EEFs invade RBCs and complete the life cycle. As illustrated by these few examples here, the use of fluorescent proteins has made significant contributions to understand the life cycle of Plasmodium in general, and of stage-dependent adaptations and stage-to-stage transitions in particular. In addition to the classical use of genetically encoded FPs for labelling cells or subcellular structures by fusion with proteins of interest, a number of Plasmodium specific applications for FPs have been invented, which are discussed in more detail below.

Plasmodium-specific applications of FPs

The unique life cycle of Plasmodium has led to the development of a number of applications where FPs have proven particularly useful. Transgenesis in Plasmodium requires usually subsequent purification of the transgenic parasites to ensure the absence of wild-type. This is usually done by creating isogenic populations founded by a single parasite. In the case of Plasmodium falciparum, isogenic lines can be produced by simply sowing individual parasites in wells and allowing them to grow in vitro. In contrast, the generation of isogenic populations in rodent malaria parasites requires the injection of single parasites into mice (~ 8–10 per transgene) to ultimately obtain multiple clones of transgenic parasites. Blood stage-specific expression of FPs enables fluorescence-activated cell sorting (FACS) of successfully transfected parasites immediately after transfection [10]. Besides saving time and animals, this method also preserves the genetic diversity of the strain as the parasite populations produced are homogenic to the transgene but polyclonally founded. A further improvement of the FACS-based approach is the fusion of FPs with luciferases. The expression of FPs enables the microscopic detection of parasites, but also the sorting with flow cytometry for different experimental set-ups. On the other hand, the luciferase fused to the FP makes it possible to visualize the sequestration of parasites in the vasculature and the spleen but also to compare the parasite burden in the liver in vivo (reviewed in detail in [11]). Other uses of parasites expressing FP-luciferase fusions are multiplexing approaches in vitro, e.g. for drug screening assays in P. falciparum [12] or the quantification of parasite burden in Plasmodium berghei [13]. Besides methodological facilitation, the use of FPs also contributed to better understand Plasmodium unique sexual reproduction. Dual fluorescent reporter lines with male and female gametocyte-specific FP expression allow monitoring of gamete fusion and ookinete conversion by flow cytometry. This evidenced how important the detachment of the erythrocyte membrane is for the subsequent fusion of male and female gametes [14]. Similarly, sexual hybridization of Plasmodium lines expressing differently coloured FPs can be exploited to bypass lethal gene defects in ookinetes and oocysts and allow the study of loss-of-function mutants in sporozoites and liver stages. Indeed, a loss-of-function parasite line constitutively expressing a fluorescent reporter can be crossed with a fluorescent reporter line expressing a FP of a different colour. When the gametes of both lines fuse, the functional allele of the fluorescent control rescues the lethal developmental defect of the loss-of-function transgene and allows the formation of an oocyst expressing both FPs. Subsequent cell division results in haploid sporozoites with different genotypes. A subset of them exclusively carries the loss-of-function allele that is trackable by its FP reporter. Cross-fertilization revealed that the prohibitin-like protein in P. berghei is not required for transmission and development of liver stages [15]. In contrast, cross-fertilized ferrochetalase-deficient P. berghei parasites are unable to complete liver development [16].

FPs have also been used to investigate transport processes in Plasmodium. Translocation of proteins across different membranes was studied by fusing GFP to murine dihydrofolate reductase (mDHFR). In the presence of membrane-permeable folate analogues (e.g. WR99210), the mDHFR adopts a very stable fold which prevents protein translocation across membranes. By adding the folate analogue, protein transport can be blocked in a time- and dose-dependent manner, which can be followed in real time by visualizing the attached GFP. Using this method, the export of parasite proteins into the cytoplasm of infected RBCs was shown to require protein unfolding [17] and, more recently, the same approach was used to jam protein import into the parasite apicoplast [18]. As these examples highlight, genetically encoded FPs are often fused to other proteins to extend their utility. In the following sections, we focus in particular on the monomeric expression of FPs to enable fluorescence-based detection of cells without approaching the subcellular level. Whilst this approach can be considered the simplest, the promoter driving FP expression and the landing site chosen can be critical to the progression of a project. Advantages and disadvantages of available promoters and landing sites as well as the properties of newly developed FPs for visualisation and small molecule sensing are discussed.

Genomic loci used for ectopic gene expression (of FPs) in P. berghei and P. falciparum

Genetically encoded FPs can be integrated into the parasite genome in various ways. Common strategies include the labeling of endogenous proteins with FPs or the knockout of genes by replacing them with genetic cassettes encoding FPs. Of note, the insertion site might affect the expression level of the reporter, which can be a problem if fluorescence quantification is required to compare different mutants. In addition, it may not always be possible to integrate a FP, for example if a genetic cassette with a different genetic cargo is to be integrated or if only single bases within a coding sequence are to be edited. In this case it is often required to use a fluorescent line with ectopical expression of a suitable FP at a separate integration site. In order to save time, resources and, in the case of rodent-infecting Plasmodium species, animals for cultivation, already existing lines should be used when possible. Commonly used parasite lines expressing FPs either as a monomer or fused to luciferase are listed in Table 1 and 2 for P. berghei and P. falciparum, respectively. If a project requires the creation of a line with the expression of a specific FP or a specific expression pattern, it is often recommended to use one of the already utilized landing sites for ectopic transgenes. Historically, the first targeted locus to integrate ectopically expressed transgenes in P. berghei was the dihydrofolate reductase (dhfr) gene because the selection marker TgDHFR-TS would restore the essential function of the endogenous gene while also providing resistance to the drugs pyrimethamine and WR99210 (see "List of abbreviations") [19]. Later studies in P. berghei focused on redundant genes like the C- and D-rRNA genes (C-/D-rRNA) [20,21,22] and the p230p gene, a member of the s48/45 domain containing 6-cysteine (6-cys) protein family [23]. In P. falciparum integrations into the locus of another 6-cys family member, Pfs47, do not interfere with life cycle progression [24], which made it a common landing site [25]. Still, P. falciparum lines lacking Pfs47 expression are unable to infect native African malaria vectors. A possible alternative to the Pfs47 locus could be the lisp1 locus, which has recently been explored in P. falciparum as target site for the ectopic expression of transgenes [26]. While lisp1 may be required for efficient merozoite exit from the liver stages, it has no effect on other stages of the life cycle [27]. Further alternatively explored loci in P. falciparum have been obc13 and pare, both believed to be redundant for the Plasmodium life cycle. Pare encodes a prodrug activation and resistance esterase that is dispensable for the parasite. In addition, the loss of pare makes the parasites resistant to the drug MMV011438 enabling negative selection [28]. The use of the obc13 locus, enabling constitutive reporter gene expression without affecting life cycle progression, is also promising [29]. The knockout of OBC13 has been described to have no phenotype in gametocytes in vitro, while in vivo oocyst numbers decrease slightly. Another potentially interesting landing site in P. falciparum is RH3, a putative pseudogene being transcribed in schizonts but not translated, possibly due to frameshift mutations [30, 31]. To further limit a possible interference with endogenous gene expression, transgenes in P. berghei have been placed into transcriptionally silent loci on chromosome 6 (SIL6) [32] and chromosome 12 (named here SIL12) [5, 33]. Similarly, the 3'UTR of the cg6 gene in P. falciparum was used to host transgenes [34]. Intuitively, intergenic sequences are preferable to landing sites in coding regions. However, changes in the transcription of neighbouring genes can occur, which are often subtle and not easy to detect. For example, SIL12 is located near the coding sequence of the mitochondrial protein MPODD, potentially limiting the usability of this landing site for studies on mitochondrial function [35].

Table 1 List of reporter lines in P. berghei with FP expression in an otherwise unaltered genetic background. Compilation of transgenic lines with ectopic expression of FPs either as monomer or in fusion with luciferase
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Table 2 List of reporter lines in P. falciparum with FP expression in an otherwise unaltered genetic background
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Promoters used to drive constitutive and stage-specific expression of FPs in P. berghei and P. falciparum

Plasmodium lines with constitutive or stage-specific cytoplasmic expression of different FPs have greatly simplified quantification, sorting and visualization of parasites. However, the application possibilities of a reporter line always depend on the promoter that controls the expression of the respective FP. Since the stages and activities of the promoters of the same gene can differ significantly between different Plasmodium species, a large number of fluorescent reporter lines with different applications has been created. Most reporter lines have been generated in P. falciparum and P. berghei, causing malaria in humans and rodents, respectively. P. berghei has proven to be particularly useful to study insect stages and their transmission, which is difficult to reproduce with P. falciparum. Application-related fluorescent reporter lines with constitutive gene expression in both parasite species enabled the use of fluorescence-based methods along the life cycle. The first promoter used to engineer reporter lines with constitutive expression was the 5’UTR of elongation factor 1α (ef1α) that can drive FP expression in both P. berghei [10, 21, 36,37,38] and P. falciparum [25, 39,40,41]. While the toolbox of constitutive promoters in P. berghei for ectopic gene expression is limited to ef1α and heat shock protein 70 (hsp70) which drives significantly stronger gene expression compared to ef1α [42,43,44,45,46], additional promoters have been used to engineer constitutive fluorescent reporter lines in P. falciparum, notably glyceraldehyde-3-phosphate dehydrogenase (gapdh), calmodulin (cam) as well as the promoters of the two housekeeping genes translation initiation factor SUI1 (sui1) and 40s ribosomal protein S30 (40s) [25, 46, 47]. Cam is a weaker driver compared to gapdh [46], and sui1 as well as 40s provide stronger gene expression than ef1α in P. falciparum [25]. Still, thus far, all tested constitutive promoters in P. falciparum are significantly weaker than the P. berghei hsp70 promoter, which impedes their usefulness for applications requiring strong fluorescence.

Stage-specific transcriptional elements have also been used to generate reporter lines. For example, the promoter of the apical membrane antigen 1 (ama1), which guides gene expression in schizonts, merozoites and sporozoites, has been used to generate transgenic P. berghei lines expressing GFP-luciferase fusion proteins. While the expression of GFP in these lines enabled the selection of transgenic parasites by FACS, their primary use was the luciferase-based localization of sequestering schizonts in infected mice [48, 49]. Equally important, Plasmodium sexual commitment has been a long-term interest of researchers because the timing of gametocyte development as well as the percentage of viable gametocytes are crucial for transmission. Moreover, gametocytes persist upon treatment with most common anti-malarial drugs, which allows parasites to continue to be transmitted to mosquitoes even during treatment. Since gametocyte development in P. falciparum takes place in different morphologically recognizable stages, it was relatively simple to find promoters that switch on the expression of FPs in relation to the developmental status. Promoter of the helical interspersed subtelomeric protein GEXP02 (gexp02), Pfs16 (pfs16) as well as the protein Pfs48/45 (pfs48/45) have been used in P. falciparum to generate fluorescent reporter lines very early on during sexual commitment. Interestingly a subset of schizonts expressed tdTomato in the gexp02 driven line although they were reported negative for the early gametocyte marker Pfs16 by immunofluorescence stainings [26]. Similarly, although placed under the control of the pfs16 promoter, FP expression was also detected in asexual blood stages [26], while a previously generated reporter line using the same promoter has been reported to display a high degree of gametocyte specificity [34]. Whether this is a natural occurring expression pattern of both gexp02 and pfs16 promoters, or technical artefacts due to the size of the selected 5’UTR fragments or to locus-specific effects linked to different genomic integration sites, remains to be investigated. Besides promoters that are active early in gametogenesis, the mal8p1.16 promoter was used to engineer a reporter line with high expression levels in mature gametocytes [34].

In contrast to P. falciparum, different gametocyte stages are not recognizable in P. berghei. The generation of gametocyte reporter lines in P. berghei has, therefore, focused on sex-specific expression. The promoter of the male development gene 1 (mdv-1/peg3) has been shown to induce higher transcriptional activity in female than in male gametocytes and was used to generate a fluorescent reporter line enabling sex differentiation by flow cytometry [14]. Similarly, the surface protein p28 and the LCCL domain-containing protein CCP2 are expressed in female but absent in male gametocytes. The ccp2 promoter has been used in combination with the male-specific promoter of the dynein heavy chain (mg1) to engineer a dual colour reporter line with male- and female-specific expression of the respective FPs [14]. Similarly, a P. berghei reporter line was developed using the p28 promoter to express mRuby in combination with mNeonGreen-tagged (mNG) α-tubulin II [50]. This line expresses mNG-tagged α-tubulin II in all stages except female gametocytes, while female gametocytes specifically express mRuby. While originally used as driver for gene expression in mature gemetocytes, it became evident with time that the etramp10.3/peg4 promoter also activates transcription in oocysts, sporozoites and liver stages (Fig. 1, Table 2). As a consequence the promoter experienced a revival for the design of fluorescent reporter lines to simplify the study of insect and pre-erythrocytic stages in P. falciparum [26, 41, 47]. The orthologue of etramp10.3/peg4 in P. berghei, named upregulated in sporozoites 4 (uis4), was used to generate a reporter line driving the expression of mCherry to study sporozoite motility in vivo [51].

Of note, the promoter of the circumsporozoite protein (csp), driving very high expression levels especially in sporozoites, was used to engineer one of the first reporter lines in P. berghei [52]. More recently the csp promoter was combined with the ef1α promoter in the fluo reporter line to drive sporozoite-specific mCherry expression and constitutive GFP expression, respectively [38] (see also Fig. 1). The parasite burden in mosquitoes can be adjusted based on the determination of parasitaemia and gametocytaemia in infected mice by flow cytometry (GFP), while the strong mCherry expression in insect stages enables software-based analysis of sporozoite motility that was not possible when using ef1α driven reporter lines. Although some promoters presented above (e.g. uis4 and etramp10.3/peg4) display transcriptional activity in liver stages, they are not exclusively expressed in this stage. In contrast the liver-specific protein 2 (lisp2) 5’UTR drives GFP expression only in P. berghei late liver stages [22]. Of note, all lines presented here display cytoplasmic localization of their respective expressed FP, and have been generated by fluorescence cassette insertion in classical genomic loci used for ectopic gene expression (Pb: 230p and c-/d-rrna; Pf: 230p, Pfs47, cg6 and lisp1) or in intergenic loci (Pb: SIL6, SIL12 and 5’UTR of CSP; Pf: 3’UTR of cg6). They can thus be used as standards for fluorescence based applications. All discussed P. falciparum and P. berghei reporter lines are listed in Table 1 and Table 2, respectively, according to their expression profile as in Fig. 1. Transgenic P. berghei, Plasmodium yoelii or Plasmodium chabaudi lines with different genetic modifications or reporter cassettes in non-classical genomic loci can be found in the rodent malaria database [53].

FPs as sensors

Beside visualization of cells, organelles and proteins, genetically encoded FPs can also be turned into versatile biosensors to measure a wide variety of physiological parameters, detect small molecules or protein/protein interactions in intact cells and specific cellular compartments [54] (Fig. 2D). This provides a key improvement compared to disruptive biochemical methods and to in vivo staining methods using fluorescent probes that cannot achieve subcellular resolution. FP sensors are divided into intensity-based and ratiometric biosensors, each having its advantages and pitfalls. In intensiometric FPs (Fig. 2A), the fluorescence intensity of a single peak increases or decreases in response to a given stimulus. Hence, these probes are sensitive to their own concentration and highly dependent on the imaging conditions (cell thickness, illumination, photobleaching), and are therefore more suited to measure changes rather than absolute parameters. On the other hand, their monochromy is an advantage for multiplexing. In ratiometric FPs (Fig. 2B), two excitation or emission peaks react differently to the same stimulus and thus information is inferred from the intensity ratio rather than intensity alone. In this group we find both dual-excitation/emission FPs and FRET-based systems (Fig. 2C). FRET, standing for Förster resonance energy transfer, is a mechanism by which energy is transferred between two fluorophores in a proximity-dependent manner that can be achieved either through rearrangement of the sensor carrying both FPs in the presence of a specific stimulus, or through the close interaction of two bait proteins, each fused to one FP, thus bringing both FPs in close proximity. Although the change of fluorescence intensity tends to be smaller for FRET sensors than for single FP sensors, FRET sensors are easier to develop and thus cover a larger range of stimuli. Of note, intensiometric sensors can be turned into ratiometric probes when fused to other FPs that are insensitive to the same stimulus. As compared to intensiometric sensors, ratiometric ones are easier to calibrate and more robust since photobleaching and probe concentration do not affect the measurement. However, these sensors require a combination of two excitation/emission filters and often present relatively small dynamic ranges.

Fig. 2
figure 2

Fluorescent protein biosensors. A–C. The mode of action of three redox biosensors as well as their fluorescence spectra are shown as examples. A rxYFP is an intensiometric biosensor with a single excitation and emission peak. It was generated by introducing two cysteines in β-strands 7 and 11 (N149C, S202C) of YFP. rxYFP fluorescence decreases when a disulfide bridge forms between the two cysteines under oxidizing conditions. B roGFP2 is a ratiometric probe that was generated similarly as rxYFP. While the reduced form of roGFP2 has a single excitation peak at 488 nm, the oxidized form has two, at 405 and 488 nm. Ratio measurement provides a readout of the parameter of interest. C ECFP-RL7-EYFP is a ratiometric FRET sensor where ECFP and EYFP have been coupled by a small linker carrying 4 cysteines. Only ECFP is excited at 434 nm. Under reducing conditions, only ECFP emits fluorescence at 477 nm. Under oxidizing conditions, two disulfide bridges form in the linker, bringing both FPs in close proximity and allowing energy transfer from ECFP to EYFP, thus shifting the emission peak to 527 nm. D A non-exhaustive list of FP biosensors according to the physiological parameter they measure. The FPs constituting these sensors and the sensor type are indicated. Additional FP biosensors for small molecules and protein activity can be found at https://www.addgene.org/fluorescent-proteins/biosensors/. a already expressed in Plasmodium; b YFP-based sensors are especially sensitive to pH and must be used in parallel with a pH control probe sharing similar pKa and properties when employed to measure parameters other than pH

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Beside choosing the probe colour and between intensiometric and ratiometric probes for a given stimulus, three additional criteria need to be taken into account to select the most suitable sensor: (1) its sensitivity to the stimulus and (2) to other unrelated physiological parameters, and (3) its dynamic range. For instance, Peredox probes, measuring NAD + /NADH, are highly sensitive to NADH and thus, cannot be used in the mitochondrial matrix where the NADH concentration is high, hindering detection of small changes. Similarly, redox sensitive probes will only be able to measure redox potentials and detect changes if the redox potential of the cellular compartment where they are expressed is in the range of potentials that can be surveyed by the probes. As an example, a probe that is sensitive to the ratio of the reduced to oxidized forms of glutathione which maintains the redox state of the thiol groups in a cell, is fully oxidized in the endoplasmic reticulum lumen, and thus cannot be used there, while it is fully reduced in the cytoplasm and mitochondria where glutathione redox potentials are close to the lower limit of roGFP2, thus enabling detection of oxidation events. In addition, some probes may be sensitive to other unrelated parameters that can affect the reading. This is for instance the case for all YFP-based probes that are highly sensitive to pH changes. Consequently, biosensors like HyPers and Sonar that are responsive to H2O2 and NAD + /NADH, respectively, are used in parallel with SypHer that has a similar pKa but is unresponsive to H2O2 and NAD + /NADH, and can thus serve as a pH control. The fluorescence intensity of the probe and pH control should be calibrated to define a pH range where they behave similarly [55]. Ideally, a control probe based on the same FP as the sensor but insensitive to the studied stimulus should be used as reference for all unrelated environmental effects. Importantly, a weak expression, a low signal-to-noise ratio or a small dynamic range would also limit the use of the biosensor, especially in vivo, where autofluorescence is high (e.g. in vertebrate liver, mosquito tissues and iRBCs). Thus, these parameters must be evaluated in the transfected parasites to ensure the sensor can be used. In addition, stable integration of the biosensor in the parasite genome should be preferred as it overcomes several issues linked to episomal expression, including a variable/low proportion of parasites expressing the probe, variable probe expression levels between cells and a decreasing expression over time [55], but also potential interference of the selection drug with the studied parameters or with the probe itself [56, 57]. Indeed, should physiological changes be measured upon drug treatment, the absence of a direct effect of the drug on the biosensor must first be ascertained.

Discoveries in Plasmodium using biosensors

Biosensors have proven useful to measure different physiological parameters in P. falciparum and to characterize the effect of anti-malarials. Using intensiometric EGFP and a quantitative flow cytometry assay, ratiometric pHluorin and/or SypHer, the pH of the digestive vacuole was estimated to be between 5 and 5.5, while that of the cytoplasm, the apicoplast and inside the mitochondrion is close to neutral [55, 57,58,59]. Of note, the accumulation of chloroquine into the digestive vacuole depends on the protonation of the haem-binding anti-malarial drug within the food vacuole [60] which led to the hypothesis that changes in the pH of the organelle could contribute to the resistance phenotype of some strains. However, neither EGFP [59] nor pHluorin [58] detected differences in the pH of the digestive vacuole between resistant and sensitive strains. Interestingly, haem quantification using the CH49Y FRET sensor demonstrated that the amount of free haem remains relatively low and tightly regulated in the parasite cytoplasm, even during extensive haemoglobin digestion at the trophozoite stage, but increases upon chloroquine treatment, likely generating oxidative stress [61]. Both hGrx1-roGFP2 and sfroGFP2, presenting a brighter signal and thus more adapted to measure redox variations across asexual stages, including merozoites, have been used to measure the redox potential of glutathione in the cytoplasm (− 300 mV), the apicoplast (− 330 mV) and mitochondria (− 270 mV) [56, 62, 63]. They are suitable to detect nitrosative and oxidative stress in the parasite [62] and can be used for single cell imaging and plate reader assays [56]. Notably, most anti-malarial drugs do not interact directly with hGrx1-roGFP2 and sfroGFP2 [56, 57, 62], underlying their utility to explore drug-induced changes in the redox milieu. Multiple drugs have a pro-oxidant effect on the cytosolic pool of glutathione, including quinolones and artemisinin [56, 62], while the mitochondrial glutathione pool remains unaffected upon treatment with these drugs [57], indicating both pools are relatively independent. The pro-oxidant effect is further supported by an increase in H2O2 levels detected by a roGFP2-Orp1 probe in parasites treated with these drugs [55]. Using the Yellow Cameleon Nano FRET sensor (YC-nano), Ca2+ levels were shown to be low in trophozoites (30 nM), but high in other stages (> 300 mM), and exposure to artemisinin did not lead to any changes in Ca2+ concentrations in the cytosol. However, these experiments were performed using the Yellow Cameleon Nano FRET sensor, hence subtle changes in the Ca2+ concentration might not have been detected [64]. Of note, GcaMP3 was used to evaluate the dynamics of the parasites Ca2+ stores [65]. Finally, FRET has also recently been used to follow interactions between the nutrient channel proteins CLAG3 and RopH2 that were fused to two GFP derivatives, mCerulan and mVenus, respectively [66]. Although not yet applied in Plasmodium, split-FPs and Bioluminescence Resonance Energy Transfer (BRET) might provide alternatives to FRET to monitor proximity in live cells while increasing the fluorescence signal or limiting autofluorescence, respectively. Indeed, in BRET, the energy is transferred from a donor luciferase to an acceptor FP and thus, no excitation light is required. It is worth mentioning that the effect of BRET can also be undesirable if FP and luciferase are fused but fluorescence and bioluminescence have different uses, e.g. for FP based cell sorting by flow cytometry and luciferase based luminometric measurement of the parasite burden in vivo. In this case the bioluminescence might be quenched, possibly reducing intensity in luminometric measurements. To avoid BRET in such experimental settings, it is important to consider that the wavelength of the emitted bioluminescence does not overlap with the excitation wavelength of the fused FP.

FPs beyond GFP and DsRed

With the continuous discovery of new FPs and improvement of existing FP scaffolds, the available collection of genetically encoded fluorescent reporters has reached a dimension that is difficult to survey. So far (March 2024), 1058 proteins are listed in the FP database that is probably not exhaustive [67]. This wide variety of available FPs, including many method-specific fluorescent reporters, can make choosing an optimal FP difficult. In addition, the genetic modification of Plasmodium requires significantly more time and effort than the transfection of e.g. mammalian cells, which likely explains why studies on Plasmodium still often rely on variants of GFP and dsRed that have proven reliable over many years. These prototypic FPs and their derivatives, mEmerald, mVenus, mTurquoise and mCherry, perform well for most applications [68,69,70,71]. Nevertheless, FP scaffolds that outperform GFP or DsRed have been discovered or engineered. A recent example of a red FP with significantly improved quantum yield and brightness compared to mCherry is mScarlet [72]. mScarlet was developed based on an in silico scaffold that combined sequences from different known RFPs, followed by several rounds of mutagenesis-based optimization. By starting mutagenesis with an artificially designed scaffold, the structure could be adapted to eliminate areas favouring dimerization, making mScarlet a true monomeric FP [72]. Due to its excellent properties, mScarlet has already been applied as a reporter for protein export in P. falciparum infected red blood cells [73] and as a marker for successful transgenesis in P. berghei [74]. mNeonGreen (mNG), emitting light in the green/yellow spectrum, is three times brighter than EGFP and matures significantly faster while similar in terms of size and quantum yield, making it therefore an excellent alternative to GFPs and YFPs. Of note, mNG has already been used in P. berghei for C-terminal tagging of the myosin A tail domain interacting protein (MTIP) and α-tubulin II [50, 75], and as a stage-specific fluorescent reporter [50]. While originating from different scaffolds, mScarlet, mNG as well as GFP, dsRed and their derivatives have in common that they possess an intrinsically encoded chromophore. This is not always the case as many FPs rely on cofactors to be functional. Since the cofactor forms the chromophore, many cofactor-dependent FPs have significantly smaller sizes (12–18 kDa) compared to prototypic FPs (~ 25 kDa) [76]. Biliverdin-dependent FPs constitute a large family [77,78,79,80,81,82], most of them with an emission and excitation maximum in the near-infrared (NIR-FPs) which is not reached by prototypical FPs. Therefore, NIR FPs complement the existing colour palette of BFPs, GFPs, YFPs and RFPs. A promising NIR FP is the recently described miRFP670nano, which is with a molecular weight of 17.1 kDa, the smallest NIR-FP known to date and even allows inter-domain protein tagging [82]. The only known bilirubin-dependent FP, UnaG, was discovered in the Japanese eel “Unagi”, [83]. UnaG combines a small size (15.6 kDa) with excitation/emission properties similar to YFPs while its chromophore maturation does not require oxygen. Obstacles in the use of miRFP670nano and UnaG rely in their dependency on their cofactors biliverdin and bilirubin, respectively. The level of both cofactors inside Plasmodium infected red blood cells is low [84] which suggests they may need cofactor supplementation when expressed in blood stages [85]. Therefore, the use of UnaG and miRFP670nano as well as FPs with similar properties will likely remain restricted to niche applications in Plasmodium, like deep tissue imaging of sporozoites and liver stages (NIR-FPs) and interdomain tagging approaches to study protein processing. In contrast, mNG and mScarlet, that can be used in a similar way to GFP and DsRed variants, have a much broader range of applications. mNG differs from GFP only in its emission spectrum, which is shifted to yellow, thus changing the overlap with other fluorophores. One difference of mScarlet from other RFPs is its long maturation time, which probably makes it unsuitable for the detection of rapid transcriptional changes in gene expression as observed in stage transitions during Plasmodium development.

Conclusions

While genetically encoded fluorescent reporters have become an indispensable tool for research in Plasmodium most work is still based on a few classical FPs. The historical difficulties in generating transgenic P. falciparum have restricted the use of FPs and the development of genetic tools which may explain the lack of strong promoters and intergenic integration sites to expand the toolbox of fluorescent P. falciparum reporter lines. The use of Plasmodium artificial chromosomes (see "List of abbreviations"), that are centromere-containing plasmids stably inherited even in the absence of drug pressure [86], could potentially provide and elegant solution for the stable expression of ectopic transgenes without altering the parasite genome. Nevertheless, they have hardly been used so far and have yet to prove their usefulness. Two major breakthroughs in the field are the adaptation of the CRISPR/Cas9 system to Plasmodium and the development of a selection linked integration methodology (see "List of abbreviations") which have opened up a new repertory of possible genetic modifications, notably in P. falciparum [87, 88]. Therefore, it can be expected to see a dramatic increase in sophisticated experimental genetic tools in malariology within the next years. This review aims to offer valuable insights into the application of FPs in Plasmodium and to encourage the updating of the community collection of plasmids to incorporate the latest generation of FPs.

List of abbreviations

CRISPR/Cas9 System: Nuclease (Cas9)-mediated bacterial anti-phage defense system called Clustered Regularly Interspaced Palindromic Repeats (CRISPR) which can be exploited to mediate genetic changes by providing artificial guide RNAs defining the cutting site for the Cas9 nuclease, notably in a double-stranded DNA genome

Dihydrofolate reductase and dihydrofolate reductase-thymidylate synthase (DHFR/DHFR-TS): The dihydrofolate reductase and the bifunctional enzyme dihydrofolate reductase-thymidylate synthase convert dihydrofolate into tetrahydrofolate which serves as a cofactor in the synthesis of purines and certain amino acids; the essentiality of tetrahydrofolate makes Plasmodium dihydrofolate reductase an ideal target for drug selection using pyrimethamine (see below) or WR99210.

Episome: Extra-chromosomal genetic material which replicates autonomously in the parasite. Episomes can be plasmids although the mechanism by which Plasmodium maintains and replicates bacterial DNA remains unknown. Selection of transfected parasites carrying episomes requires a selectable marker, and episomes are only retained upon drug pressure. The number of episomes per parasite varies extensively.

Plasmodium artificial chromosomes (PACs): are based on a plasmid named pFCEN containing an artificial P. falciparum centromere, that allows transfected parasites to retain the plasmid as a single copy (like a chromosome), even in the absence of drug pressure, which is not the case for episomes (see above).

Pyrimethamine: a drug which competes with dihydrofolate at the active site of dihydrofolate reductases and, as a consequence, inhibits its enzymatic activity; human dihydrofolate reductase as well as mutated variants of protozoan dihydrofolate reductases, and dihydrofolate reductase-thymidylate synthases are resistant to inhibition and can be used as positive selection markers during transgenesis.

Selection-linked integration (SLI): A method to rapidly select for parasite transformants in P. falciparum using plasmids that contain two positive selection markers. The first marker selects for uptake and episomal inheritance of transfected DNA, while the second marker is only expressed upon genomic integration. The formation of the second resistance is achieved by fusing the selection marker with the open reading frame of the protein of interest via a self-cutting peptide (e.g. T2A). The enrichment of episome-containing parasites significantly increases the probability of finding parasites that have integrated the plasmid into the genome when selecting for the second selection marker in a time-delayed manner

Availability of data and materials

Not applicable.

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Acknowledgements

We thank Dr. Eric Marois and Dr. Mirko Singer for critical reading of the manuscript. We also thank Dr. Markus Ganter for providing the template for the life cycle displayed in Fig. 1 and all reviewers for their insightful comments. We apologize to all authors whose works we could not cite due to journal restrictions.

Funding

Open Access funding enabled and organized by Projekt DEAL. This work was supported by the French Centre National de la Recherche Scientifique, the Institut National de la Santé et de la Recherche Médicale, the Universities of Strasbourg & Saarland (bachelor fellowship to PJT), the Laboratoire d’Excellence (LabEx) ParaFrap (grant LabEx ParaFrap ANR-11-LABX-0024) and the ANR PlasmoPrim (grant ANR-17-CE15-0013). DK received funding through a DFG postdoctoral fellowship (KL 3251/1-1).

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Authors and Affiliations

  1. Inserm, CNRS, Université de Strasbourg, UPR9022/U1257, Mosquito Immune Responses (MIR), IBMC, F-67000, Strasbourg, France

    Pia J. Thiele, Raquel Mela-Lopez, Stéphanie A. Blandin & Dennis Klug

  2. Institute of Physiology and Pathophysiology, Department of Molecular Cell Physiology, Philipps University Marburg, 35037, Marburg, Germany

    Dennis Klug

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  1. Pia J. Thiele
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  2. Raquel Mela-Lopez
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DK, PT and SB conceptualised the review and wrote the original draft. RML and SB contributed both chapters on the use of fluorescent probes as sensors. All authors read, edited and approved the final manuscript.

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Correspondence to Dennis Klug.

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Thiele, P.J., Mela-Lopez, R., Blandin, S.A. et al. Let it glow: genetically encoded fluorescent reporters in Plasmodium. Malar J 23, 114 (2024). https://doi.org/10.1186/s12936-024-04936-9

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Malaria Journal

ISSN: 1475-2875

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