- Open Access
Molecular and phylogenetic characterization of Cryptosporidium species in the saffron finch Sicalis flaveola
BMC Veterinary Research volume 18, Article number: 449 (2022)
Cryptosporidium is the most common protozoan that can infect a wide variety of animals, including mammals and birds. Fecal samples of six saffron finches, Sicalis flaveola, from a commercial establishment were screened for the presence of Cryptosporidium by the modified Ziehl–Neelsen technique and nested PCR of the 18S rRNA gene followed by sequencing of the amplified fragments.
The species Cryptosporidium galli was identified in all six saffron fiches, in addition to Cryptosporidium andersoni in one of the birds, indicating a mixed infection. Only two birds had feathers that were ruffled and dirty with feces. Concomitant infection with Isospora spp. was observed in all birds.
Saffron finches are a possible host of C. andersoni and this is the first report of this species in a captive bird and the third report of parasitism by C. galli in Sicalis flaveola.
Protozoa of the genus Cryptosporidium belong to the Phylum Miozoa, Subphylum Myzozoa, Infraphylum Apicomplexa, Superclass Sporozoa, Class Gregarinomorphea, Subclass Cryptogregaria and Order Cryptogregarida . Cryptosporidium is one of the most important parasitic protozoa that can be transmitted through food and water contamination and is recognised as a major contributor to morbidity and is estimated to cause an annual global loss of 13 million disability adjusted life years (DALYs) .
Cryptosporidium is characterized by extensive genetic variation and pathogenicity. To date, there are 44 valid species and about 60 genotypes reported from all over the world [3–6]. There are 8 species of Cryptosporidium that infect birds: Cryptosporidium meleagridis, Cryptosporidium baileyi, Cryptosporidium galli, Cryptosporidium ornithophilus, Cryptosporidium proventriculi, Cryptosporidium avium, Cryptosporidium parvum and Cryptosporidium andersoni [7, 8].
Cryptosporidium baileyi infects the epithelium of a wide variety of organs, such as the trachea and the bursa of Fabricius, while C. meleagridis infects the small intestine and cecum [9, 10]. Cryptosporidium galli causes changes in the proventriculus as the parasite develops in the epithelial cells of this organ and does not affect either the intestines or the respiratory tract . C. ornithophilus n. sp. infects the caecum, colon and bursa Fabricii . C. proventriculi infects the microvilli in the proventriculus and ventriculus . C. avium infects the microvilli in the ileum and caecum . C. parvum develops lesions in the small intestine and cecum and can cause disruption of intestinal epithelial integrity [14, 15]. C. andersoni has been found in the feces of wild bird [8, 16–18] but its site of infection in birds is not yet defined.
The aim of the present study was identify and characterize molecularly Cryptosporidium species in fecal samples of saffron finches, Sicalis flaveola, from a commercial farm in the city of Campos dos Goytacazes, state of Rio de Janeiro, Brazil.
Cryptosporidium oocysts were detected in all fecal samples by microscopic analysis of smears stained using the Ziehl–Neelsen technique (Fig. 1).
Molecular analysis revealed amplification of Cryptosporidium 18S rRNA gene in all samples analyzed. By sequencing the fragment amplified by nested PCR (n-PCR), the species C. galli was identified in all samples, but in one of the birds, a mixed infection was detected since in one of the sequencing runs, the species C. andersoni was identified. The C. galli isolates from the present study shared 99.71–100% similarity with other C. galli isolates according to nBlast analysis, and the C. andersoni isolate from one of the birds shared 100% identity with C. andersoni isolated from a whooper swan (Cygnus cygnus). Molecular characterization of the seven Cryptosporidium sequences was performed with phylogenetic reconstructions of the 18S rRNA gene using a total of 343 positions in the final dataset. Phylogenetic reconstructions of the Cryptosporidium 18S rRNA gene sequences from S. flaveola can be seen in Fig. 2.
The sporulated oocysts of C. galli (n = 117) were 5.81 ± 0.78 (3.97–8.09) by 4.86 ± 0.66 (3.3–7.23) µm on average, with a length/width ratio of 1.20 ± 0.12 (0.95–1.50). The oocysts of the positive sample for two Cryptosporidium species were not measured. The microscopic analysis also detected oocysts of Isospora spp. Two birds had feathers ruffled and soiled with feces.
Common techniques used to diagnose Cryptosporidium infection are microscopic analysis and n-PCR . Despite microscopy being an intensive procedure that demands time and experience, the extraction of DNA from fecal samples of S. flaveola was performed only by means of previous microscopy. As discussed by Nakamura et al. , performing PCR on samples previously identified as positive by microscopy implies a lower cost, as the reagents are expensive. Microscopy is an affordable and quick technique; however, it does not identify Cryptosporidium species and is less sensitive and specific. Therefore, n-PCR was performed to allow the identification of the species after amplicon sequencing.
In the present study, we identified only 2 of the 8 species of Cryptosporidium already found in birds. The 100% positivity of saffron finches, family Emberizidae, was high, but the number of samples collected and analyzed was low, making it difficult to compare the prevalence with that reported in most studies of Cryptosporidium in captive and wild birds. One factor that may interfere with the rate of Cryptosporidium infection is a difference in the age of the animals [21, 22], although almost all reports of Cryptosporidium infections in captive or wild birds do not specify the age range of the animals examined.
Silva et al.  carried out a study in which 480 samples of passerine feces were collected from Araçatuba, São Paulo. Of these samples, 105 were positive for Cryptosporidium, with n-PCR and sequencing revealing all infections to be of the species C. galli. Similarly, Antunes et al.  detected the species C. galli in all samples studied through molecular analysis, with four canaries (Serinus canaria) and eight cockatiels (Nymphicus hollandicus) in captivity. These works corroborate the finding of the present study in which C. galli was detected in all PCR-positive samples.
The mean size of C. galli oocysts obtained in the present study was smaller than the mean size of C. galli reported by Ryan et al.  and by Qi et al. . The acid-fast staining causes shrinkage and deformation of oocysts and this could explain the smaller size of oocysts in this study as compared to other studies. Since the sizes of the oocysts of different species of Cryptosporidium are very similar, oocyst morphometry alone is not sufficient to distinguish the species, making molecular studies necessary for accurate identification.
Among the species/genotypes of Cryptosporidium in birds, only two named species, C. baileyi and C. galli, were identified in the saffron finch, S. flaveola, in previous studies [20, 27, 28]. Nakamura et al.  conducted a study of 966 stool samples from birds belonging to 18 families. These captive or wild birds came from three Brazilian states: Goiás, Paraná and São Paulo. In a specimen of S. flaveola, the species C. baileyi (GQ227475) was diagnosed through PCR and sequencing of the 18S rRNA gene. In 2012, Sevá and colleagues  analyzed 242 fecal samples from wild birds seized by the environmental control agency of São Paulo State. Four S. flaveola were positive for Cryptosporidium, three birds harbored the species C. galli (GU816048, GU816069, HM126668), and one was positive for the species C. baileyi (GU816042). Nakamura et al.  collected a total of 1027 fecal samples from birds of the orders Psittaciformes and Passeriformes. These birds were from captivity or the wild and came from Divisão Técnica de Medicina Veterinária e Manejo da Fauna Silvestre (DEPAVE-3) of São Paulo. Of the 108 positive samples, 40 were sequenced, one of which was from S. flaveola and was positive for C. galli according to n-PCR sequencing (accession number in GenBank not available). Even though our research represents the third diagnostic report of C. galli in S. flaveola, further studies are still needed on species or genotypes of Cryptosporidium that can infect this species of Passeriformes.
A coinfection of C. galli and C. andersoni occurred in one of the birds in the present study, although only monoinfections were previously found in S. flaveola [20, 27, 28]. According to Máca and Pavlásek , the intensive rearing of birds in breeders can be problematic, as it is associated with a large number of birds in a relatively small area, increasing the possibility of bacterial, viral and parasitic diseases and their rapid spread compared to those in wild birds.
The birds in the present study lived in separate cages but were kept in the same environment and close to each other. As reported by Nakamura et al. , this can result in the spread of infection through direct contact with feces or human transport of oocysts during routine management related to cleaning. In addition, the saffron finch cages were close to the cages of other bird species, which may have contributed to the interspecific spread of Cryptosporidium infections.
Specifically, C. galli infections are associated with other pathogens , and these associations can lead to weight loss, lameness, pelvic limb joint swelling and high mortality in captive birds . Although the birds in the present study were infected with Isospora oocysts, they did not show any of these clinical symptoms. Due to the association of infections by C. galli and Isospora in the birds of the present study, it was not possible to determine which agent was responsible for the feathers ruffled and soiled with feces observed on two of the birds, since both infections can cause the observed characteristics. According to Cox et al. , in mixed infections, the burden of one or both infectious agents may be increased, that of one or both may be suppressed, or that of one may be increased and that of the other suppressed.
Passerines infected with C. galli can shed oocysts intermittently for 12–13 months [23, 24]. The determination of intermittent and prolonged shedding of C. galli oocysts in fecal samples, in addition to demonstrating that this species causes chronic infection in birds, also maintains the species between generations of birds through contact between parents and progeny. In view of this, it is necessary to adopt strict sanitary management measures to prevent the occurrence of infections in breeders, commercial establishments and nongovernmental organizations that receive apprehended wild birds.
The C. andersoni isolate from S. flaveola (Isolate 4b) clustered with the other isolates of the same species from previous studies (MT648437 and KT175411) with high (98%) bootstrap support (Fig. 2). The branch of the C. andersoni species clustered with the isolates of C. galli, which is also a gastric parasite, suggesting that these two Cryptosporidium species are close relatives. Cryptosporidium andersoni is a species found mainly in cattle and humans [32, 33] but was previously reported in the bird Podargus strigoides in an Australian study  and in an ostrich, Struthio camelus, from a zoo in southwestern France . Similar to Ng et al. , we were unable to determine whether the presence of C. andersoni oocysts in the fecal samples of birds analyzed in the present study was due to a real infection or accidental contamination by mechanical transport, since the birds in the present study had close contact with humans. In addition, animals can also be infected indirectly after drinking water contaminated with Cryptosporidium. In view of the above, studies are needed to discover whether birds are natural hosts or only carriers of C. andersoni, since studies have already reported that a species of Cryptosporidium may have a wider host range than originally assumed .
In conclusion, the high C. galli parasite load in all birds in this research shows that the saffron finch, S. flaveola, is a host of this protozoan species, although this is the third report of parasitism in this bird species. In addition, S. flaveola may contribute to the maintenance of intraspecific and interspecific infections in environments with large numbers of birds. This is the first report of C. andersoni in a captive bird and the low prevalence in our studies and the few reports of coccidia from this species in birds prevent us from inferring that this species of passerine is a good host or if it is simply a carrier of the protozoan. Further research is required to define the public health importance of Cryptosporidium in feces of birds.
Material and methods
Fecal samples and the Ziehl–Neelsen method
Fecal samples were collected from six adult saffron finches, Sicalis flaveola, from a commercial establishment in the city of Campos dos Goytacazes, Rio de Janeiro, Brazil. This study was approved by the Biodiversity Authorization and Information System (SISBIO) under protocol n° 78,016–1/2022 and all experimental protocols were approved by the ethics committee in the use of animals (protocol n° 523). The six birds were in separate cages, and all fecal content deposited at the bottom of the cage during a 24-h period was collected and placed in a sterile collection tube. The tubes were identified and transported in isothermal boxes with ice to the Center for Advanced Research in Parasitology of the Universidade Estadual do Norte Fluminense Darcy Ribeiro. A part of the fecal content was examined for the presence of oocysts of Cryptosporidium spp. by microscopy of fecal smears stained by the modified Ziehl–Neelsen technique according to Angus . Measurements were made using a Zeiss AxioVision Sample Images Software and are provided in micrometers.
DNA extraction and nested PCR
From the other part of the fecal content, genomic DNA was extracted using a DNA and tissue kit (QIAGEN) with some modifications of the manufacturer's protocol . DNA samples were stored at − 20 °C, and all samples were screened for Cryptosporidium using n-PCR to amplify fragments of the 18S subunit of the rRNA gene [37, 38], with subsequent sequencing of amplified fragments. Primers P1: 5-TTTCTAGAGCTAATACATGCG-3, P2: 5-CCCATTTCCTTCGAAACAGGA-3 and P3: 5-GGAAGGGTTGTATTTATTAGATAAAG-3, P4: 5-AAGGAGTAAGGAACAACCTCCA-3 were used for the primary (~ 1325 bp) and secondary (~ 830 bp) reactions, respectively. The second amplification products were examined with 1% (w/v) agarose gel electrophoresis after staining with DNA Green (Solarbio, Beijing, China). In addition, Cryptosporidium parvum DNA was used as a positive control, and ultrapure water was used as a negative control.
Sequencing and phylogenetic analysis
The amplified fragment (~ 830 bp) resulting from the secondary reaction of n-PCR was purified using the GFX PCR DNA Band Purification® Kit (GE Health Sciences, Champaign, IL, USA) and sequenced with the aid of DYEnamic® ET Kit Cycle Sequencing® Terminator Dye (GE Health Sciences, Champaign, IL, USA) on a MegaBACE® sequencer (GE Health Sciences, Champaign, IL, USA). Sequencing reactions were performed at least three times in both directions with the n-PCR secondary reaction primers. The consensus sequence was analyzed using CodonCode Aligner v.2.0.4 software (CodonCode Corp., Dedham, MA) and aligned with Cryptosporidium reference sequences published in GenBank (https://blast.ncbi.nlm.nih.gov/Blast.cgi) using MEGA X software  by the neighbor-joining method  after estimating the distance using the Kimura 2-parameter model . All positions containing gaps and missing data were eliminated from the dataset (full delete option). In the construction of the phylogenetic tree, Eimeria tenella (KT184354) was used as an outgroup. Group confidence was assessed by bootstrap values using 1000 replicates.
The following sequences were used to construct the phylogenetic tree: MK311144 (C. baileyi) from Erythrura gouldiae, GQ227475 (C. baileyi) from Sicalis flaveola, MK311145 (C. baileyi) from Carduelis psaltria, MK311141 (Avian genotype I) from Serinus canaria, GQ227479 (Avian genotype I) of Serinus canaria, HM116381 (Avian genotype V) of Nymphicus hollandicus, DQ650341 (Avian genotype II) of Eolophus roseicapilla, DQ002931 (Avian genotype II) of Struthio camelus, HM116382 (C. meleagridis) of Columba livia, HM116383 (C. meleagridis) from Bombycilla garrulus, HM116384 (C. meleagridis) from Streptopelia orientalis, DQ650344 (Avian genotype IV) from Zosterops japonica, MK311135 (C. proventriculi) from Poicephalus gulielmi, MK311136 (C. proventriculi) from Agapornisico rosellis, GU816048 (C. galli) from Sicalis flaveola, GU816049 (C. galli) from Saltator similis, GU816054 (C. galli) from Sporophila angolensis, KT175411 (C. andersoni) from slaughterhouse wastewater, MT648437 (C. andersoni) from Cygnus sp., KJ939306 (C. parvum) from Accipiter nisus, MH636820 (C. parvum) from an unspecified bird, KU058877 (C. avium) from Melopsittacus undulatus, KU058878 (C. avium) from Cyanoramphus novaezelandiae, MN969963 (C. ornithophilus) from Nymphicus hollandicus and MN969962 (C. ornithophilus) isolated from Anser anser.
Availability of data and materials
The 18S rRNA gene nucleotide sequences were deposited in the GenBank database under accession numbers OM436006-OM436011 (C. galli) and OM491513 (C. andersoni).
Ruggiero MA, Gordon DP, Orrell TM, Bailly N, Bourgoin T, Brusca RC, Cavalier-Smith T, Guiry MD, Kirk PM. Correction: A Higher Level Classification of All Living Organisms. PLoS ONE. 2015;10(6):e0130114. https://doi.org/10.1371/journal.pone.0130114.Erratumfor:PLoSOne.2015;10(4):e0119248.
Khalil IA, Troeger C, Rao PC, Blacker BF, Brown A, Brewer TG, Colombara DV, De Hostos EL, Engmann C, Guerrant RL, Haque R, Houpt ER, Kang G, Korpe PS, Kotloff KL, Lima AAM, Petri WA Jr, Platts-Mills JA, Shoultz DA, Forouzanfar MH, Hay SI, Reiner RC Jr, Mokdad AH. Morbidity, mortality, and long-term consequences associated with diarrhoea from Cryptosporidium infection in children younger than 5 years: a meta-analyses study. Lancet Glob Health. 2018;6:e758–68.
Čondlová Š, Horčičková M, Sak B, Květoňová D, Hlásková L, Konečný R, Stanko M, McEvoy J, Kváč M. Cryptosporidium apodemi sp. n. and Cryptosporidium ditrichi sp. n. (Apicomplexa: Cryptosporidiidae) in Apodemus spp. Eur J Protistol. 2018;63:1–12.
Holubová N, Tůmová L, Sak B, Hejzlarová A, Konečný R, McEvoy J, Kváč M. Description of Cryptosporidium ornithophilus n sp (Apicomplexa: Cryptosporidiidae) in farmed ostriches. Parasit Vectors. 2020;13:1–17.
Wang R, Zhao G, Gong Y, Zhang L. Advances and perspectives on the epidemiology of bovine Cryptosporidium in China in the past 30 years. Front Microbiol. 2017;8:1–6.
Xiao L, Fayer R, Ryan U, Upton SJ. Cryptosporidium taxonomy: recent advances and implications for public health. Clin Microbiol Rev. 2004;17:72–97.
Ryan UM, Feng Y, Fayer R, Xiao L. Taxonomy and molecular epidemiology of Cryptosporidium and Giardia - a 50 year perspective (1971–2021). Int J Parasitol. 2021;51:1099–119.
Wang Y, Zhang K, Chen Y, Li X, Zhang L. Cryptosporidium and cryptosporidiosis in wild birds: a one health perspective. Parasitol Res. 2021;120:3035–44.
Zha HB, Jiang JS. Life cycle of Cryptosporidium meleagridis in quails. Acta Vet Zootechn. 1994;25:273–8.
Bermudez AJ, Ley DH, Levy MG, Barnes HJ, Gerig TM. Experimental cryptosporidiosis in turkey poults. In: Proceedings Meeting American Veterinary Medical Association. Chicago: Annals; 1987.
Pavlásek I. Cryptosporidia: biology, diagnosis, host spectrum, specificity, and the environment. Klin Mikrobiol Infekcni Lek. 1999;3:290–301.
Holubová N, Zikmundová V, Limpouchová Z, Sak B, Konečný R, Hlásková L, Rajský D, Kopacz Z, McEvoy J, Kváč M. Cryptosporidium proventriculi sp. n. (Apicomplexa: Cryptosporidiidae) in Psittaciformes birds. Eur J Protistol. 2019;69:70–87.
Holubová N, Sak B, Horčičková M, Hlásková L, Květoňová D, Menchaca S, McEvoy J, Kváč M. Cryptosporidium avium n. sp. (Apicomplexa: Cryptosporidiidae) in birds. Parasitol Res. 2016;115:2243–51.
Zylan K, Bailey T, Smith HV, Silvanose C, Kinne J, Schuster RK, Hyland K. An outbreak of cryptosporidiosis in a collection of Stone curlews (Burhinus oedicnemus) in Dubai. Avian Pathol. 2008;37:521–6.
Nakamura AA, Meireles MV. Cryptosporidium infections in birds–a review. Rev Bras Parasitol Vet Braz J Vet Parasitol. 2015;24:253–67.
Kassa H, Harrington BJ, Bisesi MS. Cryptosporidiosis: A brief literature review and update regarding Cryptosporidium in feces of Canada geese (Branta canadensis). J Environ Health. 2004;66:34–40.
Ng J, Pavlasek I, Ryan U. Identification of novel Cryptosporidium genotypes from avian hosts. Appl Environ Microbiol. 2006;72:7548–53.
Osman M, El Safadi D, Benamrouz-Vanneste S, Cian A, Moriniere R, Gantois N, Delgado-Viscogliosi P, Guyot K, Bosc S, Chabé M, Petit T, Viscogliosi E, Certad G. Prevalence, transmission, and host specificity of Cryptosporidium spp. in various animal groups from two French zoos. Parasitol Res. 2017;116:3419–22.
Jex AR, Smith HV, Monis PT, Campbell BE, Gasser RB. Cryptosporidium – biotechnological advances in the detection, diagnosis, and analysis of genetic variation. Biotechnol Adv. 2008;26:304–17.
Nakamura AA, Simões DC, Antunes RG, da Silva DC, Meireles MV. Molecular characterization of Cryptosporidium spp. from fecal samples of birds kept in captivity in Brazil. Vet Parasitol. 2009;166:47–51.
de Graaf DC, Vanopdenbosch E, Ortega-Mora LM, Abbassi H, Peeters JE. A review of the importance of cryptosporidiosis in farm animals. Int J Parasitol. 1999;29:1269–87.
Epidemiology NG. In: Fayer R, Xiao L, editors. Cryptosporidium and Cryptosporidiosis. Boca Raton: CRC Press and IWA Publishing; 2008. p. 79–118.
Silva DC, Homem CG, Nakamura AA, Teixeira WF, Perri SH, Meireles MV. Physical, epidemiological, and molecular evaluation of infection by Cryptosporidium galli in Passeriformes. Parasitol Res. 2010;107:271–7.
Antunes RG, Simões DC, Nakamura AA, Meireles MV. Natural infection with Cryptosporidium galli in canaries (Serinus canaria), in a cockatiel (Nymphicus hollandicus), and in lesser seed-finches (Oryzoborus angolensis) from Brazil. Avian Dis. 2008;52:702–5.
Ryan UM, Xiao L, Read C, Sulaiman IM, Monis P, Lal AA, Fayer R, Pavlásek I. A redescription of Cryptosporidium galli Pavlásek, 1999 (Apicomplexa:Cryptosporidiidae) from birds. J Parasitol. 2003;89:809–13.
Qi M, Wang R, Ning C, Li X, Zhang L, Jian F, Sun Y, Xiao L. Cryptosporidium spp. in pet birds: genetic diversity and potential public health significance. Exp Parasitol. 2011;128:336–40.
Sevá AP, Funada MR, Richtzenhain L, Guimarães MB, Souza SO, Allegretti L, Sinhorini JA, Duarte VV, Soares RM. Genotyping of Cryptosporidium spp. from free-living wild birds from Brazil. Vet Parasitol. 2011;175:27–32.
Nakamura AA, Homem CG, da Silva AM, Meireles MV. Diagnosis of gastric cryptosporidiosis in birds using a duplex real-time PCR assay. Vet Parasitol. 2014;205:7–13.
Máca O, Pavlásek I. Cryptosporidium infections of ring-necked pheasants (Phasianus colchicus) from an intensive artificial breeding programme in the Czech Republic. Parasitol Res. 2016;115:1915–22.
Lindsay DS, Blagburn BL, Hoerr FJ, Smith PC. Cryptosporidiosis in zoo and pet birds. J Protozool. 1991;38:180S-181S.
Cox FEG. Concomitant infections, parasites and imune responses. Parasitol. 2001;122:S23–38.
Chalmers RM, Katzer F. Looking for Cryptosporidium: the application of advances in detection and diagnosis. Trends Parasitol. 2013;29:237–51.
Ryan UM, Fayer R, Xiao L. Cryptosporidium species in humans and animals: current understanding and research needs. Parasitol. 2014;141:1667–85.
Widmer G, Sullivan S. Genomics and population biology of Cryptosporidium species. Parasite Immunol. 2012;34:61–71.
Angus KW. Cryptosporidiosis in domestic animals and humans. In Pract. 1987;9:47–9.
Santín M, Trout JM, Xiao L, Zhou L, Greiner E, Fayer R. Prevalence and age-related variation of Cryptosporidium species and genotypes in dairy calves. Vet Parasitol. 2004;122:103–17.
Xiao L, Escalante L, Yang C, Sulaiman I, Escalante AA, Montali RJ, Fayer R, Lal AA. Phylogenetic analysis of Cryptosporidium parasites based on the small-subunit rRNA gene locus. Appl Environ Microbiol. 1999;65:1578–83.
Xiao L, Alderisio K, Limor J, Royer M, Lal AA. Identification of species and sources of Cryptosporidium oocysts in storm waters using a small-subunit rRNA-based diagnostic and genotyping tool. Appl Environ Microbiol. 2000;66:54926–5498.
Kumar S, Stecher G, Li M, Knyaz C, Tamura K. MEGA X: Molecular Evolutionary Genetics Analysis across computing platforms. Mol Biol Evol. 2018;35:1547–9.
Saitou N, Nei M. The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol. 1987;4:406–25.
Kimura MA. Simple method for estimating evolutionary rate of base substitutions through comparative studies of nucleotide sequences. J Mol Evol. 1980;16:111–20.
The authors would like to thank CAPES (Coordination for the Improvement of Higher Education Personnel) for granting the scholarship to T.K.S., Elizeu during the development of this research.
Financial support was received from FAPERJ (Fundação de Amparo à Pesquisa do Estado do Rio de Janeiro) through Scientist of Our State scholarship (grant number 232568).
Ethics approval and consent to participate
All methods in this study were performed according to the relevant guidelines and regulations. This study was approved by the Biodiversity Authorization and Information System (SISBIO) under protocol n° 78016–1/2022. All experimental protocols were approved by the ethics committee in the use of animals (protocol n° 523) of the Universidade Estadual do Norte Fluminense.
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 licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. 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 in a credit line to the data.
About this article
Cite this article
de Oliveira, F.C.R., Gallo, S.S.M., Elizeu, T.K.S. et al. Molecular and phylogenetic characterization of Cryptosporidium species in the saffron finch Sicalis flaveola. BMC Vet Res 18, 449 (2022). https://doi.org/10.1186/s12917-022-03553-5
- Cryptosporidium galli
- Cryptosporidium andersoni
- Molecular biology
- Sicalis flaveola