- Short report
- Open Access
Establishment of an in vitro chicken epithelial cell line model to investigate Eimeria tenella gamete development
Parasites & Vectors volume 11, Article number: 44 (2018)
Eimeria tenella infection leads to acute intestinal disorders responsible for important economic losses in poultry farming worldwide. The life-cycle of E. tenella is monoxenous with the chicken as the exclusive host; infection occurs in caecal epithelial cells. However, in vitro, the complete life-cycle of the parasite has only been propagated successfully in primary chicken kidney cells, which comprise undefined mixed cell populations; no cell line model has been able to consistently support the development of the sexual stages of the parasite. We therefore sought to develop a new model to study E. tenella gametogony in vitro using a recently characterised chicken cell line (CLEC-213) exhibiting an epithelial cell phenotype.
CLEC-213 were infected with sporozoites from a precocious strain or with second generation merozoites (merozoites II) from wild type strains. Sexual stages of the parasite were determined both at the gene and protein levels.
To our knowledge, we show for the first time in CLEC-213, that sporozoites from a precocious strain of E. tenella were able to develop to gametes, as verified by measuring gene expression and by using antibodies to a microgamete-specific protein (EtFOA1: flagellar outer arm protein 1) and a macrogamete-specific protein (EtGAM-56), but oocysts were not observed. However, both gametes and oocysts were observed when cells were infected with merozoites II from wild type strains, demonstrating that completion of the final steps of the parasite cycle is possible in CLEC-213 cells.
The epithelial cell line CLEC-213 constitutes a useful avian tool for studying Eimeria epithelial cell interactions and the effect of drugs on E. tenella invasion, merogony and gametogony.
Coccidiosis has a high economic impact on poultry farming worldwide . This disease is caused by species of Eimeria, a genus of obligate intracellular parasites belonging to the phylum Apicomplexa; Eimeria spp. invade and multiply in intestinal epithelial cells . Eimeria tenella is one of the most pathogenic species infecting chickens . Its life-cycle is comprised of endogenous asexual multiplication and sexual development. Asexual multiplication consists of - typically, for wild type strains - three rounds of merogony, resulting in successive generations of schizonts, containing merozoites. This step is followed by sexual development (gametogony) with the formation of microgametes (mature male gametocytes) and macrogametes (mature female gametocytes) . Each microgametocyte produces approximately 100 motile microgametes that are able to fertilise a macrogamete resulting in the formation of a zygote. The latter becomes encapsulated in a protective wall, forming an oocyst that is released from the host into the external environment. The precocious strain develops with a shortened prepatent period and presents only one round of merogony before entering gametogony. This strain is currently used for immunization as its pathogenicity is attenuated [4,5,6]. In vitro cell cultures permit limited parasite development, often with cessation of development at the first generation of merozoites (merozoites I) [7,8,9,10,11]. Macrogametes, microgametes and oocysts have only been observed in primary cultures of chick embryonic kidney cells or chicken kidney cells (PCKC), but oocyst yields remain consistently low [7, 12]. However, given that Eimeria spp. are highly host-specific , it may be possible to develop an in vitro assay based on chicken epithelial cell lines to study sexual stages of E. tenella life-cycle, host-pathogen interactions and large-scale drug screening.
In the first part of this study, we compared the ability of E. tenella to invade and develop to first generation schizonts in different cell lines. We then tested: (i) a commonly used cell line for E. tenella studies, Madin-Darby bovine kidney (MDBK) epithelial-like cells; (ii) a transimmortalized mouse intestinal epithelial cells (m-ICcl2), since the digestive tract is the site of Eimeria infection; and (iii) the chicken lung epithelial cell line (CLEC-213), cells of which are polarized, develop junctional complexes, express the cell to cell adhesion molecule, E-cadherin, and exhibit microvilli at the apical cell surface . We then reasoned that, since in the literature, there are no chicken intestinal or caecal epithelial cell lines characterised yet, a cell line obtained from the natural host of E. tenella and from epithelial tissue should be tested alongside mammalian cell lines. As we observed the presence of extracellular merozoites II only when using CLEC-213, we then determined the ability of the parasite to develop further only in this recently characterised cell line . In this avian epithelial cell model, we observed the production of macrogametes and microgametes, using specific markers EtGAM-56 and EtFOA1, respectively , thus proving the occurrence of gametogony after infection with the precocious strain and oocyst production after infection with second generation merozoites (merozoites II) of the wild type strain.
Epithelial cell lines
MDBK cells, m-ICcl2 cells and CLEC-213 cells were grown as described by Tierney et al. , Bens et al.  and Esnault et al. , respectively. Cells were plated in 24-well plates for the different assays.
Different protocols either in vitro and in vivo were applied to obtain oocysts, sporozoites, merozoites I, merozoites II and gametocytes. To obtain oocysts, 4–6 week-old outbred PA12 White Leghorn chickens were inoculated with 104 sporulated oocysts of E.tenella wild type Wisconsin strain (Wis; ), wild type recombinant strains expressing the yellow fluorescent protein (Wis-YFP), mCherry strain (INRA-mCherry) or with 106 sporulated oocysts of the precocious E. tenella Wis-F-96 strain . Recombinant strains were generated as described by Yan et al. ; see below. Chickens were sacrificed after 7 and 5 days post-infection for the wild type strains and the precocious strain, Wis-F-96, respectively. Unsporulated oocysts were collected from the caeca, then sporulated, and sporozoites were purified as described by Shirley .
Merozoites I were obtained from supernatants of infected MDBK cells at 72 h p.i. (in vitro) . Merozoites II were obtained from PA12 chickens that had been inoculated orally with 2.5 × 105 sporulated oocysts of E. tenella Wis or INRA-m-Cherry 5 days earlier, as described previously . Gametocytes were isolated from caeca of E. tenella Wis infected chicken as described previously .
Transgenic Eimeria tenella
Recombinant strains were generated using an adaptation of the protocol described by Yan et al. . The Wis strain was transfected with a plasmid expressing the yfp gene under the E. tenella mic1 promoter to allow visualization of parasites in invasion and schizont development assays. The INRA strain PAPt36  was transfected with the mCherry gene under the E. tenella actin promoter, to facilitate visualization of sexual stages of parasite development in the CLEC-213 cells, where a high background green autofluorescence interferes with detection of YFP signals as parasites developed. Wild type Wis and INRA strains were compared in vivo and did not show, in our experimental conditions with an inoculum of 5000 oocysts, any significant differences in parasite development as shown by oocyst excretion and pathogenicity (lesion scores; data not shown). Similarly, parasites expressing YFP or mCherry protein did not display any differences in parasite development as shown by oocyst excretion (data not shown). Transgenic E. tenella oocysts, sporozoites and merozoites II were obtained as described above.
In vitro parasite development assays
Invasion assays were performed as described previously . Briefly, 2 × 105 epithelial cells per well (MDBK, m-ICcl2, CLEC-213) were co-cultured on glass coverslips with 4 × 105 purified sporozoites (Wis-YFP) for 3 h at 41 °C, 5% CO2; in preliminary experiments, the infection rate was higher at 41 °C than at 37 °C in all cell lines, confirming the data described by Tierney et al. . After washing and fixing the cells with paraformaldehyde (4%; Santa Cruz Biotechnology, Dallas, TX, USA), monolayers were mounted in Vectashield mounting media with DAPI (1.5 μg/ml; Vector Laboratories, Burlingame, CA, USA). For each coverslip, a minimum of three microscope fields were observed (Zeiss Axiovert 200 microscope, Carl Zeiss, Göttingen, Germany). More than 200 cells were counted per condition using ImageJ software. The percentage of infected cells was calculated and values are reported as mean ± SD of at least four independent replicates.
Schizont development was studied by infecting 2 × 105 epithelial cells per well (MDBK, m-ICcl2, CLEC-213), cultured overnight on glass coverslips, with 4 × 105 purified sporozoites (Wis-YFP) as described above. After 3 h of co-culture, extracellular sporozoites were removed by washing and cells were kept in culture for an additional 48 h. Cells were washed, fixed and mounted. The percentage of schizonts was calculated relative to the number of infected cells. A minimum of three microscope fields were observed for each coverslip (Zeiss Axiovert 200 microscope, Carl Zeiss); more than 200 cells were counted for each condition. Values are reported as mean ± SD of at least four independent replicates.
The development of sexual stages of E. tenella was observed only in CLEC-213 cells (2 × 105 cells per well) infected with either 3 × 106 merozoites II from wild type parasites or 4 × 105 purified sporozoites from the precocious Wis-F-96 in complete cell culture medium for 3 h at 41 °C, 5% CO2. After removal of extracellular parasites, cells were cultured for an additional 2 days or 5 days for cells infected with merozoites II or sporozoites, respectively. Then, after washing, cells were fixed with paraformaldehyde (4%; Santa Cruz Biotechnology). The presence of micro and macrogametes was analyzed by specific immunostaining (described below) or by detection of mCherry signal at a wavelength of 620 nm.
Detection of microgametes and macrogametes in vitro
EtGAM-56 and EtFOA1 antigens, expressed specifically by macrogametes and microgametes, respectively, were detected after staining with specific antibodies (polyclonal rabbit anti-EtGAM-56; 1/100  and monoclonal mouse anti-FOA1 1/100; ) and the appropriate secondary antibodies (goat anti-rabbit conjugated with Alexa 594; goat anti-mouse conjugated with Alexa 594; 1/1000; Invitrogen, Eugene, OR, USA). Cell monolayers were mounted as described above and parasite stages were visualised using AxioVision Sofware (Zeiss Axiovert 200 microscope, Carl Zeiss).
In addition to detection using specific antibodies, gene expression of Etgam56 and Etfoa1 was studied in different developmental stages of E. tenella, after infection of CLEC-213 with merozoites II from wild type strains (Wis) or sporozoites from the precocious strain (Wis-F-96) to confirm the presence of microgametes and macrogametes. Cells or parasites (sporozoites, merozoites I, gametes) were lysed in RA1 lysis buffer (NucleoSpin RNA, Macherey Nagel, Düren, Germany); RNA was extracted as described in the manufacturer’s manual and suspended in nuclease-free water. The Superscript™ II First Strand Synthesis System (Invitrogen), with random hexamer primers and oligo(dT)15 primer (Promega, Madison, WI, USA), was used to synthetize cDNA. For studying the development of gametes, segments of cDNAs were amplified by qPCR (Bio-Rad Chromo4, Bio-Rad, Hercules, CA, USA) using SYBR Green master mix (Bio-Rad), specific primers to the housekeeping gene, Et18S (forward primer, 5′-CTG ATG CAT GCA ACG AGT TT-3′ and reverse primer, 5′-GAC CAG CCC CAC AAA GTA AG-3′), the microgamete-specific gene, Etfoa1 (ETH_00025255 from ToxoDB release 34, www.toxodb.org; forward primer, 5′-TCT CGC ATT CCT CAC AGA TG-3′ and reverse primer, 5′-ATT TCG CCT TGT GGA TGA AC-3′) and the macrogamete-specific gene, Etgam56 (ETH_00007320 from ToxoDB release 34; forward primer, 5′-AGT GGC TGG AGA ACT TCG TG-3′ and reverse primer, 5′-ATG CGG TTC GTG ATC ATG TC-3′, Eurogentec, Seraing, Belgium). The qPCR was performed using the following protocol: 95 °C for 3 min and 40 cycles at 95 °C for 10 s and 60 °C for 30 s followed by 65 °C for 30 s. The melting curve was generated at 65 °C for 5 s followed by gradual heating (0.5 °C/s) to 95 °C. For each experiment, qPCR were performed in triplicate and expression of EtGam56 and Etfoa1 was normalised to Ct values obtained for E. tenella small ribosomal subunit 18S RNA using the formula: 2-(Ctgene – CtEt18S). Gene expression values are expressed as mean ± SD of at least two independent biological and three technical replicates.
Data were analyzed using ANOVA followed by Dunn’s multiple comparisons test using GraphPad Prism® 6 (GraphPad Software Inc., La Jolla, CA, USA).
We compared parasite invasion and development to schizonts in different cell lines (MDBK, m-ICcl2 and CLEC-213). For all cell lines, we observed similar percentages (~60%) of parasite invasion (Fig. 1a). We assessed the ability of the parasite to develop further by counting the number of schizonts I after 48 h of infection; we found that 20–30% of infected cells in all cell lines harboured schizonts (Fig. 1b). For all cell lines, merozoites I were found in the cell culture medium at 72 h p.i.; there was no merogony II when using MDBK or m-ICcl2. However, extracellular merozoites II were observed in CLEC-213 cells (Fig. 2c) suggesting the possibility for further parasite development with this specific cell line.
In order to increase the probability of gamete formation, CLEC-213 were infected with merozoites II isolated from the caeca of infected chickens. Merozoites II (INRA-mCherry) were able to invade the cells. After 2 days of infection, the presence of forms suggesting the presence of microgametes, macrogametes and unsporulated oocysts was observed by microscopy (Fig. 3). To confirm this observation, we used specific markers described by Walker et al. : EtGAM-56, a macrogamete specific protein incorporated into the oocyst wall and EtFOA1, a flagellar outer arm protein (also known as a dynein intermediate chain protein), which is specific to microgametes. First, we confirmed the increase of Etfoa1 and Etgam56 gene expression in purified gametes compared to sporozoites or merozoites I obtained in vivo as described by Walker et al. . Then, CLEC-213 were infected with merozoites II from the wild-type Wis strain of E. tenella, and Etfoa1 and Etgam56 gene expression levels were measured by RT-qPCR. Additionally, EtFOA1 and EtGAM56 protein expression was detected by immunofluorescence. In these conditions, an increase in Etfoa1 and Etgam56 gene expression was observed compared to cells at previous time points (Fig. 4a); this observation was confirmed by the detection of forms that were revealed by using specific antibodies for EtFOA1 and EtGAM56 suggesting the presence of microgametes and macrogametes, respectively (Fig. 4b (i, ii)).
Maintaining CLEC-213 in culture for 7 days can be challenging. We therefore attempted to replicate our results using sporozoites from the precocious strain, Wis-F-96, which displays a shorter parasite cycle than the wild type strain (7 days versus 5 days in vivo ). In these experimental conditions, we were again able to demonstrate an increase in Etfoa1 and Etgam56 gene expression, this time at day 5 post-infection (Fig. 4a), and were able to confirm the presence of microgametes and macrogametes by immunofluorescence (Fig. 4b (iii, iv)). However, we were unable to observe any oocysts after infection of CLEC-213 cells with sporozoites of WIS-F-96, though we cannot rule out that they were present at levels below our ability to detect at this earlier time-point.
Eimeria tenella is able to invade many different cell lines in vitro, as shown by Tierney et al. . However, the parasite’s life-cycle has been observed to proceed to completion, in vitro only in chick embryonic kidney cells or primary chicken kidney cells (PCKC), where sexual stages (i.e. macrogametes and microgametes) as well as oocysts have been observed after infection with sporozoites [7, 12, 22,23,24,25]. The complete life-cycle has also been achieved by in ovo infection of chorioallantoic membranes of chick embryos . In most currently tested cell lines, E. tenella develops only asexually, halting at the first generation of schizont in cultures of mammalian fibroblasts, mammalian epithelial cells, and avian fibroblasts [8, 26]. In vitro invasion of chick embryo kidney, chick embryo fibroblast, mouse fibroblast, human amnion, and HeLa cell cultures by E. acervulina sporozoites do not lead to further parasite development . However, studies using, non-poultry species of Eimeria (e.g. E. bovis, E. ovinoidalis, E. ninakohlyakimovae) have shown that the parasite can develop to various stages (merozoites I and a few gametocyte-like stages) in several cell types, including bovine, human and porcine endothelial cell lines, bovine foetal gastrointestinal cells, bovine kidney epithelial cells and African green monkey kidney epithelial cells [28,29,30,31,32]. More particularly, the development of E. nieschulzi macrogamonts and oocysts were observed when cultured with mixed cells derived from inner fetal organs . Here, we show similar levels of parasite invasion and development to the first generation of schizont in bovine epithelial-like kidney (MDBK), murine intestinal epithelial (m-ICcl2) and avian epithelial (CLEC-213) cells. For all cell lines, merozoites I were observed in the cell culture medium at 72 h p.i. but no extracellular merozoites II were observed when using MDBK or m-ICcl2 cells. These observations confirmed previous data using MDBK cells [8,9,10,11, 26] and, furthermore, demonstrated that a mammalian intestinal epithelial cell line (m-ICcl2) and an avian, non-intestinal epithelial cell line (CLEC-213) were at least equally permissive to invasion and initial asexual reproduction by E. tenella. However, in our experimental conditions, extracellular merozoites II were observed only in CLEC-213 cells, suggesting the possibility for further parasite development in this specific chicken epithelial cell line.
In order to maximize the chance of achieving development of sexual stages of E. tenella in vitro and minimize the time taken to reach these stages of development, we implemented two strategies: first, we infected CLEC-13 cells with purified merozoites II harvested from infected caeca and secondly, we infected CLEC-213 cells with sporozoites of a strain of E. tenella (Wis-F-96) that enters gametogony after only a single asexual cycle. In both cases, we observed forms consistent with microgametes and macrogametes, within two days of infection of cells with wild type merozoites II and within five days of infection with the precocious-strain sporozoites. To confirm the characterization of the putative gametes, we used specific markers described by Walker et al. . Briefly, EtGAM-56 is a macrogamete specific protein that is destined for incorporation into the oocyst wall. EtGAM-56 co-localises to wall forming bodies that are characterised by their doughnut-like appearance. EtFOA1 is a flagellar outer arm protein 1, also known as a dynein intermediate chain protein that is specific to microgametes . We studied the development of the parasite by measuring gene expression of Etfoa1 and Etgam56 and we confirmed that these genes are mainly expressed in gametes as shown in enriched gamete fractions compared to the free stages of the parasite (sporozoite, Sp, and merozoites I, M1). We then demonstrated the presence of gametes when cells were infected with merozoites II, 2 days p.i. as shown both by an increase in Etfoa1 and Etgam56 gene expression and by protein detection using specific antibodies. When cells were infected with sporozoites from the precocious strain for five days, we also observed an increase in gamete gene expression and we again detected the presence of gametes with specific antibodies. Additionally, we were able to observe fully-formed, unsporulated oocysts in the CLEC-213 cell cultures originally infected with the wild type merozoites II, demonstrating that completion of the final steps of the parasite cycle is possible in CLEC-213 cells. We also infected CLEC-213 cells with E. tenella Wis wild type strain; however, because the reproductive cycle of this parasite strain is longer than that for the precocious strain , we did not consistently observe sexual stages. It cannot be ruled out that optimisation of culture conditions for these cells may allow sexual development of the wild type parasite.
Thus overall, we have demonstrated for the first time, when using sporozoites from a precocious strain or merozoites II from a wild type strain, that in CLEC-213, a chicken epithelial cell line permits the development of sexual stages - both microgametes and macrogametes - of the parasite E. tenella in vitro, resulting in production of oocysts. Although, the infected culture leads to only relatively low yields of gametes, it is important to note that they can be detected and relative burden assessed easily by qPCR. Thus, this new avian epithelial cell model of infection holds great promise and constitutes a first step towards the development of a new tool for drug screening, and for assessment of the effect of immune factors on the Eimeria life-cycle, as it is now possible to carry out investigations on both asexual and sexual stages in vitro.
Chicken lung epithelial cells
Flagellar outer arm protein 1
Macrogamete specific protein
First generation merozoites
Madin-Darby bovine kidney epithelial cells
Transimmortalized mouse intestinal cells
Second generation merozoites
Primary chicken kidney cells
Yellow fluorescent protein
Dalloul RA, Lillehoj HS. Poultry coccidiosis: recent advancements in control measures and vaccine development. Expert Rev Vaccines. 2006;5(1):143–63.
Sharman PA, Smith NC, Wallach MG, Katrib M. Chasing the golden egg: vaccination against poultry coccidiosis. Parasite Immunol. 2010;32(8):590–8.
Kipper M, Andretta I, Lehnen CR, Lovatto PA, Monteiro SG. Meta-analysis of the performance variation in broilers experimentally challenged by Eimeria spp. Vet Parasitol. 2013;196(1–2):77–84.
McDougald LR, Jeffers TK. Comparative in vitro development of precocious and normal strains of Eimeria tenella (Coccidia). J Protozool. 1976;23(4):530–4.
Williams RB, Carlyle WW, Bond DR, Brown IA. The efficacy and economic benefits of Paracox, a live attenuated anticoccidial vaccine, in commercial trials with standard broiler chickens in the United Kingdom. Int J Parasitol. 1999;29(2):341–55.
Jeffers TK. Attenuation of Eimeria tenella through selection for precociousness. J Parasitol. 1975;61(6):1083–90.
Strout RG, Ouellette CA. Gametogony of Eimeria tenella (coccidia) in cell cultures. Science. 1969;163(3868):695–6.
Tierney J, Mulcahy G. Comparative development of Eimeria tenella (Apicomplexa) in host cells in vitro. Parasitol Res. 2003;90(4):301–4.
Chai JY, Lee SH, Kim WH, Yun CK. Development of Eimeria tenella in MDBK cell culture with a note on enhancing effect of preincubation with chicken spleen cells. Kisaengchunghak Chapchi. 1989;27(2):87–100. (In korean)
Kogut MH, Lange C. Interferon-gamma-mediated inhibition of the development of Eimeria tenella in cultured cells. J Parasitol. 1989;75(2):313–7.
Schmatz DM, Crane MS, Murray PK. Eimeria tenella: parasite-specific incorporation of 3H-uracil as a quantitative measure of intracellular development. J Protozool. 1986;33(1):109–14.
Zhang J, Wilson E, Yang S, Healey MC. Increasing the yield of Eimeria tenella oocysts in primary chicken kidney cells. Avian Dis. 1996;40(1):63–7.
Chapman HD. Milestones in avian coccidiosis research: a review. Poult Sci. 2014;93(3):501–11.
Esnault E, Bonsergent C, Larcher T, Bed’hom B, Vautherot JF, Delaleu B, et al. a novel chicken lung epithelial cell line: characterization and response to low pathogenicity avian influenza virus. Virus Res. 2011;159(1):32–42.
Walker RA, Sharman PA, Miller CM, Lippuner C, Okoniewski M, Eichenberger RM, et al. RNA Seq analysis of the Eimeria tenella gametocyte transcriptome reveals clues about the molecular basis for sexual reproduction and oocyst biogenesis. BMC Genomics. 2015;16:94.
Bens M, Bogdanova A, Cluzeaud F, Miquerol L, Kerneis S, Kraehenbuhl JP, et al. Transimmortalized mouse intestinal cells (m-ICc12) that maintain a crypt phenotype. Am J Phys. 1996;270(6 Pt 1):C1666–74.
Doran DJ, Vetterling JM, Augustine PC. Eimeria tenella - in vivo and in vitro comparison of Wisconsin, Weybridge, and Beltsville strains. Proc Helm Soc Wash. 1974;41(1):77–80.
Yan W, Liu X, Shi T, Hao L, Tomley FM, Suo X. Stable transfection of Eimeria tenella: constitutive expression of the YFP-YFP molecule throughout the life cycle. Int J Parasitol. 2009;39(1):109–17.
Shirley MW. Eimeria species and strains of chicken. In: Biotechnology-guidelines on techniques in coccidiosis research. Luxembourg: European Commission DGXII; 1995. p. 1–24.
Bessay M, Le Vern Y, Kerboeuf D, Yvore P, Quere P. Changes in intestinal intra-epithelial and systemic T-cell subpopulations after an Eimeria infection in chickens: comparative study between E acervulina and E. tenella. Vet Res. 1996;27(4–5):503–14.
Bussiere FI, Brossier F, Le Vern Y, Niepceron A, Silvestre A, de Sablet T, et al. Reduced parasite motility and micronemal protein secretion by a p38 MAPK inhibitor leads to a severe impairment of cell invasion by the apicomplexan parasite Eimeria tenella. PLoS One. 2015;10(2):e0116509.
Long PL. Observations on the growth of Eimeria tenella in cultured cells from the parasitized chorioallantoic membranes of the developing chick embryo. Parasitology. 1969;59(4):757–65.
Doran DJ, Augustine PC. Comparative development of Eimeria tenella from sporozoites to oocysts in primary kidney cell cultures from gallinaceous birds. J Protozool. 1973;20(5):658–61.
Hofmann J, Raether W. Improved techniques for the in vitro cultivation of Eimeria tenella in primary chick kidney cells. Parasitol Res. 1990;76(6):479–86.
Jiang L, Zhao Q, Zhu S, Han H, Dong H, Huang B. Establishment of Eimeria tenella (local isolate) in chicken embryos. Parasite. 2012;19(3):285–9.
Patton WH. Eimeria tenella: cultivation of the asexual stages in cultured animal cells. Science. 1965;150(3697):767–9.
Strout RG, Solis J, Smith SC, Dunlop WR. In vitro Cultivation of Eimeria acervulina (Coccidia). Exp Parasitol. 1965;17(3):241–6.
Hermosilla C, Barbisch B, Heise A, Kowalik S, Zahner H. Development of Eimeria bovis in vitro: suitability of several bovine, human and porcine endothelial cell lines, bovine fetal gastrointestinal, Madin-Darby bovine kidney (MDBK) and African green monkey kidney (VERO) cells. Parasitol Res. 2002;88(4):301–7.
Silva LM, Vila-Vicosa MJ, Cortes HC, Taubert A, Hermosilla C. Suitable in vitro Eimeria arloingi macromeront formation in host endothelial cells and modulation of adhesion molecule, cytokine and chemokine gene transcription. Parasitol Res. 2015;114(1):113–24.
Carrau T, Silva LM, Perez D, Ruiz de Ybanez R, Taubert A, Hermosilla C. First description of an in vitro culture system for Eimeria ovinoidalis macromeront formation in primary host endothelial cells. Parasitol Int. 2016;65(5 Pt B):516–9.
Ruiz A, Behrendt JH, Zahner H, Hermosilla C, Perez D, Matos L, et al. Development of Eimeria ninakohlyakimovae in vitro in primary and permanent cell lines. Vet Parasitol. 2010;173(1–2):2–10.
Chen H, Wiedmer S, Hanig S, Entzeroth R, Kurth M. Development of Eimeria nieschulzi (Coccidia, Apicomplexa) gamonts and oocysts in primary fetal rat cells. J Parasitol Res. 2013;2013:591520.
We are thankful to Alain Vandewalle (UFR de Médecine Bichat, France) for the cell line, m-ICcl2, to Janene Bumstead, Damer Blake and Fiona Tomley (Royal Veterinary College, University of London, UK) who kindly provided us the Wis and Wis-F-96 strains of E. tenella and the MDBK cell line. We are also grateful to Sébastien Lavillatte and Edouard Guitton (INRA Centre Val de Loire-PFIE, France) for their skills in animal care.
This work was supported by INRA.
Availability of data and materials
The data supporting the conclusions are included within the article. The raw data are available upon request to the corresponding author.
Ethics approval and consent to participate
Experimental protocols were performed in accordance with the French legislation (Décret: 2001-464 29/05/01), the EEC regulation (86/609/CEE) about laboratory animals and after authorization by the local ethics committee for animal experimentation (CEEA VdL): 2012-11-09 that was renewed on 2016-03-04.
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
About this article
Cite this article
Bussière, F.I., Niepceron, A., Sausset, A. et al. Establishment of an in vitro chicken epithelial cell line model to investigate Eimeria tenella gamete development. Parasites Vectors 11, 44 (2018). https://doi.org/10.1186/s13071-018-2622-1
- Eimeria tenella
- Chicken epithelial cells