Application of PCR-HRM method for microsatellite polymorphism genotyping in the LDHA gene of pigeons (Columba livia)

Magdalena Jedrzejczak-Silicka; Adam Lepczynski; Filip Gołębiowski; Daniel Dolata; Andrzej Dybus

doi:10.1371/journal.pone.0256065

Abstract

High-resolution melting (HRM) is a post-PCR method that allows to discriminate genotypes based on fluorescence changes during the melting phase. HRM is used to detect mutations or polymorphisms (e.g. microsatellites, SNPs, indels). Here, the (TTTAT)_3-5 microsatellite polymorphism within intron 6 of the LDHA gene in pigeons was analysed using the HRM method. Individuals (123 homing pigeons) were genotyped using conventional PCR. Birds were classified into groups based on genotype type and the results were tested by qPCR-HRM and verified using sequencing. Based on the evaluated protocol, five genotypes were identified that vary in the number of TTTAT repeat units (3/3, 4/4, 3/4, 4/5, and 5/5). Sequencing have confirmed the results obtained with qPCR-HRM and verified that HRM is a suitable method for identification of three-allele microsatellite polymorphisms. It can be concluded that the high-resolution melting (HRM) method can be effectively used for rapid (one-step) discrimination of the (TTTAT)_3-5 microsatellite polymorphism in the pigeon’s LDHA gene.

Citation: Jedrzejczak-Silicka M, Lepczynski A, Gołębiowski F, Dolata D, Dybus A (2021) Application of PCR-HRM method for microsatellite polymorphism genotyping in the LDHA gene of pigeons (Columba livia). PLoS ONE 16(8): e0256065. https://doi.org/10.1371/journal.pone.0256065

Editor: Hoh Boon-Peng, UCSI University, MALAYSIA

Received: July 19, 2020; Accepted: August 1, 2021; Published: August 19, 2021

Copyright: © 2021 Jedrzejczak-Silicka et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Data Availability: All relevant data are within the paper and its Supporting Information files.

Funding: The authors received no financial support for the research, authorship, and publication of this article. FG is affiliated with QIAGEN, and DD is affiliated with Bio-Techne, both of which are commercial companies. FG and DD provided technical support (Rotor-Gene Q Series Software 2.3.1), as well as other contributions detailed in the Author Contributions section. QIAGEN and Bio-Techne had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: FG is affiliated with QIAGEN, and DD is affiliated with Bio-Techne, both of which are commercial companies. This does not alter our adherence to PLOS ONE policies on sharing data and materials. There are no patents, products in development or marketed products associated with this research to declare.

Introduction

LDHA–lactate dehydrogenase isoform A (specific for muscle) is a member of a larger LDH gene family encoding L-lactate dehydrogenase (LDH, EC.1.1.1.27) [1,2]. Lactate dehydrogenase regulates aerobic and anaerobic metabolism, which has an significant impact on the physiological condition of the body, e.g. muscle endurance, recovery, aerobic capacity, survivability during racing competitions as well as overall physiological performance [1–4]. LDHA plays a crucial role as a coenzyme in the interconversion of pyruvate and lactate with nicotinamide dinucleotide [3,5,6]. The latest research suggest that lactate is a specific “cellular fuel”, including hippocampal nerve cells that are responsible for consolidating information from short-term to long-term memory, and spatial memory that determines navigation ability [3,7–9].

In 2002 for the first time the presence of LDHA gene polymorphism in pigeons was described [10]. Subsequent studies demonstrated that allele A of the LDHA gene (g.2582481G>A) was more frequent in the groups of pigeons with elevated homing performance [11,12]. The analysis of the effect of LDHA gene polymorphism (SNP, g.2582481G>A) on the racing performance of homing pigeons showed the difference in the value of ace points between animals with GG and GA genotypes. The study showed that allele A could be associated with better results of pigeons in competition flights [13,14]. Therefore, the LDHA gene is called the “Speed Gene” by commercial genotyping services. The (TTTAT)_3-5 microsatellite polymorphism within intron 6 of the LDHA gene in pigeons has been described for the first time by Ramadan et al. [7] who found three different allele lengths (GenBank: AB744076, AB744077, AB744078) [3,7]. Ramadan et al. [3] found in Japanese and Egyptian pigeon populations that individuals carrying the LDHA S+ genotype (all genotypes containing minor allele S, i.e. 3 repeats, were classified as the S+) had higher EBV (estimated breeding value) resulting i.a. in greater survivability. Since Ramadan and co-workers [3] published their findings no other works has focused on that (TTTAT)_3-5 microsatellite polymorphism in intron 6 of the LDHA gene.

Microsatellites (called simple sequence repeats − SSRs or short tandem repeats − STRs) are DNA segments composed of short (2–6 nucleotides), tandemly repeated (to over 200 times) motifs in the same orientation [15–18]. Short tandem repeats are often found in both intergenic and intragenic regions (rarely occurring within coding regions; trinucleotide repeats in or near genes are associated with certain inherited disorders) in prokaryotes and eukaryotes, including humans (accounting for approximately 3% of total human genome) [17–19]. The nature of microsatellites is complex—STRs are highly mutable (duplicative mutation rates range from 1 × 10⁻³ to 1 × 10⁻⁴ per generation) and demonstrate variability in length and sequence composition [17,18,20]. In contrast, other types of mutations (e.g., deletions, substitutions) are 4–5 times rarer with an estimated mutation rate of about 1.1 × 10^-n per site per generation [18,20]. The importance of microsatellite DNA as a powerful marker with a broad spectrum of applications should not be underestimated [21]. Microsatellites are widely used as valuable elements in population genetics because SSR markers are highly variable even cross closely related taxa [21]. Moreover, data obtained from microsatellite analyses have confirmed that individual microsatellites tend to be more polymorphic, and thus more informative, providing greater resolution in genetic studies than other molecular markers, including SNPs [21]. For example, Y-chromosome short tandem repeats (Y-STRs) are powerful human genome marker and have been used for many years in forensic practice [22]. The traditional approach used in microsatellites genotyping procedures is based on locus-specific polymerase chain reaction (PCR) for product amplification and polyacrylamide gel electrophoresis for genotypes identification [22]. Since the late 1990s, short tandem repeats (STRs) have been analysed using capillary electrophoresis (CE)–an automated technique utilizing laser-induced fluorescence to identify PCR products (amplicons are generated using fluorescence-labelled primers). However, studying microsatellites in the genome are more difficult compared to other common sequences.

Importantly, replication in microsatellite studies occurs during in vitro amplification of microsatellite sequences, resulting in the appearance of “stutter bands” or “shadow bands” in agarose electrophoresis or additional stutters picks in capillary electrophoresis [23–28]. “Stutter bands” may appear during the amplification of long and short tandem repeats [24,29–31]. The molecular mechanism of Taq DNA polymerase slippage during the amplification of repetitive DNA sequences and accumulation of products of different sizes (e.g. slipped strand mispairing; SSM) is not well explained [24,32]. Hommelsheim et al. [32] has found that polymerase DNA dissociates from the template because the appearance of hairpin loop structures (slippage). Due to the slippage process during the first PCR replication cycle [31], the obtained fragments act as megaprimers that randomly anneal with other sequences at variable positions (insertion or deletion of repeats may be occur). They are subsequently amplified by DNA polymerase, resulting in artifact formation that serve as templates in the subsequent amplification cycles, eventually including cause a ladder effect [24,32,33]. Slippage might take place at the active site of the enzyme or before substrate binding to the enzyme [34].

Moreover, besides of “stutter bands” there is another PCR artifacts class that must be taken into consideration–the heteroduplexes. As was stated by Kulibaba and Liashenko [35] amplification of microsatellite loci is usually accompanied by the formation of many additional fragments (artifacts) − heteroduplex DNA in the course of PCR is frequent. A heteroduplex is formed by the annealing of two individual single-stranded DNA in which antiparallel chains have different origin (derived from different alleles). In addition, mentioned artifacts are often situated near the target ones and cause difficulties in performing the precise genotyping [35]. On the other hand, sequencing allows to detect the stutter bands in PCR products, i.e. different product lengths due to an error in the number of repeat units [24].

We suppose that the reason for the lack of analysis of (TTTAT)_3-5 microsatellite polymorphism in intron 6 of the LDHA gene polymorphism is caused by conventional PCR limitation. The main difficulty is the heteroduplexes formation during PCR reaction in case of heterozygotes samples and problems in the interpretation of the results of PCR products after agarose electrophoresis. Due to mentioned problems we applied the high resolution melting (HRM) method to detect the (TTTAT)_3-5 microsatellite polymorphism in intron 6 of the LDHA gene as an alternative that offers easier results interpretation based on melting curves that directly translates into labour efficiency and reduction of time consumption. Based on the above information the aim of the study was to present a new approach to microsatellite polymorphism genotyping in the LDHA gene using HRM method with final results verification by DNA sequencing method.

Methods

Ethical approval

This study was carried out in strict accordance with the recommendations of the National Ethics Committee on Animal Experimentation. The protocol was approved by the Local Ethics Committee for Animal Testing of the West Pomeranian University of Technology in Szczecin (Protocol Number: 36/2012).

DNA extraction

The present study comprised a total of 123 racing pigeons (from two racing lofts located in the Lubusz Province, Poland). Blood samples of all individuals were collected from the medial metatarsal vein into collection tubes containing anticoagulant (K₃EDTA). Genomic DNA was extracted from 5 μl of whole peripheral blood using the MasterPure^TM DNA Purification Kit for Blood version II (Epicentre Biotechnologies, Madison, WI, USA), according to the vendor’s protocol.

Genotyping with conventional PCR and gel electrophoresis

The (TTTAT)_3-5 microsatellite polymorphism within intron 6 of the LDHA gene was analysed using conventional PCR reaction. PCR primers (Table 1) used in present study were designed based on the genomic sequence (GenBank accession no. NW_004973198.1, ref. 7) using Primer 3 software (https://primer3.ut.ee/). PCR reaction mixtures contained ~80 ng of genomic DNA, 15 pmol of each primer, 1 x PCR buffer, 1.5 mM MgCl₂, 200 μM dNTP, 0.4 unit of Taq polymerase (Eurx, Gdańsk, Poland) and nuclease-free water (AppliChem, Darmstadt, German) in a total volume of 15 μl. The PCR amplification program was as follows: 5 min initial denaturation at 94°C followed by 35 cycles (denaturation at 94°C for 30 s, primer annealing at 61°C for 30 s and product synthesis at 72°C for 30 s) and final elongation at 72°C for 5 min (Biometra T-Personal thermocycler, Biometra GmbH, Göttingen Germany). Finally, PCR products were separated by horizontal electrophoresis (80 V, 400 mA, 240 min; Mini-Sub Cell GT Systems, Bio-Rad, Hercules, CA, United States) on a 5% agarose gel (Norgen Biotek Corp., Canada) [4].

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Table 1. The new primer set flanking the (TTTAT)_3-5 microsatellite located within the intron 6 of the LDHA gene.

https://doi.org/10.1371/journal.pone.0256065.t001

Urea-PAGE electrophoresis

After PCR amplification, samples were loaded onto a denaturing urea 20% polyacrylamide gels and electrophoretically separated for one hour at 20 W using Mini-PROTEAN Tetra cell (Bio-Rad, Hercules, CA, USA) electrophoretic chamber. Then, the gel was washed with 1 x TBE (ChemLand, Stargard Szczecinski, Poland) for about 15 min to remove the urea and soaked in 0.5 μg/ml ethidium bromide (AppliChem GmbH, Darmstadt, Germany) in aqueous solution for 45 min. The PCR products were examined under the UV light using UV-Transilluminator (Vilber Lourmat, Marne-la-Vallee Cedex, France) and each band of heterozygotes samples was isolated separately from the gel. DNA from desired amplicons were isolated by crush-and-soak method as was described elsewhere [36,37]. Concentration of each DNA sample was determined using the Quant-iT^TM dsDNA BR Assay Kit and a Qubit fluorometer (Invitrogen, Carlsbad, CA, USA). Afterwards, DNA samples were concentrated using Clean-Up Concentrator Kit (A&A Biotechnology, Gdańsk, Poland) following the vendor’s instructions and delivered to a custom DNA sequencing service.

Moreover, due to heteroduplexes DNA (in the course of PCR) urea-PAGE was conducted under identical experimental conditions as described above. Resulted gel was washed with 10% ethanol solution (Chempur, Piekary Slaskie, Poland) for 15 minutes and subsequently soaked in 1% nitric acid solution (ChemLand, Stargard Szczecinski, Poland) for 10 minutes. After washing step, gel was soaked in 0.2% silver nitrate solution with 0.075% formaldehyde solution (ChemLand, Stargard Szczecinski, Poland) for 30 minutes. Next gel was washed in 10% acetic acid solution (Chempur, Piekary Slaskie, Poland) for 10 minutes and subsequently washed twice in miliQ water. Immediately after staining gel image acquisition was performed using a GS-800™ Calibrated Densitometer (Bio-Rad, Hercules, CA, USA) with the aid of Quantity One^® 1-D image analysis software (Bio-Rad, Hercules, CA, USA).

qPCR-HRM analysis

Individuals (genotyped using conventional PCR) were classified into five groups based on genotype type (3/3, 4/4, 3/4, 4/5, 5/5) and the results were tested by qPCR-HRM. PCR master mixtures contained 100 ng of genomic DNA (all gDNA samples were quantified using The Quant-iT^TM dsDNA Assay Kit; Life Technologies, Carlsbad, CA, USA), 250 nM of each primer, 4 μl of 5x AmpliQ HOT EvaGreen HRM Mix (Novazym, Poznań, Poland) and nuclease-free water (AppliChem GmbH, Darmstadt, Germany) in a total volume of 20 μl. The qPCR-HRM analysis was performed a Rotor-Gene Q instrument (QIAGEN GmbH, Hilden, Germany). The qPCR-HRM thermal profile was as follows: 15 min at 95°C for initial denaturation, subsequent 40 cycles (denaturation at 95°C for 15 s, primer annealing at 61°C for 20 s and product synthesis at 72°C for 20 s) and final elongation at 72°C for 1 min for complete product extension. Final elongation was then followed by pre-hold temperatures − 95°C for 15 s and 50°C for 15 s for product re-association and heteroduplex formation. Fluorescence data acquisition (melting curves) was performed during the melting phase (temperature change from 70 to 95°C at a transition rate of 0.1°C each step). High resolution melting curve analysis was performed using the Rotor-Gene Q Series Software 2.3.1 (QIAGEN GmbH, Hilden, Germany).

Verification by DNA sequencing

PCR amplicons representing all identified genotypes (3/3, 4/4, 3/4, 4/5, 5/5) and additional amplicons (results obtained for (TTTAT)₃/(TTTAT)₄ and (TTTAT)₄/(TTTAT)₅ heterozygotes) isolated from urea-PAA gels were sequenced at the forward and reverse direction by each respective primer (Table 1), ABI Prism^™ BigDye^™ Terminator Cycle Sequencing Kit and ABI Prism^™ Sequencer (Thermo Fisher Scientific, Waltham, Massachusetts, USA) by a custom DNA sequencing service (Genomed S.A., Warsaw, Poland). Three independent experiments were conducted to confirm the results obtained by sequencing. Sequences of all five samples were analysed using the BioEdit Sequence Alignment Editor (https://bioedit.software.informer.com/7.2/).

Results and discussion

After PCR reaction, the obtained amplicons spanning the (TTTAT)_3-5 microsatellite polymorphism within intron 6 of the LDHA gene were separated on a high-resolution agarose gel and the presence of five genotypes (of six potential) was confirmed in the analysed population of homing pigeons (Fig 1A and 1B). Three homozygous genotypes (3/3, 4/4, 5/5) were visualised in agarose electrophoresis as a single amplicons. In contrast, two heterozygous genotypes 3/4, 4/5 (genotype 3/5 was affirmed of be absent in the examined individuals of homing pigeons) identified in agarose electrophoresis demonstrated two amplicons corresponded to alleles of different length and additional amplicon (heteroduplex) above PCR product (Fig 1A–heterozygote samples–C and D, additional amplicons–heteroduplexes were marked by stars). Due to additional band in heterozygous samples additional analysis was conducted to eliminate doubts about actual length of obtained PCR products. Moreover, chosen urea-PAGE method gave possibility to confirm our suspicious about the origin of unwanted amplicons in heterozygous samples. Result of electrophoresis under denaturing condition clearly confirmed five genotypes with two heterozygotes (Fig 1B).

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Fig 1.

PCR analyses of five identified genotypes (A-E) using agarose gel electrophoresis (A) and urea-PAGE (B). Lines: M. O’RangeRuler 20 bp DNA Ladder (Thermo Scientific). A. (TTTAT)₃/(TTTAT)₃ homozygote. B. (TTTAT)₄/(TTTAT)₄ homozygote. C. (TTTAT)₃/(TTTAT)₄ heterozygote. D. (TTTAT)₄/(TTTAT)₅ heterozygote. E. (TTTAT)₅/(TTTAT)₅ homozygote. PCR plausible heteroduplexes marked by stars.

https://doi.org/10.1371/journal.pone.0256065.g001

Simultaneously, sequencing method as a gold standard was performed to validate the results obtained by PCR. Three samples from each group (five groups, A-E) were arbitrarily selected from the whole analysed group and subjected to DNA sequencing. The results of sequencing were presented in Fig 2. The sequencing analyses were performed for each PCR product (left panel of Fig 2) and for each amplicon isolated out for polyacrylamide gels (right panel of Fig 2). Clearly, such proceedings demonstrated DNA sequence variation in the number of TTTAT repeat motifs. Based on sequencing, it was stated that samples A, B and E were homozygotes and contained (TTTAT)₃, (TTTAT)₄ and (TTTAT)₅ repeat units, respectively. The two remaining samples, C and D, were identified as (TTTAT)₃/(TTTAT)₄ and (TTTAT)₄/(TTTAT)₅ heterozygotes, respectively. The most importantly the length of alleles (number of TTTAT repeat motif) of C and D samples were verified.

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Fig 2. The sequencing results for the (TTTAT)_3-5 microsatellite polymorphism in the LDHA gene.

A. (TTTAT)₃/(TTTAT)₃ homozygote. B. (TTTAT)₄/(TTTAT)₄ homozygote. C. (TTTAT)₃/(TTTAT)₄ heterozygote. D. (TTTAT)₄/(TTTAT)₅ heterozygote. E. (TTTAT)₅/(TTTAT)₅ homozygote.

https://doi.org/10.1371/journal.pone.0256065.g002

Finally, preliminary results obtained using conventional PCR and sequencing were tested using the qPCR-HRM method. Based on melting curve analysis (MCA) five different melting profiles were recognized as a result of disassociation (melting) behaviour of each sample (Fig 3A and 3B). The normalized HRM profiles and the difference graph (sample A genotype 3/3 was selected as reference) clearly show the five different melting profiles (A to E, Fig 3). HRM results showed no discrepancy between the identified alleles/genotypes from PCR and qPCR-HRM techniques.

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Fig 3. Results of qPCR-HRM analysis.

A. The normalized HRM profile of five identified genotypes. B. The difference graph (sample A genotype 3/3 was selected as reference). A. (TTTAT)₃/(TTTAT)₃ homozygote. B. (TTTAT)₄/(TTTAT)₄ homozygote. C. (TTTAT)₃/(TTTAT)₄ heterozygote. D. (TTTAT)₄/(TTTAT)₅ heterozygote. E. (TTTAT)₅/(TTTAT)₅ homozygote.

https://doi.org/10.1371/journal.pone.0256065.g003

Results obtained in conventional PCR and agarose electrophoresis analyses (Fig 1A) literally presented their limitations. Result of homozygote samples can be easily read, but in case of heterozygote samples the interpretation is limited due to additional amplicons (additional amplicons were marked with the asterisk; Fig 1A). Because the additional amplicons were observed only in heterozygotes we suggested that those amplicons are heteroduplexes. The heteroduplex is a double stranded DNA molecule that is formed by the annealing of two individual single-stranded DNA (derived from different alleles) of different repeat size during PCR. Presented findings correspond to Kulibaba and Liashenko [35] results. The appearance of additional fragments—heteroduplexes in heterozygous samples are common. The reason for heteroduplexes formation is presence of different in length alleles that exhibit different electrophoretic mobilities, that is why those structure are formed only in the case of heterozygotes [35]. Worth mentioning is fact that demonstrated artifacts are often situated near the target ones and cause difficulties in performing the precise genotyping [35], thus the main problem in this type of research is the specificity of the described polymorphism.

In our study solution of the problem described above was the application of the urea-PAGE to verify results observed in conventional PCR and agarose gel electrophoresis. As was presented in Fig 1B only two amplicons of different sizes were observed in denaturing PAGE, thus showing that the additional amplicons found in sample D and E in the agarose gel electrophoresis, are heteroduplexes. Moreover, precise determination of product lengths and in the number of TTTAT repeat units was obtained by DNA sequencing. Using the traditional Sanger sequencing method as gold standard in determination of analysed sequences. The microsatellite polymorphism can be also analysed using the traditional Sanger sequencing method, but microsatellite polymorphism analysis is challenging even for this technique. In our study sequencing of whole PCR product of heterozygotes did not solve the problem (left panel of Fig 2). In this type of microsatellite polymorphism it is necessary to analyse single amplicons isolated from the gel. Use of the agarose gel in this case did not provide sufficient resolution, especially in heterozygote samples, thus polyacrylamide electrophoresis was performed. This fact caused implementation of extensive laboratory procedures, low effectiveness, time-consumption methods and higher costs [38–40].

In order to avoid the limitations found in this study the HRM method was used for microsatellite polymorphism genotyping in the LDHA gene (Fig 3). Although the HRM is a post-PCR analysis (the melting pattern of the amplicons after products generation), in this study each sample represents one of five genotype. The interpretation of the results obtained via HRM is much easier than in conventional PCR and agarose electrophoresis analyses. Moreover, HRM method is much more efficient and less time-consuming that conventional methods. Hence, an accurate, powerful tool for genotype discrimination/genetic screening is needed. The high resolution melting analysis (HRM) has become an attractive and alternative method for determining different various genetic variations such as SNPs, insertions/deletions, microsatellite markers, DNA methylation, but also unknown DNA polymorphisms. HRM analysis is a one-tube and post-PCR method based on the intercalation of fluorescence dye into double-strand DNA. Fluorescence changes during dsDNA melting enable to discriminate genotypes [22]. High-resolution melting analysis is a relatively easy and rapid (the entire procedure can be completed in 1.5–2 hours), one-step, cost-effective application [22,41,42]. Moreover, it was found that STRs analysed by HRM had more genotypes than in capillary electrophoresis [22,41,42]. Demonstrated in this study method gave possibility to rapid discrimination of the (TTTAT)_3-5 microsatellite polymorphism in the pigeon’s LDHA gene, that may serve as an rapid test for the commercial genotyping services. We suspect that microsatellite nature of analysed polymorphism in the LDHA gene caused lack of results in different populations of pigeons. Only Japanese and Egyptian population have been studied by Ramadan and colleagues [3,7] who presented four different genotypes (3/3, 4/4, 3/4, 4/5 repeats units for Japanese and 3/3, 4/4, 3/4, 5/5 for Egyptian birds) in the group of homing pigeons. Presented alternative approach–HRM analysis can potentially contribute to filling the knowledge gap about the frequency of LDHA microsatellite polymorphisms in pigeon populations and their potential effect on phenotypes.

Conclusions

Herein, the (TTTAT)_3-5 microsatellite polymorphism within intron 6 of the LDHA gene was analysed using the HRM method. The usability of HRM analysis of the selected microsatellite polymorphism was confirmed and the problem of the artifacts–heteroduplexes in heterozygote samples, which appear in the conventional amplification process was solved. The evaluated method can potentially contribute to filling the knowledge gap about the frequency of LDHA microsatellite polymorphisms in pigeon populations and their potential effect on phenotypes. Finally, provides a possibility for researches and breeders to see the complete picture of the significance of the LDHA gene in homing as well as non-homing pigeons.

Supporting information

S1 Fig. The original gel image of PCR analyses of five identified genotypes using agarose gel electrophoresis.

From the left: O’RangeRuler 20 bp DNA Ladder (Thermo Scientific); (TTTAT)₃/(TTTAT)₃ homozygote; (TTTAT)₄/(TTTAT)₄ homozygote; (TTTAT)₃/(TTTAT)₄ heterozygote; (TTTAT)₄/(TTTAT)₅ heterozygote; (TTTAT)₅/(TTTAT)₅ homozygote; O’RangeRuler 20 bp DNA Ladder (Thermo Scientific), respectively.

https://doi.org/10.1371/journal.pone.0256065.s001

(TIF)

S2 Fig. The original urea-polyacrylamide gel electrophoresis of PCR analyses of five identified genotypes using agarose gel electrophoresis.

From the left: O’RangeRuler 20 bp DNA Ladder (Thermo Scientific); (TTTAT)₃/(TTTAT)₃ homozygote; (TTTAT)₄/(TTTAT)₄ homozygote; (TTTAT)₃/(TTTAT)₄ heterozygote; (TTTAT)₄/(TTTAT)₅ heterozygote; (TTTAT)₅/(TTTAT)₅ homozygote, respectively.

https://doi.org/10.1371/journal.pone.0256065.s002

(TIF)

S3 Fig. The original image of qPCR-HRM analysis.

The normalized HRM profile of five identified genotypes.

https://doi.org/10.1371/journal.pone.0256065.s003

(TIF)

S4 Fig. The original image of qPCR-HRM analysis.

The difference graph (sample A genotype 3/3 was selected as reference).

https://doi.org/10.1371/journal.pone.0256065.s004

(TIF)

S5 Fig. The original image of sequencing results for the (TTTAT)_3-5 microsatellite polymorphism in the LDHA gene (direct PCR).

https://doi.org/10.1371/journal.pone.0256065.s005

(TIF)

S6 Fig. The original image of sequencing results for the (TTTAT)_3-5 microsatellite polymorphism in the LDHA gene (amplicons isolated from urea-PAGE gel).

https://doi.org/10.1371/journal.pone.0256065.s006

(TIF)

References

1. Lupiáñez JA, Salguero LG, Torres NV, Peragón J, Meléndez-Hevia E. Metabolic support of the flight promptness of birds. Comp. Biochem. Physiol. B Biochem. Mol. Biol. 1996; 11: 439–443.
- View Article
- Google Scholar
2. Mannen H, Tsoi SC, Krushkal JS, Li WH, Li SS. The cDNA cloning and molecular evolution of reptile and pigeon lactate dehydrogenase isozymes. Mol. Biol. Evol. 1997; 14: 1081–1087. pmid:9364765
- View Article
- PubMed/NCBI
- Google Scholar
3. Ramadan S, Miyake T, Yamaura J, Inoue-Murayama M. LDHA gene is associated with pigeon survivability during racing competitions. PLoS ONE. 2018; 13: e0195121. pmid:29775483
- View Article
- PubMed/NCBI
- Google Scholar
4. Jedrzejczak-Silicka M., Yu YH., Cheng YH., Dybus A. The influence of LDHA gene polymorphism on relative level of its expression in racing pigeons. Acta Sci. Pol. Zootechnica. 2018; 17: 9–16.
- View Article
- Google Scholar
5. Van Hall G, Gonzaâlez-Alonso J, Sacchetti M, Saltin B. Skeletal muscle substrate metabolism during exercise: methodological considerations. Proc. Nutr. Soc. 1999; 58: 899–912. pmid:10817157
- View Article
- PubMed/NCBI
- Google Scholar
6. Van Hall G. Lactate as a fuel for mitochondrial respiration. Acta Physiol. Scand. 2000; 168: 643–656. pmid:10759601
- View Article
- PubMed/NCBI
- Google Scholar
7. Ramadan S, Yamaura J, Miyake T, Inoue-Murayama M. DNA polymorphism within LDHA-A gene in pigeon (Columba livia). J. Poult. Sci. 2013; 50: 194–197.
- View Article
- Google Scholar
8. Newman LA, Korol DL, Gold PE. Lactate produced by glycogenolysis in astrocytes regulates memory processing. PloS One. 2011; 6: e28427. pmid:22180782
- View Article
- PubMed/NCBI
- Google Scholar
9. Proia P, Di Liegro CM, Schiera G, Fricano A, Di Liegro I. Lactate as a metabolite and a regulator in the central nervous system. Int. J. Mol. Sci. 2016; 17: 1450. pmid:27598136
- View Article
- PubMed/NCBI
- Google Scholar
10. Dybus A, Kmieć M. PCR-RFLPs within the lactate dehydrogenase (LDH-A) gene of the domestic pigeon (Columba livia var. domestica). J. Appl. Genet. 2002; 43: 501–504. pmid:12441634
- View Article
- PubMed/NCBI
- Google Scholar
11. Dybus A, Pijanka J, Cheng CH, Sheen F, Grzesiak W, Muszyńska M. Polymorphism within the LDHA gene in the homing and non-homing pigeons. J. Appl. Genet. 2006; 47: 63–66. pmid:16424611
- View Article
- PubMed/NCBI
- Google Scholar
12. Dybus A. Nucleotide sequence variation of lactate dehydrogenase A and B genes in pigeons. 2009. Post-doctoral Thesis. The Publishing House of the West Pomeranian University of Technology in Szczecin.
- View Article
- Google Scholar
13. Proskura WS, Cichoń D, Grzesiak W, Zaborski D, Sell-Kubiak E, Cheng Y-H, et al. Single nucleotide polymorphism in the LDHA gene as a potential marker for the racing performance of pigeons. J. Poult. Sci. 2014. 51: 364–368.
- View Article
- Google Scholar
14. Proskura WS, Dybus A, Łukaszewicz A, Hardziejewicz E, Pawlina E. The single nucleotide polymorphisms in lactate dehydrogenase-A (LDHA) and feather keratin (F-KER) genes and racing performance of domestic pigeon. Zesz. Nauk. UP Wroc. Biol. Hod. Zwierz. 2015; 76: 37–42.
- View Article
- Google Scholar
15. Gebhardt C. Molecular markers, maps and population genetics. In: Vreugdenhil D, Bradshaw J, Gebhardt C, Govers F, Taylor M, MacKerron D, Ross H. Potato biology and biotechnology. Advances and perspectives. Elsevier Science; 2007. pp. 77–89.
- View Article
- Google Scholar
16. Dardé ML, Ajzenberg D, Smith J. Population structure and epidemiology of Toxoplasma gondii. In: Weiss LM, Kim K. Toxoplasma Gondii. The model apicomplexan: perspectives and methods. Academic Press; 2007, pp. 49–80. https://doi.org/10.1016/B978-012369542-0/50005-2
17. McMahon K, Paciorkowski AR, Walters-Sen LC, Milunsky JF, Bassuk A, Darbro B, et al. Neurogenetics in the genome era. In: Swaiman K, Ashwal S, Ferriero D, Schor N, Finkel R, Gropman A, Pearl P, Shevell M. Swaiman’s pediatric neurology. Elsevier; 2017, pp. 257–267. https://doi.org/10.1016/B978-0-323-37101-8.00034–5
18. Herrera RJ, Bertrand RG. The nature of evolution. In: Herrera RJ, Bertrand RG. Ancestral DNA, human origins, and migrations. Academic Press; 2018, pp. 1–31. https://doi.org/10.1016/B978-0-12-804124-6.00001-X
19. Turnpenny P, Elladr S. Emery’s elements of medical genetics. 15^th ed. Elsevier; 2017.
20. Brinkmann B, Klintschar M, Neuhuber F, Huhe J, Rolf B. Mutation rate in human microsatellites: Influence of the structure and length of the tandem repeat. Am. J. Hum. Genet. 1998; 62: 1409–15. pmid:9585597
- View Article
- PubMed/NCBI
- Google Scholar
21. Arthofer W, Steiner FM, Schlick-Steiner BC. Rapid and cost-effective screening of newly identified microsatellite loci by high-resolution melting analysis. Mol. Genet. Genomics 2011; 286: 225–235. pmid:21847526
- View Article
- PubMed/NCBI
- Google Scholar
22. Deng JQ, Liu BQ, Wang Y, Liu W, Cai JF, Long R, et al. Y-STR genetic screening by high-resolution melting analysis. Genet. Mol. Res. 2016; 15: gmr.15017266. pmid:26909950
- View Article
- PubMed/NCBI
- Google Scholar
23. Jennings TN, Knaus BJ, Mullins TD, Haig SM, Cronn RC. Multiplexed microsatellite recovery using massively parallel sequencing. Mol. Ecol. Resour. 2011; 1:1060–7. pmid:21676207
- View Article
- PubMed/NCBI
- Google Scholar
24. Hosseinzadeh-Colagar A, Haghighatnia MJ, Amiri Z, Mohadjerani M, Tafrihi M. Microsatellite (SSR) amplification by PCR usually led to polymorphic bands: Evidence which shows replication slippage occurs in extend or nascent DNA strands. Mol. Biol. Res. Commun. 2016; 5: 167–174. pmid:28097170
- View Article
- PubMed/NCBI
- Google Scholar
25. Ellegren H. Microsatellites: Simple sequences with complex evolution. Nat. Rev. Genet. 2004; 5: 435–445. pmid:15153996
- View Article
- PubMed/NCBI
- Google Scholar
26. Ogliari JB, Boscariol RL, Camargo LEA. Optimization of PCR amplification of maize microsatellite loci. Genet. Mol. Biol. 2000; 23: 395–398.
- View Article
- Google Scholar
27. Brookes C, Bright JA, Harbison S, Buckleton J. Characterising stutter in forensic STR multiplexes. Forensic Sci. Int. Genet. 2012; 6: 58–63. pmid:21388903
- View Article
- PubMed/NCBI
- Google Scholar
28. Harr B, Zangerl B, Schlötterer C. Removal of microsatellite interruptions by DNA replication slippage: phylogenetic evidence from Drosophila. Mol. Biol. Evol. 2000; 17: 1001–1009. pmid:10889213
- View Article
- PubMed/NCBI
- Google Scholar
29. Castillo-Lizardo M, Henneke G, Viguera E. Replication slippage of the thermophilic DNA polymerases B and D from the Euryarchaeota Pyrococcus abyssi. Front. Microbiol. 2014; 5: 1–10. pmid:24478763
- View Article
- PubMed/NCBI
- Google Scholar
30. Ananda G, Walsh E, Jacob KD, Krasilnikova M, Eckert KA, Chiaromonte F, et al. Distinct mutational behaviors differentiate short tandem repeats from microsatellites in the human genome. Genome Biol. Evol. 2013; 5: 606–620. pmid:23241442
- View Article
- PubMed/NCBI
- Google Scholar
31. Gemayel R, Vinces MD, Legendre M, Verstrepen KJ. Variable tandem repeats accelerate evolution of coding and regulatory sequences. Annu. Rev. Genet. 2010; 44: 445–477. pmid:20809801
- View Article
- PubMed/NCBI
- Google Scholar
32. Hommelsheim CM, Frantzeskakis L, Huang M, Ülker B. PCR amplification of repetitive DNA: a limitation to genome editing technologies and many other applications. Sci. Rep. 2014; 4: 5052. pmid:24852006
- View Article
- PubMed/NCBI
- Google Scholar
33. Riet J, Ramos LRV, Lewis RV, Marins LF. Improving the PCR protocol to amplify a repetitive DNA sequence. Genet. Mol. Res. 2017; 16: gmr16039796. pmid:28973773
- View Article
- PubMed/NCBI
- Google Scholar
34. Kunkel TA, Bebenek K. DNA replication fidelity. Annu. Rev. Biochem. 2000; 69: 497–529. pmid:10966467
- View Article
- PubMed/NCBI
- Google Scholar
35. Kulibaba RA, Liashenko YV. Influence of the PCR artifacts on the genotyping efficiency by the microsatellite loci using native polyacrylamide gel electrophoresis. Cytol. Genet. 2016; 50: 162–167.
- View Article
- Google Scholar
36. Moorey SE, Walker BN, Elmore MF, Elomer JB, Rodning SP, Biase FH. Rewiring of gene expression in circulating white blood cells is associated with pregnancy outcome in heifers (Bos taurus). Sci. Rep. 2020; 10: 16786. pmid:33033295
- View Article
- PubMed/NCBI
- Google Scholar
37. Green MR, Sambrook J. Isolation of DNA fragments from polyacrylamide gels by the crush and soak method. Cold Spring Harb. Protoc. 2019;754. pmid:30710028
- View Article
- PubMed/NCBI
- Google Scholar
38. Vianna JA, Noll D, Mura-Jornet I, Valenzuela-Guerra P, González-Acuña D, Navarro C, et al. Comparative genome-wide polymorphic microsatellite markers in Antarctic penguins through next generation sequencing. Genet. Mol. Biol. 2017; 40: 676–687. pmid:28898354
- View Article
- PubMed/NCBI
- Google Scholar
39. Litt M, Hauge X, Sharma V. Shadow bands seen when typing polymorphic dinucleotide repeats: some causes and cures. BioTechniques. 1993; 15: 280–284. pmid:8373596
- View Article
- PubMed/NCBI
- Google Scholar
40. Demir G, Alkan C. Characterizing microsatellite polymorphisms using assembly-based and mapping-based tools. Tur. J. Biol. 2019; 43: 264–273. pmid:31496881
- View Article
- PubMed/NCBI
- Google Scholar
41. Nicklas JA, Noreault-Conti T, Buel E. Development of a fast, simple profiling method for sample screening using high resolution melting (HRM) of STRs. J. Forensic Sci. 2012; 57: 478–488. pmid:22150300
- View Article
- PubMed/NCBI
- Google Scholar
42. Nguyen Q, McKinney J, Johnson DJ, Roberts KA, et al. STR Melting Curve Analysis as a Genetic Screening Tool for Crime Scene Samples. J. Forensic Sci. 2012; 57: 887–899. pmid:22486563
- View Article
- PubMed/NCBI
- Google Scholar

[ref1] 1. Lupiáñez JA, Salguero LG, Torres NV, Peragón J, Meléndez-Hevia E. Metabolic support of the flight promptness of birds. Comp. Biochem. Physiol. B Biochem. Mol. Biol. 1996; 11: 439–443.
View Article
Google Scholar

[2] View Article

[3] Google Scholar

[ref2] 2. Mannen H, Tsoi SC, Krushkal JS, Li WH, Li SS. The cDNA cloning and molecular evolution of reptile and pigeon lactate dehydrogenase isozymes. Mol. Biol. Evol. 1997; 14: 1081–1087. pmid:9364765
View Article
PubMed/NCBI
Google Scholar

[5] View Article

[6] PubMed/NCBI

[7] Google Scholar

[ref3] 3. Ramadan S, Miyake T, Yamaura J, Inoue-Murayama M. LDHA gene is associated with pigeon survivability during racing competitions. PLoS ONE. 2018; 13: e0195121. pmid:29775483
View Article
PubMed/NCBI
Google Scholar

[9] View Article

[10] PubMed/NCBI

[11] Google Scholar

[ref4] 4. Jedrzejczak-Silicka M., Yu YH., Cheng YH., Dybus A. The influence of LDHA gene polymorphism on relative level of its expression in racing pigeons. Acta Sci. Pol. Zootechnica. 2018; 17: 9–16.
View Article
Google Scholar

[13] View Article

[14] Google Scholar

[ref5] 5. Van Hall G, Gonzaâlez-Alonso J, Sacchetti M, Saltin B. Skeletal muscle substrate metabolism during exercise: methodological considerations. Proc. Nutr. Soc. 1999; 58: 899–912. pmid:10817157
View Article
PubMed/NCBI
Google Scholar

[16] View Article

[17] PubMed/NCBI

[18] Google Scholar

[ref6] 6. Van Hall G. Lactate as a fuel for mitochondrial respiration. Acta Physiol. Scand. 2000; 168: 643–656. pmid:10759601
View Article
PubMed/NCBI
Google Scholar

[20] View Article

[21] PubMed/NCBI

[22] Google Scholar

[ref7] 7. Ramadan S, Yamaura J, Miyake T, Inoue-Murayama M. DNA polymorphism within LDHA-A gene in pigeon (Columba livia). J. Poult. Sci. 2013; 50: 194–197.
View Article
Google Scholar

[24] View Article

[25] Google Scholar

[ref8] 8. Newman LA, Korol DL, Gold PE. Lactate produced by glycogenolysis in astrocytes regulates memory processing. PloS One. 2011; 6: e28427. pmid:22180782
View Article
PubMed/NCBI
Google Scholar

[27] View Article

[28] PubMed/NCBI

[29] Google Scholar

[ref9] 9. Proia P, Di Liegro CM, Schiera G, Fricano A, Di Liegro I. Lactate as a metabolite and a regulator in the central nervous system. Int. J. Mol. Sci. 2016; 17: 1450. pmid:27598136
View Article
PubMed/NCBI
Google Scholar

[31] View Article

[32] PubMed/NCBI

[33] Google Scholar

[ref10] 10. Dybus A, Kmieć M. PCR-RFLPs within the lactate dehydrogenase (LDH-A) gene of the domestic pigeon (Columba livia var. domestica). J. Appl. Genet. 2002; 43: 501–504. pmid:12441634
View Article
PubMed/NCBI
Google Scholar

[35] View Article

[36] PubMed/NCBI

[37] Google Scholar

[ref11] 11. Dybus A, Pijanka J, Cheng CH, Sheen F, Grzesiak W, Muszyńska M. Polymorphism within the LDHA gene in the homing and non-homing pigeons. J. Appl. Genet. 2006; 47: 63–66. pmid:16424611
View Article
PubMed/NCBI
Google Scholar

[39] View Article

[40] PubMed/NCBI

[41] Google Scholar

[ref12] 12. Dybus A. Nucleotide sequence variation of lactate dehydrogenase A and B genes in pigeons. 2009. Post-doctoral Thesis. The Publishing House of the West Pomeranian University of Technology in Szczecin.
View Article
Google Scholar

[43] View Article

[44] Google Scholar

[ref13] 13. Proskura WS, Cichoń D, Grzesiak W, Zaborski D, Sell-Kubiak E, Cheng Y-H, et al. Single nucleotide polymorphism in the LDHA gene as a potential marker for the racing performance of pigeons. J. Poult. Sci. 2014. 51: 364–368.
View Article
Google Scholar

[46] View Article

[47] Google Scholar

[ref14] 14. Proskura WS, Dybus A, Łukaszewicz A, Hardziejewicz E, Pawlina E. The single nucleotide polymorphisms in lactate dehydrogenase-A (LDHA) and feather keratin (F-KER) genes and racing performance of domestic pigeon. Zesz. Nauk. UP Wroc. Biol. Hod. Zwierz. 2015; 76: 37–42.
View Article
Google Scholar

[49] View Article

[50] Google Scholar

[ref15] 15. Gebhardt C. Molecular markers, maps and population genetics. In: Vreugdenhil D, Bradshaw J, Gebhardt C, Govers F, Taylor M, MacKerron D, Ross H. Potato biology and biotechnology. Advances and perspectives. Elsevier Science; 2007. pp. 77–89.
View Article
Google Scholar

[52] View Article

[53] Google Scholar

[ref16] 16. Dardé ML, Ajzenberg D, Smith J. Population structure and epidemiology of Toxoplasma gondii. In: Weiss LM, Kim K. Toxoplasma Gondii. The model apicomplexan: perspectives and methods. Academic Press; 2007, pp. 49–80. https://doi.org/10.1016/B978-012369542-0/50005-2

[ref17] 17. McMahon K, Paciorkowski AR, Walters-Sen LC, Milunsky JF, Bassuk A, Darbro B, et al. Neurogenetics in the genome era. In: Swaiman K, Ashwal S, Ferriero D, Schor N, Finkel R, Gropman A, Pearl P, Shevell M. Swaiman’s pediatric neurology. Elsevier; 2017, pp. 257–267. https://doi.org/10.1016/B978-0-323-37101-8.00034–5

[ref18] 18. Herrera RJ, Bertrand RG. The nature of evolution. In: Herrera RJ, Bertrand RG. Ancestral DNA, human origins, and migrations. Academic Press; 2018, pp. 1–31. https://doi.org/10.1016/B978-0-12-804124-6.00001-X

[ref19] 19. Turnpenny P, Elladr S. Emery’s elements of medical genetics. 15^th ed. Elsevier; 2017.

[ref20] 20. Brinkmann B, Klintschar M, Neuhuber F, Huhe J, Rolf B. Mutation rate in human microsatellites: Influence of the structure and length of the tandem repeat. Am. J. Hum. Genet. 1998; 62: 1409–15. pmid:9585597
View Article
PubMed/NCBI
Google Scholar

[59] View Article

[60] PubMed/NCBI

[61] Google Scholar

[ref21] 21. Arthofer W, Steiner FM, Schlick-Steiner BC. Rapid and cost-effective screening of newly identified microsatellite loci by high-resolution melting analysis. Mol. Genet. Genomics 2011; 286: 225–235. pmid:21847526
View Article
PubMed/NCBI
Google Scholar

[63] View Article

[64] PubMed/NCBI

[65] Google Scholar

[ref22] 22. Deng JQ, Liu BQ, Wang Y, Liu W, Cai JF, Long R, et al. Y-STR genetic screening by high-resolution melting analysis. Genet. Mol. Res. 2016; 15: gmr.15017266. pmid:26909950
View Article
PubMed/NCBI
Google Scholar

[67] View Article

[68] PubMed/NCBI

[69] Google Scholar

[ref23] 23. Jennings TN, Knaus BJ, Mullins TD, Haig SM, Cronn RC. Multiplexed microsatellite recovery using massively parallel sequencing. Mol. Ecol. Resour. 2011; 1:1060–7. pmid:21676207
View Article
PubMed/NCBI
Google Scholar

[71] View Article

[72] PubMed/NCBI

[73] Google Scholar

[ref24] 24. Hosseinzadeh-Colagar A, Haghighatnia MJ, Amiri Z, Mohadjerani M, Tafrihi M. Microsatellite (SSR) amplification by PCR usually led to polymorphic bands: Evidence which shows replication slippage occurs in extend or nascent DNA strands. Mol. Biol. Res. Commun. 2016; 5: 167–174. pmid:28097170
View Article
PubMed/NCBI
Google Scholar

[75] View Article

[76] PubMed/NCBI

[77] Google Scholar

[ref25] 25. Ellegren H. Microsatellites: Simple sequences with complex evolution. Nat. Rev. Genet. 2004; 5: 435–445. pmid:15153996
View Article
PubMed/NCBI
Google Scholar

[79] View Article

[80] PubMed/NCBI

[81] Google Scholar

[ref26] 26. Ogliari JB, Boscariol RL, Camargo LEA. Optimization of PCR amplification of maize microsatellite loci. Genet. Mol. Biol. 2000; 23: 395–398.
View Article
Google Scholar

[83] View Article

[84] Google Scholar

[ref27] 27. Brookes C, Bright JA, Harbison S, Buckleton J. Characterising stutter in forensic STR multiplexes. Forensic Sci. Int. Genet. 2012; 6: 58–63. pmid:21388903
View Article
PubMed/NCBI
Google Scholar

[86] View Article

[87] PubMed/NCBI

[88] Google Scholar

[ref28] 28. Harr B, Zangerl B, Schlötterer C. Removal of microsatellite interruptions by DNA replication slippage: phylogenetic evidence from Drosophila. Mol. Biol. Evol. 2000; 17: 1001–1009. pmid:10889213
View Article
PubMed/NCBI
Google Scholar

[90] View Article

[91] PubMed/NCBI

[92] Google Scholar

[ref29] 29. Castillo-Lizardo M, Henneke G, Viguera E. Replication slippage of the thermophilic DNA polymerases B and D from the Euryarchaeota Pyrococcus abyssi. Front. Microbiol. 2014; 5: 1–10. pmid:24478763
View Article
PubMed/NCBI
Google Scholar

[94] View Article

[95] PubMed/NCBI

[96] Google Scholar

[ref30] 30. Ananda G, Walsh E, Jacob KD, Krasilnikova M, Eckert KA, Chiaromonte F, et al. Distinct mutational behaviors differentiate short tandem repeats from microsatellites in the human genome. Genome Biol. Evol. 2013; 5: 606–620. pmid:23241442
View Article
PubMed/NCBI
Google Scholar

[98] View Article

[99] PubMed/NCBI

[100] Google Scholar

[ref31] 31. Gemayel R, Vinces MD, Legendre M, Verstrepen KJ. Variable tandem repeats accelerate evolution of coding and regulatory sequences. Annu. Rev. Genet. 2010; 44: 445–477. pmid:20809801
View Article
PubMed/NCBI
Google Scholar

[102] View Article

[103] PubMed/NCBI

[104] Google Scholar

[ref32] 32. Hommelsheim CM, Frantzeskakis L, Huang M, Ülker B. PCR amplification of repetitive DNA: a limitation to genome editing technologies and many other applications. Sci. Rep. 2014; 4: 5052. pmid:24852006
View Article
PubMed/NCBI
Google Scholar

[106] View Article

[107] PubMed/NCBI

[108] Google Scholar

[ref33] 33. Riet J, Ramos LRV, Lewis RV, Marins LF. Improving the PCR protocol to amplify a repetitive DNA sequence. Genet. Mol. Res. 2017; 16: gmr16039796. pmid:28973773
View Article
PubMed/NCBI
Google Scholar

[110] View Article

[111] PubMed/NCBI

[112] Google Scholar

[ref34] 34. Kunkel TA, Bebenek K. DNA replication fidelity. Annu. Rev. Biochem. 2000; 69: 497–529. pmid:10966467
View Article
PubMed/NCBI
Google Scholar

[114] View Article

[115] PubMed/NCBI

[116] Google Scholar

[ref35] 35. Kulibaba RA, Liashenko YV. Influence of the PCR artifacts on the genotyping efficiency by the microsatellite loci using native polyacrylamide gel electrophoresis. Cytol. Genet. 2016; 50: 162–167.
View Article
Google Scholar

[118] View Article

[119] Google Scholar

[ref36] 36. Moorey SE, Walker BN, Elmore MF, Elomer JB, Rodning SP, Biase FH. Rewiring of gene expression in circulating white blood cells is associated with pregnancy outcome in heifers (Bos taurus). Sci. Rep. 2020; 10: 16786. pmid:33033295
View Article
PubMed/NCBI
Google Scholar

[121] View Article

[122] PubMed/NCBI

[123] Google Scholar

[ref37] 37. Green MR, Sambrook J. Isolation of DNA fragments from polyacrylamide gels by the crush and soak method. Cold Spring Harb. Protoc. 2019;754. pmid:30710028
View Article
PubMed/NCBI
Google Scholar

[125] View Article

[126] PubMed/NCBI

[127] Google Scholar

[ref38] 38. Vianna JA, Noll D, Mura-Jornet I, Valenzuela-Guerra P, González-Acuña D, Navarro C, et al. Comparative genome-wide polymorphic microsatellite markers in Antarctic penguins through next generation sequencing. Genet. Mol. Biol. 2017; 40: 676–687. pmid:28898354
View Article
PubMed/NCBI
Google Scholar

[129] View Article

[130] PubMed/NCBI

[131] Google Scholar

[ref39] 39. Litt M, Hauge X, Sharma V. Shadow bands seen when typing polymorphic dinucleotide repeats: some causes and cures. BioTechniques. 1993; 15: 280–284. pmid:8373596
View Article
PubMed/NCBI
Google Scholar

[133] View Article

[134] PubMed/NCBI

[135] Google Scholar

[ref40] 40. Demir G, Alkan C. Characterizing microsatellite polymorphisms using assembly-based and mapping-based tools. Tur. J. Biol. 2019; 43: 264–273. pmid:31496881
View Article
PubMed/NCBI
Google Scholar

[137] View Article

[138] PubMed/NCBI

[139] Google Scholar

[ref41] 41. Nicklas JA, Noreault-Conti T, Buel E. Development of a fast, simple profiling method for sample screening using high resolution melting (HRM) of STRs. J. Forensic Sci. 2012; 57: 478–488. pmid:22150300
View Article
PubMed/NCBI
Google Scholar

[141] View Article

[142] PubMed/NCBI

[143] Google Scholar

[ref42] 42. Nguyen Q, McKinney J, Johnson DJ, Roberts KA, et al. STR Melting Curve Analysis as a Genetic Screening Tool for Crime Scene Samples. J. Forensic Sci. 2012; 57: 887–899. pmid:22486563
View Article
PubMed/NCBI
Google Scholar

[145] View Article

[146] PubMed/NCBI

[147] Google Scholar

Figures

Abstract

Introduction

Methods

Ethical approval

DNA extraction

Genotyping with conventional PCR and gel electrophoresis

Urea-PAGE electrophoresis

qPCR-HRM analysis

Verification by DNA sequencing

Results and discussion

Conclusions

Supporting information

S1 Fig. The original gel image of PCR analyses of five identified genotypes using agarose gel electrophoresis.

S2 Fig. The original urea-polyacrylamide gel electrophoresis of PCR analyses of five identified genotypes using agarose gel electrophoresis.

S3 Fig. The original image of qPCR-HRM analysis.

S4 Fig. The original image of qPCR-HRM analysis.

S5 Fig. The original image of sequencing results for the (TTTAT)3-5 microsatellite polymorphism in the LDHA gene (direct PCR).

S6 Fig. The original image of sequencing results for the (TTTAT)3-5 microsatellite polymorphism in the LDHA gene (amplicons isolated from urea-PAGE gel).

References

S5 Fig. The original image of sequencing results for the (TTTAT)_3-5 microsatellite polymorphism in the LDHA gene (direct PCR).

S6 Fig. The original image of sequencing results for the (TTTAT)_3-5 microsatellite polymorphism in the LDHA gene (amplicons isolated from urea-PAGE gel).