# Transfection of Platyhelminthes

Authors: Bárbara Moguel; Raúl J. Bobes; Julio C. Carrero; Juan P. Laclette
Journal: BioMed Research International
 (2015)

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## Abstract

Flatworms are one of the most diverse groups within Lophotrochozoa with more than 20,000 known species, distributed worldwide in different ecosystems, from the free-living organisms in the seas and lakes to highly specialized parasites living in a variety of hosts, including humans. Several infections caused by flatworms are considered major neglected diseases affecting countries in the Americas, Asia, and Africa. For several decades, a particular interest on free-living flatworms was due to their ability to regenerate considerable portions of the body, implying the presence of germ cells that could be important for medicine. The relevance of reverse genetics for this group is clear; understanding the phenotypic characteristics of specific genes will shed light on developmental traits of free-living and parasite worms. The genetic manipulation of flatworms will allow learning more about the mechanisms for tissue regeneration, designing new and more effective anthelmintic drugs, and explaining the host-parasite molecular crosstalk so far partially inaccessible for experimentation. In this review, availability of transfection techniques is analyzed across flatworms, from the initial transient achievements to the stable manipulations now developed for free-living and parasite species.


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## Body

## 1. Platyhelminth Transfection Studies

The phylum Platyhelminthes or flatworms represent one of the most diverse groups within Lophotrochozoa with about 20,000 species distributed worldwide including free-living and parasitic organism classified into 17 major groups [1, 2]. All these acoelomate worms have bilateral symmetry; they are hermaphrodite with some exceptions and have a simple centralized nervous system and a mesodermal germ layer [3, 4]. Flatworms are characterized by a high degree of morphological diversity and reproduction modes (Table 1). The phenomenon of asexual reproduction that is uncommon in the animal kingdom occurs in all major groups of flatworms. This supports the presence of a population of totipotent stem cells called “neoblasts” in free-living worms and “germ or germinal cells” on flukes and tapeworms [4]. Several human infections caused by flatworms are considered major neglected tropical diseases (NTDs) by the World Health Organization: cysticercosis, schistosomiasis, fascioliasis, paragonimiasis, and echinococcosis [5].Table 1
Main characteristics of the groups where genetic transfection has been achieved
*.
Group
Biologic interactions
Adult body
Life cycle
Example of genus
Tricladida
Mostly free-living
Nonsegmented
Simple
Dugesia, Schmidtea
Trematoda
Endoparasites of invertebrates and vertebrates
Nonsegmented
Complex
Fasciola, Schistosoma
Cestoda
Endoparasites of vertebrates
Segmented
Complex
Taenia, EchinococcusDeveloping techniques to manipulate flatworms is a growing topic in contemporary research as judged by the number of reports published during the last decade [6]. Maintenance of parasite species under laboratory conditions has been challenging and genetic manipulation is still difficult [7]. However, since the 90s, attempts have been made to identify and characterize the regions controlling the expression of genes in several species of flatworms [8]. Due to the lack of a good expression system for heterologous genes in these organisms, several mammalian cell lines have been employed as transfection targets to identify functional promoters in flatworms [9, 10]. In this regard, the recently described genomes for several of these organisms, including the free-living planarianSchmidtea Mediterranean [11], and the parasitesSchistosoma mansoni,S. japonicum [12, 13],Taenia solium [14, 15],Echinococcus granulosus, andE. multilocularis [15] represent a considerable advantage. Those genome projects allowed us to identify orthologous genes of each species and group and their functional promoters as well as to carry outin silico metagenomic studies. Transfection studies for each of the three groups of Platyhelminthes done so far are described in this short review.


### 1.1. Tricladida

Planarians have the capacity of regenerating complete worms from a small fragment of their bodies [16]. In 1981, Baguñà described a group of cells conferring these regenerative properties as “neoblasts” [16–18]. In order to understand the basis of tissue regeneration in these flatworms, several studies were conducted [18], which could represent a valuable contribution to human regenerative medicine [16] as well as to the establishment of stable germ cell lines useful in transfection studies [19]. However, it was not until the advent of the molecular biology and genetic tools that further investigation in this phenomenon was possible. Thus, in 1999 the Dglvs gene (Dugesia VASA-like) was reported as the first gene expressed in neoblasts [20] and, almost simultaneously, a successful application of RNA interference (RNAi) was reported [21]. Since then, several related neoblast genes have been described and strategies for transient transfections have been developed for Tricladida [16]. The most used method for introducing exogenous genes in the different stages of these organisms is microinjection, which is also frequently used for silencing genes such as Djpum, nanos, ß-catenin, ndk, DjFGFR1, and DjFGFR2 [16, 18, 22, 23]. This method, although highly efficient in adult flatworms, was very invasive for early developmental stages. More recently, a novel method for introducing exogenous materials into developing planarian embryos by nanosecond exposure of eggs to pulsed laser has been reported. This represents the first report of planarian embryos being genetically modified without compromising their normal development [17]. However, availability of suitable vectors for stable transfections is required to allow incorporation of exogenous genetic material into the genome of these organisms. For example, in the case of planarians three mobile elements (mariner, Hermes, and PiggyBac) have been introduced using the green fluorescent protein (EGFP: enhanced green fluorescent protein) as reporter gene, using microinjection followed by electroporation to transfect the parenchymal cells of adult flatworms [19]. Until now, the three transposons have shown good efficiency of integration into the genome in neoblast cells. PiggyBac and Hermes appear to be quite stable showing a good expression after eight months of transfection [19].


## 1.1. Tricladida

Planarians have the capacity of regenerating complete worms from a small fragment of their bodies [16]. In 1981, Baguñà described a group of cells conferring these regenerative properties as “neoblasts” [16–18]. In order to understand the basis of tissue regeneration in these flatworms, several studies were conducted [18], which could represent a valuable contribution to human regenerative medicine [16] as well as to the establishment of stable germ cell lines useful in transfection studies [19]. However, it was not until the advent of the molecular biology and genetic tools that further investigation in this phenomenon was possible. Thus, in 1999 the Dglvs gene (Dugesia VASA-like) was reported as the first gene expressed in neoblasts [20] and, almost simultaneously, a successful application of RNA interference (RNAi) was reported [21]. Since then, several related neoblast genes have been described and strategies for transient transfections have been developed for Tricladida [16]. The most used method for introducing exogenous genes in the different stages of these organisms is microinjection, which is also frequently used for silencing genes such as Djpum, nanos, ß-catenin, ndk, DjFGFR1, and DjFGFR2 [16, 18, 22, 23]. This method, although highly efficient in adult flatworms, was very invasive for early developmental stages. More recently, a novel method for introducing exogenous materials into developing planarian embryos by nanosecond exposure of eggs to pulsed laser has been reported. This represents the first report of planarian embryos being genetically modified without compromising their normal development [17]. However, availability of suitable vectors for stable transfections is required to allow incorporation of exogenous genetic material into the genome of these organisms. For example, in the case of planarians three mobile elements (mariner, Hermes, and PiggyBac) have been introduced using the green fluorescent protein (EGFP: enhanced green fluorescent protein) as reporter gene, using microinjection followed by electroporation to transfect the parenchymal cells of adult flatworms [19]. Until now, the three transposons have shown good efficiency of integration into the genome in neoblast cells. PiggyBac and Hermes appear to be quite stable showing a good expression after eight months of transfection [19].


## 2. Digenean Trematodes

Trematode infections reach high prevalence in developing countries [5, 24]. The helminth infection with the largest global prevalence is schistosomiasis with 207 million cases worldwide, mainly caused by three species of blood flukes:S. haematobium,S. mansoni, andS. japonicum. In the case of trematodes, extensive studies on vaccines, drug development, and diagnostic methods are available [24]. Moreover, the complete genomes ofS. mansoni andS. japonicum have been elucidated [12, 13]. Attempts of identifying genes and introducing heterologous genetic material have been carried out for more than a decade. New technologies have enabled success to identify, to silence, and to carry out transient transfections of several genes. Stable transfections have been achieved, allowing the approach to questions about the involvement of specific genes in disease pathogenesis or the identification of new target candidates for drug treatment [24]. Several reviews are available where the genomic history of schistosomes, including advances on transfection, is well organized [8, 10, 25–29]. Table 2 summarizes the progress in the transfection ofS. mansoni andS. japonicum.Table 2
Transfection of heterologous genes in Schistosomes.
Species
Agent and method
Promoter
Reportergene
Life stage transfected
Transfection type
References
S. mansoni
RNA and plasmid by particle bombardment
Spliced Leader
Luciferase
Adult worm
Transient
[34]
Plasmid by particle bombardment
Hsp70
GFP
Adult worm and sporocysts
Transient
[35]
Plasmid by particle bombardment
ER60
GFP
Female miracidia with sporocysts
Transient
[36]
Plasmid by particle bombardment
SmCNA
GFP
Adult worm
Transient
[37]
Plasmid by particle bombardment
ER60
GFP
Adult worm
Transient
[38]
Plasmid by particle bombardment
Hsp70
EGFP
Miracidia
Transient
[39]
RNA by electroporation
—
Luciferase
Schistosomula
Transient
[40]
RNA by particle bombardment and electroporation
—
Luciferase
Sporocysts, miracidia, and adult worm
Transient
[41]
VSVG-pseudo MMLV plasmid by cation polybrene
SL and hsp70
EGFP and Luciferase
Schistosomula
Transient
[42]
Electroporation
SmACT1.1
Luciferase
Schistosomula
Transient
[43]
PiggyBac by electroporation
Actin and HSP70
Luciferase
Schistosomula
Stable
[44]
VSVG-pseudo MMLV plasmid by lipofectamine
Sma-Zinc
Luciferase
Adult worm and schistosomula
Stable
[45]
RNA and VSVG-pseudo MMLV by electroporation
—
CY3 and luciferase
Eggs
Stable
[46]
MLV pseudotyped plasmid by lipofectamine or polyethylenimine
MLV 5′, Pol II,vasa-like, Actin, Pol III U6
Luciferase and EGFP
Schistosomula, eggs, and adult worms
Stable
[47]
S. japonicum
Plasmid by electroporation
CMV
EGFP and luciferase
Schistosomula and adult worm
Transient
[48]
VSVG-pseudo pantropic retrovirus plasmid by cation polybrene
LTR
hTERT
Schistosomula
Stable
[49]
SL: splice leader, hsp70: heat-shock protein 70, ER60: endoplasmic reticulum 60, SmCNA:Schistosoma mansoni calcineurin 1, CMV: cytomegalovirus, SmAct 1: Schistosoma mansoni actin 1, Sma-Zinc: Schistosoma mansoni Zinc finger protein, hTERT: human telomerase reverse transcriptase, VSVG: vesicular stomatitis virus glycoprotein, MMLV: Moloney murine leukemia retroviral, and LTR: retrovirus long terminal repeat.Other trematodes causing infections of high global prevalence (>40 million cases) [24], such asClonorchis sinensis (liver fluke),Opisthorchis viverrini (liver fluke),Paragonimus spp (lung fluke),Fasciolopsis buski (intestinal fluke), andFasciola hepatica (intestinal fluke), have not been successfully transfected; successful methodologies developed forS. mansoni could be adapted for these trematodes [27]. However, the promoter region of cathepsin 1 fromF. hepatica has been characterized through transient transfection of mammalian Vero cells [30]. Another case is theParagonimus westermani retrotransposon sequences belonging to three LTR (long terminal retrotransposons) retrotransposon families [31]. Two of these retrotransposon sequences appeared to maintain their mobile activities as suggested by the presence of mRNA transcripts [31]. The ability to integrate into the flatworm genome makes transposons and retrotransposons excellent candidates to develop stable transfections [32].Three methods have been exploited for nucleic acid delivery into schistosomes [28]: biolistic (particle bombardment/gene gun), electroporation, and infectious retroviral vectors (Table 2). Electroporation has been considered as the most efficient method for transfection of sporocysts and schistosomules. However, biolistic has also been successfully used on miracidia and adults [33]. The choice of a delivery method depends on the organism and the life cycle stage under study. Moreover, experiences in schistosomes can also help to choose and adapt one transfection method on related organisms.An application of transient transfection methodologies is the silencing of specific genes through RNAi, involving studies on worm viability, development, tegument physiology, egg development, signaling pathways, and drug discovery. Efficacy of RNAi can be influenced by the method of delivery: the more often used in schistosomes are soaking and electroporation [8] and the most frequently used RNAi in schistosomes is dsRNA (long double stranded), followed by siRNA (small interfering) [29]. The properties of each RNAi have been important to define their use; for example, it has been suggested that siRNA accumulates faster in certain tissues [50], whereas dsRNA is more stable to RNAse digestion [51]. In addition, dsRNA experiments are cheaper than the siRNAs counterpart [29, 51]; however, siRNAs can be more efficient inhibitors when multiple sequence oligonucleotides are used against the same target [8, 28, 29, 51, 52]. Developments of RNA silencing in schistosomes and other trematodes have accumulated during the last decade (Table 3).Table 3
RNA silencing in trematode parasites.
Species
Rnai
Target gene
Life stage target
Silencing efficacy
References
S. mansoni
dsRNA
SGTP1 and GAPDH
Miracidia and sporocyst
70–80% (t); 40% (p)
[55]
dsRNA
SmCB1
Schistosomula
10-fold (t)
[56]
dsRNA
SmCB1 and SmCB31
Cercariae and adult worms
80% (t)
[57]
dsRNA and siRNA
SmAP
Cercariae and adult worms
>90% (t); >70% (p)
[58]
siRNA
SmRPNII/POH1
Schistosomula
80% (t)
[59]
dsRNA
Cathepsin D
Schistosomula
100% (t)
[60]
siRNA
HGPRTase
Cercariae
↓ 27% parasite load, 65%  (t)
[53]
dsRNA
SmLAP 1 and SmLAP2
Eggs
↓ 80% hatching
[61]
dsRNA
32 genes (antioxidants, transcription factors, cellular signaling, and metabolic enzymes)
Miracidia
Mobility, growth, and viability affected
[62]
siRNA
SmAP
Adult worms
80% (t)
[63]
dsRNA
SmTK4
Adult worms
17–63% (p)
[64]
dsRNA
SmAQP
Adult worms
90–95% (t)
[65]
dsRNA
SmPAL
Adult worms
Inconsistent results
[66]
dsRNA
SmGTP-1 and SmGTP-4
Adult worms
In vivo: SmGTP-1 55% (t), SmGTP-4 85% (t);
In vitro: SmGTP-1, 70% (t), SmGTP-4, 90% (t)
[67]
dsRNA
11 genes
Schistosomula
40–75% (t)
[68]
dsRNA
SmCa1 and SmCa2
Miracidia
35% (p)
[69]
sh-RNA
Luciferase
Schistosomula
47.5% (p)
[70]
dsRNA
SmAP
Adult worms
95% (t)
[71]
dsRNA
Sm-NPP-1
Schistosomula and adult worms
55% (t)
[72]
siRNA
SmCD59
Schistosomula
60% (t)
[73]
dsRNA
SmCaMK2, SmJNK, SmERK1, SmERK2, and SmRas
Schistosomula
SmERK1 92% (t), SmERK2 56% (t), SmRas 42% (t)
[74]
dsRNA
SmACC-1 and SmACC-2
Schistosomula
SmACC-1 60% (t),SmACC-2 90% (t)
[75]
siRNA
SmAP, SmNPP-5, and SmATPDase1
Schistosomula and Adult worms
SmAP 90% (t),SmNPP-5 >90% (t), SmATPDase1 80% (t)
[54]
siRNA
Sm5HTR
Schistosomula and adult worms
Larvae: 100% (t) and↓ 80% motility; adult male and female: 90% (t) and ↓ 60% motility, 80% (t) and ↓ 50% motility, respectively
[76]
S. japonicum
dsRNA
SjGCP
Adult worms
75% (t)
[77]
siRNA
Mago Nashi
Schistosomula
66–81% (t)
[78]
dsRNA
Prxs 1 and Prxs 2
Schistosomula and adult worms
~20% (t)
[79]
dsRNA
(SHSP) Sjp40
Adult worms
80% (t)
[80]
siRNA
SjAR (SiRNA1 and SiRNA2)
Schistosomula
48% (t) and 73% (t)
[81]
S. haematobium
siRNA and dsRNA
Luciferase and Sh-tsp-2
Eggs, schistosomula, and adult worms
>75% (p) for both
[82]
F. hepatica
dsRNA
FheCL and FheCB
Metacercariae
FheCL1: 80% (t)
[83]
dsRNA
FhLAP
Young larvae
>90% (p)
[84]
SGTP: facilitated diffusion glucose transporter, GAPDH: glyceraldehyde-3-phosphato-dehydrogenase, SmCB:Schistosoma mansoni cathepsin B, SmAP: Schistosoma mansoni alkaline phosphatase, SmRPNII/POH1: Schistosoma mansoni proteasome subunit, HGPRTase: hypoxanthine-guanine phosphoribosyl transferase, SmLAP:Schistosoma mansoni leucine aminopeptidase, SmTK4: Schistosoma mansoni SYK kinase, SmAQP: Schistosoma mansoni aquaporin gene, SmPAL: Schistosoma mansoni peptidylglycine alpha-amidating lyase, SmGTP: Schistosoma mansoni glucose transporter, SmCa: Schistosoma mansoni calmodulin sensing, Sm-NPP-1: Schistosoma mansoni neuropeptide precursor 1, SmCaMK: Schistosoma mansonicalmodulin-binding kinase, SmJNK: Schistosoma mansoni C-JUN-N-terminal kinase, SmERK: Schistosoma mansoni extracellular signal-regulated kinase, SmRAS: small GTPase superfamily, SmACC: Schistosoma mansoni acetylcholine-gated chloride channels, SmHTR: Schistosoma mansoni serotonin-activated G protein-coupled R, SjGCP: Schistosoma japonicum gynecophoral canal, Prxs: peroxiredoxin, Sjp40: Schistosoma japonicum short heat-shock protein, SjAR: Schistosoma japonicumaldose reductase, FheCL and FheCB: Fasciola hepatica cathepsin L and B, FhLAP: Fasciola hepatica leucine aminopeptidase, and sh-tsp-2: transcription of tetraspanin 2.  (↓): knockdown; (t): transcript; (p): protein.Table3 shows that although the most widely used RNAi is dsRNA gene silencing also can be efficiently achieved with siRNA [29]. The RNAi agent and the delivery method can be defined after the gene target and the stage of the parasites are selected. It is worth mentioning that initial attempts towards knocking down the expression ofS. mansoni essential genes throughin vivo administration of siRNA on infected hosts have produced encouraging results [53]. This strategy, that takes advantage of the low mRNA levels of the homologue gene in the host’s tissues (hypoxanthine-guanine phosphoribosyl transferase: HGPRTase), is restricted in the case of other essential genes [54].


## 3. Cestodes

Among cestodes the most important infections in public health are cysticercosis and hydatosis or echinococcosis, with high global prevalence in endemic countries [5, 85]. In the case of these parasites, extensive studies on immunodiagnosis, drug and vaccine development, and so forth have been carried out [85–87]. However, transfection studies on cestodes have been scarce. An important development in the manipulation of these parasites is the isolation of germinal cells lines. ForT. crassiceps it was possible to regenerate complete cysticerci from cellular clusters [88]; forE. multilocularis new metacestodes were regenerated from the germinal layer [89]; in the case ofE. granulosus, the isolation andin vitro maintenance and propagation of germinal cells have been reported [90, 91]. The most significant development in the transfection of cestode parasites was achieved onE. multilocularis using axenic cultures of metacestodes. After some time in coculture with rat hepatocytes, the germinal cells formed a laminar layer and then clustered until the regeneration of the metacestode vesicles [92]. The first attempts of a transient transfection were done by lipofection of germinal cells with a cyanofluorescent gene as a reporter under the control ofelp (encoding the ezrin-radixin-moesin- (ERM-) like protein), anE. multilocularis gene promoter [92]. Transient expression of the fluorescent protein was detected. Furthermore, these cells ofE. multilocularis were infected with the intracellular bacteriumListeria monocytogenes, demonstrating a good nucleic acid carrier system [92]. The use of an attenuated, self-destructive bacteria is exciting, as it can reach the cytosol of the host cells and induce the expression of a heterologous gene under the control of the P
acta promoter [93]. This approach could be useful for other Platyhelminthes where cell lines can be isolated and maintainedin vitro. In the case of gene silencing, an experiment in whichelp and 14-3-3 were used as target genes, employing soaking and electroporation to deliver the siRNA, showed that the protein expression of 14-3-3 andelp decreases ~22% and ~72%, respectively, on day fifteen, after transfection of the protoscoleces ofE. multilocularis [94]. Another silencing experiment was performed in the cestode of ruminantsMoniezia expansa; the aim was to silence the transcription of actin (Me-act-1) gene using dsRNA. The reduction of actin expression was detected by immunohistochemistry and western blot techniques, in addition to severe damage in the morphology of tegument [95]. These studies demonstrated that the transfection and gene silencing techniques can be successfully used in cestodes. In fact, we have achieved successful transient transfection ofT. crassiceps cysticerciin vitro by microinjection using a cytomegalovirus promoter and GFP as a reporter (submitted for publication). In addition, we are conducting assays to achieve stable transfection using PiggyBac transposon, as well as developing strategies for the introduction of dsRNA to silence target genes inT. crassiceps.Thus, the genetic manipulation of cestode parasites is currently under examination with the goal of developing reliable methodologies for stable transfection andin vitro maintenance of cell lines.


## 4. Conclusion

The new technologies for genetic manipulation and transgenesis have been used in trematode parasites, specifically inS. mansoni [29], which is a starting point for other flatworms. However, the progress in helminths and especially in cestodes has been limited by the inability to produce stable cell lines, although the recent advances inEchinococcus are encouraging. It is important to remark that the advance in Platyhelminth parasites is still limited in comparison with the protozoan parasitic organisms, where highly reproducible transfection methods, including stable transfections [9], have been available for some time. Transposons, bacteria, viruses, and constructs with sequences that allow integration of exogenous sequences into the flatworms genome have been already used, but successful experiments have been only reported forSchistosoma [10, 28, 29]. It is expected that similar gains can be achieved in other flatworms. If so, molecular helminthology will be transformed from descriptive to more functional investigations. The need to develop methods for the production andin vitro cultivation of germ cell lines for genetic manipulation is emphasized [89].



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