Feasibility of Non-Invasive Molecular Method for Sexing of Parrots.
Abstract. - The aim of this study was to test the feasibility and efficacy of a non-invasive molecular method for gender identification of parrots, using different types of samples and the Chromo Helicase DNA-binding (CHD) gene as a molecular marker. DNA was isolated primarily from feathers and the amplification of the CHD gene was performed using 2550F/2718R primers. In order to compare the reliability of different sources of DNA, we used buccal swab, blood and feces. All sample types exerted successful sexing results with the exception of feces samples where the success rate was 25%. Sexing was successfully determined in 239 birds belonging to 32 species of parrots. In 6 species (Amazona finschi, A. leucocephala, Aratinga aurea, Barnardius zonarius, Coracopsis nigra and Nymphicus hollandicus), 2550F/2718R primers proved to work well for the first time. Species used in this study are on the IUCN red list of threatened species.
Furthermore, Amazona finschi, A. leucocephala, Cacatua moluccensis and C. sulphurea are on the list of CITES Apendix I. Since the failure in reproduction is one of the main causes of illegal trafficking of parrots, the non-invasive and universal molecular sexing method we tested may be a very useful tool in the preservation of endangered parrot species.
Key words: Psittaciformes, conservation, molecular sexing, CHD gene, 2550F/2718R.
Avian order Psittaciformes (parrots) accounts for around 375 species in 86 genera (BirdLife International, 2013) They are commonly held in captivity, with over 20 000 parrots housed in Zoological Gardens and other animal holding facilities and millions more held in private hands (Young et al., 2012). Therefore, trapping wild parrots for pet trade, as well as hunting, habitat loss and competition from invasive species led to the decrease of wild parrot populations, making them more exploited than any other group of birds (Snyder et al., 2000). In fact, nineteen parrot species are extinct, 15 are critically endangered, 34 endangered, 48 vulnerable and 42 near threatened (International Union for Conservation of Nature - IUCN 2012). In globally threatened species, the sex ratio distortion seems to be often larger than in non- threatened species, suggesting that their extinction risk could be higher than currently estimated (Donald, 2007).
A number of recent studies have been focused on the development of efficient molecular methods for sex identification, which are gaining undivided attention as an aid in research and conservation of many bird species (Cerit and Avanus, 2007).
According to Jensen et al. (2003) it is critically important to minimize handling-induced stress when sexing chicks, fragile individuals, or endangered species. That implies selection of samples for DNA extraction without risk for survival of birds. In light of that, the following types of samples were proposed as favourable: blood (Hoysak and Weatherhead, 1991; Lanctot, 1994; Gaunt and Oring, 1999; Goymann and Wingfield 2004), feathers (Bello et al., 2006), buccal swab (Handel et al., 2006) and feces (Idaghdour et al., 2003). Although blood sampling has no significant effect on the short-term and long-term survival of developing birds (Sheldon et al., 2008), Brown and Brown (2009) suggested caution in collecting blood from wild birds.
This study was based on Chromo Helicase DNA-binding genes (CHDW/CHDZ genes) (Ellegren and Sheldon, 1997) due to their proven usage in almost all bird species, with the exception of ratites (Griffiths et al., 1996). Due to its high degree of conservation, Ellegren (1996) suggested that the CHD gene is an interesting marker which provides an opportunity for developing a universal method for molecular Psittaciformes sexing. Generally, PCR amplification of the CHD gene with primers used in this study produces a single Z-band in male and two bands (Z and W) in female birds due to the difference in intron size. However, errors can occur due to allelic dropout, where females are miss-sexed as males (Arnold et al., 2003; Robertson and Gemmell, 2006) or due to the formation of heteroduplex DNA molecules, where males can be misidentified as females (Casey et al., 2009).
Taking all given facts into account, the aim of this study was to test the feasibility and efficacy of molecular sex identification in Psittaciformes using different types of samples for DNA extraction (blood, feathers, buccal swab and feces) and applying the protocol that had proven to work well in our previous research (Vucicevic et al., 2012).
MATERIALS AND METHODS
A total of 239 individuals were sampled for gender identification. Sampled birds belong to 32 parrot species. Among a total of 398 samples, there were 239 feather samples, 15 blood samples, 72 buccal samples and 72 feces samples (Table 1). Samples were provided by Zoological Gardens and private breeders.
Blood was collected with a sterile cotton swab after clipping a toenail; one to three thoracic feathers were sampled by plucking and quills were cut into 2-5 mm long pieces; sterile cotton swabs were used to collect buccal and feces samples.
Isolation of DNA
DNA was isolated by using the KAPA Express Extract kit (KAPA Biosystems Cat. No. KK7152), following the kit protocol. The incubation step lasted 20 min at 75degC and additional 5 min at 95degC. Fifty uL of the obtained DNA isolate was added to 200 ul 1x TE buffer (Serva, Cat. No.39799.01). Ten uL of the obtained dilution of DNA isolate were used in the PCR reaction.
The following set of primers was used for the amplification of the CHD gene: 2550F (5'-GTTACTGATTCGTCTACGAGA-3') and 2718R (5'-ATTGAAATGATCCAGTGCTTG-3') published by Fridolfosson and Ellegren (1999).
The amplification was carried out in 25 uL reaction volume containing 12.5 uL of KAPA2G Robust HotStart ReadyMix (Cat. No. KK7152, Kapa Biosystems), 1.25 uL volume of 1uM final concentration of each primer from 2550F/2718R primer set and 10 uL DNA sample.
The recommended thermal protocol of KAPA2G Robust HotStart ReadyMix was used: 3 min of initial denaturation at 95degC, followed by 45 cycles of denaturation (15 sec at 95degC), primer annealing (15 sec at 52degC), and extension (15 sec at 72degC). The final extension step at 72degC lasted 8 min.
Visualization of PCR products
The PCR products were visualised with UV light after staining the 2% agarose gel with ethidium bromide. A commercial O'RangeRuler 50 bp DNA Ladder (Fermentas) and Nippon 100bp DNA Ladder were used as the size markers to determine Z- and W-bands.
Gender of sampled birds (N=239) was successfully identified using feather samples. The results were additionally confirmed using other types of samples: 72 buccal swabs, 15 blood samples and 72 feces samples. All types of samples from a single individual gave the same result.
However, when feces were used as a sample, gender identification had a success rate of 25% using the same KAPA2G Robust HotStart ReadyMix and 2550F/2718R primer set. After electrophoresis of PCR products, parrots' gender was determined by visualization on agarose gel as two bands in females (Z and W) or one band in males (Z) with the difference range of 150 to 250 bp between Z- and W-bands, which made separation and visualization simple and reliable (Fig.1).
Primers 2550F/2718R were for the first time successfully used for amplification of CHD gene of Amazona finschi, A. leucocephala, Aratinga aurea, Barnardius zonarius, Coracopsis nigra and Nymphicus hollandicus.
All species sampled in this study are on the IUCN red list of threatened species (Table I). Four species (Amazona finschi, A. leucocephala, Cacatua moluccensis and C. sulphurea) are on the list of CITES Appendix 1 (the Convention on International Trade in Endangered Species of Wild Fauna and Flora).
Parrots are considered to be amongst the most heavily traded birds on Earth (Collar, 2000). In countries where parrot export and import are illegal, the time spent for the reproduction process, consequently causes very significant financial losses (Cahill et al., 2006).
Conservation techniques such as enhanced education, generation of public awareness and support, habitat protection, and law enforcement initiatives are highly effective and economical for dealing with a problems posed by the bird trade (Snyder et al., 2000; Mahboob and Nisa, 2009). Snyder et al. (2000) indicated that for management of vulnerable and endangered species (as the majority of parrots), potential bias in sex ratio is of great concern. Same group of authors gave general recommendations for parrots' reintroduction programs, where it is advised to determine the sex of individuals who are about to be released into the wild. Additionally, numerous bird protection programs aimed at preservation of various species through intensive bird breeding imply that the sex of individuals is accurately identified (Ito et al., 2003).
Still, captive breeding as a conservation technique used for increasing extant populations, correcting sex-ratio imbalances, re-establishing extirpated populations, and/or establishing new populations is considered to be expensive (Wilson et al., 1994).
Therefore, economical, non-invasive and precise method for the sexing of parrots is indispensable. In that regard, the aim of this study was to assess the effectiveness of a molecular method for sex determination in parrots and samples were taken from species with a relatively wide distribution throughout the Psittaciformes order. In previous studies (Miyaki et al., 1998; Taylor and Parkin, 2008), sexing various species of parrots was mostly conducted with P2/P8 primer set described by Griffits et al. (1998). Ong and Vellayan (2008) indicated that 2550F/2718R primer set, which was used in this research, provides a higher confidence level of establishing the sex of birds even without the use of polyacrylamide gels as is required in some bird species with the use of primers P2/P8 and 1237L/1272H (Kahn et al., 1998).
In this study, primers of 2550F/2718R for the first time enabled successful sex determination in Amazona finschi, Aratinga aurea, Barnardius zonarius and Coracopsis nigra, but also in Amazona ochrocephala and Nymphicus hollandicus where previous attempts with the same primers failed (Wang et al., 2007). Nevertheless, gender of Nymphicus hollandicus (Cerit and Avanus, 2007) and Amazona ochrocephala (Taylor and Parkin, 2008) was previously successfully determined with P2/P8 primer set.
In birds, feathers represent the most common sample for DNA isolation since sampling is easy and causes minimum pain if plucked or no pain at all if collected after molting (Seki, 2006; Leekaew et al., 2008). For that reason, we used feathers in this study as source of DNA for gender identification and proved its reliability in all sampled individuals. In addition, alternative sources of DNA, such as blood (Bush et al., 2000) or buccal swab (Seki, 2003) also gave reliable results (Table 1). In our study feces exerted only 25% success rate in sex determination, probably due to PCR inhibitors, such as pigments (Baignet et al., 2005), dead cells, RNA (Nielsen et al., 2000), or various microorganisms. Having in mind that Robertson et al. (1999) suggested avian feces as is good source of DNA when ecological questions need to be resolved in rapid and non-invasive manner, further research should be carried out to improve and simplify sexing of parrots when feces is sampled.
In this study both feathers, buccal swab and blood proved to be very reliable sources of genomic DNA with a 100% success rate. Still, for all sampling procedures of biological material, except for sampling feces and molted feathers, bird handling is necessary. Invasiveness of a procedure can be judged based on the degree of pain, tissue injury and duration of a procedure. Plucking feathers takes less time than the other two methods, and thus discomfort of individuals is considerably smaller (Directive 2010/63/EU). Thus, sampling of feathers is favored by several ornithological societies (McDonald and Griffith, 2011). Taking into account all above mentioned, it would be recommended that feathers are used as DNA source in all cases where possible.
The method for determining sex in parrots presented in this study is a reliable, economical, fast, simple and does not include aggressive sampling for DNA extraction, a fact highly important when dealing with bird species thatare endangered or on the CITES list.
This study was supported by the Ministry of Education and Science of Serbia, Grant No. III46002. We declare that the experiment comply with the current laws of Serbia, where it was performed.
ARNOLD, K. E., ORR, K. J. AND GRIFFITHS R., 2003. Primary sex ratios in birds: problems with molecular sex identification of undeveloped eggs. Mol. Ecol., 12:3451-3458.
BAIGNET, S., PETHERBRIDGE, L., HOWES, K., SMITH, L., CURRIE, R. AND NAIR, V., 2005. Absolute quantitation of Marek's disease virus genome copy number in chicken feather and lymphocyte samples using real-time PCR. J. Virol. Methods, 123: 53-56.
BELLO, N., FRANCINO, O. AND SANCHEZ, A., 2001. Isolation of genomic DNA from feathers. J. Vet. Diagn. Inv., 13: 162, 164
BIRDLIFE INTERNATIONAL, 2013. IUCN red list for birds. Downloaded from http://www.birdlife.org on 11/04/2013.
BROWN, M. B. AND BROWN, C. R., 2009. Blood sampling reduces annual survival in cliff swallows (Petrochelidon pyrrhonota). Auk, 126: 853-861.
BUSH, J. D., MILLER, M. P., PAXTON, E. P., SOGGE, M. K. AND KEIM, P., 2000. Genetic variation in the endangered Southwestern willow flycatcher. Auk,117:586-595.
CAHILL, A. J., WALKER, J. S. AND MARSDEN, S. J., 2006.Recovery within a population of the critically endangered citron-crested cockatoo Cacatua sulphurea citrinocristata in Indonesia after 10 years of international trade control. Oryx, 40: 1-7.
CASEY, A.E., JONES, K.L., SANDERCOCK, B.K. AND WISELY, S.M., 2009. Heteroduplex molecules cause sexing errors in a standard molecular protocol for avian sexing. Mol. Ecol. Resour., 9: 61-65.
CERIT, H. AND AVANUS, K., 2007. Sex identification in avian species using DNA typing methods. Wld. Poult. Sci. J., 63: 91-99.
COLLAR, N. J., 2000. Globally threatened parrots: criteria, characteristics and cures. Int. Zool. Jb., 37: 2l-35.
DIRECTIVE 2010/63/EU OF THE EUROPEAN PARLIAMENT AND OF THE COUNCIL of 22 September 2010 on the protection of animals used for scientific purposes. L 276/33, 20.10.2010, pages 65-68.
DONALD, P.F., 2007. Adult sex ratios in wild bird populations. Ibis, 149: 671-692
ELLEGREN, H., 1996. First gene on the avian W chromosome provides a tag for universal sexing on non-ratite birds. Proc. Roy. Soc. B, Biol. Sci., 263: 1635-1641.
ELLEGREN, H. AND SHELDON, B., 1997. New tools for sex identification and the study of sex allocation in birds. Trends Ecol. Evol., 12: 255-259.
FRIDOLFSSON, A. AND ELLEGREN, H., 1999. A simple and universal method for molecular sexing of non-ratite birds. J. Avian Biol., 30: 116-121.
GAUNT, A.S. AND ORING, L.W., 1999. Guidelines to the use of wild birds in research. Ornithol. Council, Washington.
GRIFFITHS, R., DAAN, S. AND DIJKSTRA, C., 1996. Sex identification in birds using two CHD genes. Proc. Roy. Soc. B, Biol. Sci., 263: 1251-1256.
GRIFFITHS, R., DOUBLE, M., ORR, K. AND DAWSON, R., 1998. A DNA test to sex most birds. Mol. Ecol., 7:1071-1075.
GOYMANN, W. AND WINGFIELD, J.C., 2004. Competing females and caring males. Sex steroids in African black coucals, Centropus grilli. Anim. Behav., 68: 733-740.
HANDEL, C.M., PAJOT L.M., TALBOT S.L. AND SAGE G.K., 2006. Use of buccal swabs for sampling DNA from nestling and adult birds. Wildl. Soc. Bull., 34: 1094-1100.
HOYSAK, D.J. AND WEATHERHEAD, P.J., 1991. Sampling blood from birds: a technique and an assessment of its effect. Condor, 93: 746-752.
IDAGHDOUR, Y., BRODERICK, D. AND KORRIDA, A.,2003. Faeces as a source of DNA for molecular studies in a threatened population of great bustards. Conserv. Genet., 4: 789-792.
ITO, H., SUDO-YAMAJI, A., ABE, M., MURASE, T. AND TSUBOTA, T., 2003. Sex identification by alternative polymerase chain reaction methods in falconiformes. Zool. Sci., 20: 339-344.
IUCN, 2012. The IUCN red list of threatened species. Version 2012.2. . Downloaded on 10 April 2013.
JENSEN, T., PERNASETTI, F. AND DURRANT, B., 2003.Condition for rapid sex determination in 47 avian species by PCR of genomic DNA from blood, shell- membrane blood vessels, and feathers. Zoo Biol., 22:561-571.
KAHN, N., JOHN, J. AND QUINN, T., 1998. Chromosome- specific intron size differences in the avian CHD gene provide an efficient method for sex identification in birds. Auk., 115: 1074-1078.
LANCTOT, R.B., 1994, Blood sampling in juvenile Buff- breasted Sandpipers: movement, mass change and survival. J. Field Ornithol., 65: 534-542.
LEEKAEW, P., SONGSERM, T., CHOOTHESA, A. AND BOONYAPRAKOB, U., 2008. A simple method to extract mitochondrial DNA in a non-invasive phylogenetic study of domestic native Thai ducks. Kasetsart J. (Nat. Sci.), 42: 41-50
MAHBOOB, S. AND NISA, Z., 2009. Diversity of avifauna of Trimmu Barrage, District Jhang, Punjab, Pakistan. Pakistan J. Zool., 41: 43-49.
McDONALD, P. AND GRIFFITH S.C., 2011, To pluck or not to pluck: the hidden ethical and scientific costs of relying on feathers as a primary source of DNA. J. Avian Biol., 42: 197-203.
MIYAKI, C., GRIFFITHS, R., ORR, K., NAHUM, L., PEREIRA, S. AND WAJNTAL, A., 1998. Sexidentification of parrots, toucans, and curassows by PCR: perspectives for wild and captive population studies. Zoo Biol., 17: 415-423.
NIELSEN, S., HOUE, H., THAMSBORG, S. AND BITSCH, V., 2000. Comparison of two enzyme-linked immunosorbent assays for serologic diagnosis of paratuberculosis (Johne's disease) in cattle using different subspecies strains of Mycobacterium avium. J. Vet. Diagn. Invest., 13: 164-166.
ONG, A. AND VELLAYAN, S., 2008. An evaluation of CHD- specific primer sets for sex typing of birds from feathers. Zoo Biol., 27: 62-69.
ROBERTSON, B. C., MINOT, E. O. AND LAMBERT, D. M.,1999. Molecular sexing of individual kakapo, Strigops habroptilus Aves, from faeces. Mol. Ecol., 8: 1347-1350.
ROBERTSON, B.C. AND GEMMELL, N. J., 2006. PCR-based sexing in conservation biology: wrong answers from an accurate methodology? Conserv. Genet., 7: 267-271.
SEKI, S. I., 2003. Molecular sexing of individual Ryukyu Robins Erithacus komadori using buccal cells as a non- invasive source of DNA. Ornithol. Sci., 2: 135-137.
SEKI, S.I., 2006. Application of molted feathers as noninvasive samples to studies on the genetic structure of pigeons (Aves: Columbidae). J. For. Res-Jpn., 11: 125-129.
SHELDON, L.D., CHIN E.H., GILL S.A., SCHMALTZ, G., NEWMAN, A.E.M. AND SOMA, K.K., 2008. Effects of blood collection on wild birds: an update. J. Avian Biol., 39: 369-378.
SNYDER, N., MCGOWAN, P., GILARDI, J. AND GRAJAL, A., 2000. Parrots. Status Survey and Conservation Action Plan 2000- 2004. IUCN, Gland, Switzerland and Cambridge, UK.
TAYLOR, T.D. AND PARKIN, D.T., 2008. Sex ratios observed in 80 species of parrots. J. Zool., 276: 89-94.
VUCICEVIC, M., STEVANOV-PAVLOVIC, M., STEVANOVIC, J., BOSNJAK, J., GAJIC, B., ALEKSIC, N. AND STANIMIROVIC, Z., 2012. Sex determination in 58 bird species and evaluation of CHD gene as a universal molecular marker in birds sexing. Zoo Biol., 31: 269-275.
WANG, L., CHEN, C., LEE, H., LI, S., LIR, J., CHIN, S., PU, C. AND WANG, C., 2007. Sexing a wider range of avian species based on two CHD1 introns with a unified reaction condition. Zoo Biol., 26: 425-431.
WILSON, M.H., KEPLER C.B., SNYDER N.F.R., DERRICKSON S.R., DEIN F.J., WILEY J.W., WUNDERLE J.M.Jr., LUGO A.E., GRAHAM D.L. AND TOONE W.D., 1994. Puerto Rican parrots and potential limitations of the metapopulation approach to species conservation. Conserv. Biol., 8:114-123.
YOUNG, A.M., HOBSON, E.A., LACKEY, L.B. AND WRIGHT, T.F., 2012. Survival on the ark: life-history trends in captive parrots. Anim. Conserv., 15: 28-53.
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|Author:||Bosnjak, Jasna; Stevanov-Pavlovic, Marija; Vucicevic, Milos; Stevanovic, Jevrosima; Simeunovic, Pred|
|Publication:||Pakistan Journal of Zoology|
|Date:||Jun 30, 2013|
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