Characterization, development and multiplexing of microsatellite markers in three commercially exploited reef fish and their application for stock identification

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Microsatellites are hypervariable, nuclear-encoded and codominant-inherited markers used for a variety of aquaculture and fisheries applications, including determining the spatial extent of fisheries stocks and other important applications of population genetics. De novo discovery of microsatellites is required for analyses in the laboratory with each non-model species studied; however the costs are high and the procedure involving cloning is time-consuming (Peters et al., 2009). The alternative to de novo development is cross-species amplification where existing microsatellite loci of related species are used on the target species; but this is often hampered by the lack of conserved flanking sequences of microsatellites or the lack of data on related species. The adoption of Next-Generation Sequencing (NGS) by researchers using microsatellite loci has made the discovery of microsatellite markers easier (Gardner et al., 2011) and is becoming the preferred method for developing microsatellites (Abdelkrim et al., 2009; Castoe et al., 2010; Fernandez-Silva et al., 2013). Once the microsatellites are identified, major cost and time reductions in the laboratory are achieved through polymerase chain reaction (PCR) multiplexing. The challenge of PCR multiplexing is to combine several microsatellite primers into one PCR cocktail to amplify several microsatellite loci at the same time.

Herein, we describe the discovery, characterization, development and multiplexing of microsatellite loci of three reef fish species of commercial and recreational significance: golden snapper (Lutjanus johnii, Lutjanidae), blackspotted croaker (Protonibea diacanthus, Sciaenidae) and grass emperor (Lethrinus laticaudis, Lethrinidae). Lutjanus johnii, is a highly prized sport and food fish and is harvested in the commercial, recreational, charter and indigenous sectors of northern Australia and many other fisheries worldwide (Allen, Swainston & Ruse, 1997). The catch of L. johnii has been declining in the Northern Territory since 1997 and this species is considered overfished (Grubert et al., 2013; Saunders et al., 2014a). Sciaenids form the basis of commercial and recreational fisheries of tropical and temperate regions worldwide (Lenanton & Potter, 1987; Rutherford et al., 1989) and several large species are considered threatened or vulnerable due to over-fishing (Rao et al., 1992; Saunders et al., 2014b; True, Loera & Castro, 1997). Among Sciaenid species, P. diacanthus is vulnerable to over-exploitation because of its predictable aggregating behavior (Bowtell, 1995; Bowtell, 1998; Phelan, Gribble & Garrett, 2008). Lethrinus laticaudis is considered an excellent eating fish and is targeted by commercial fishers and recreational anglers across northern Australia (Coleman, 2004). Although L. laticaudis is considered robust to fishing pressure (Grubert, Kuhl & Penn, 2010) due to its high reproductive capacity (i.e., serial batch spawners, high spawning frequency, high batch fecundity) (Ayvazian et al., 2004), it is heavily exploited in some areas. These three fish species are of high economic value and the sustainability of the fisheries they support is potentially threatened by over harvesting and thus requires the development of suitable management programs. The development of genetic tools is necessary to further investigate their population genetics and assess stock structure.

In this study, we provide novel polymorphic microsatellite loci for the three species. We also describe a fast and cost-effective protocol for species-specific microsatellite marker discovery using genomic sequencing and multiplexing. Finally, we explore the relevance of the described microsatellite markers for further population genetics by looking at the genetic differences found between two locations in the Northern Territory for the three study species. This will inform us on the potential to use these markers for the identification of stocks for management purposes. This is the first report of the nuclear genomes of the three study species and provides useful baseline information for future genetic studies of these important species.

Materials and Methods

Sample and extraction

Samples selected for the production of the microsatellite loci were derived from muscle tissue collected by the Northern Territory Department of Primary Industries and Fisheries and the Western Australian Department of Fisheries under Charles Darwin University Animal Ethics permit A13014. The L. johnii sample was a 210 mm male caught at 6 m depth in Darwin Harbour, Northern Territory, Australia (Middle Arm, 130°58′0.24′′E, 12°39′0.97′′S) in 2013. The P. diacanthus sample was a 890 mm male caught in Fenton patches, Northern Territory, Australia (130°42.084′E, 12°10.664′S) in 2013. The L. laticaudis sample (WAM16-001) was a 419 mm male collected from East of the Lacepede Islands, Western Australia, Australia in 2013. Genomic DNA from L. johnii and P. diacanthus was extracted using Qiagen DNeasy Blood & Tissue columns (Qiagen, Germantown, MD, USA) following the manufacturer’s instructions. Lethrinus laticaudis genomic DNA was extracted using a salting-out method as described in Broderick et al. (2011). Genomic DNA from all samples for testing the loci and further genotyping was extracted using ISOLATE II Genomic DNA Kit (Bioline) following the manufacturer’s instructions. This resulted in 100 µL of eluted DNA for each sample. All the DNA extracts were quantified using the Qubit v3 (ThermoFisher) fluorometric method.

Next-generation sequencing and primer selection

The purified genomic DNA of L. johnii and P. diacanthus was prepared for direct shotgun sequencing using the Iron ExpressTM fragment library kit and sequenced on an IonTorrent Personal Genome Machine using an Ion318 chip (Life Technologies Corporation, Grand Island, NY, USA). The purified genomic DNA of L. laticaudis was sequenced on an Illumina® MiSeq as part of a 2 × 300 bp run at the Australian Genome Research Facility. Because two different NGS platforms were used to scan the genomes of the three species we were able to compare their performance for microsatellite design and to assess whether equivalent results were obtainable from each platform. Lutjanus and Lethrinus genera and Sciaenidae are known to have genome size comparable to other fish species (average size for Lutjanus = 1,066 Mb, Lethrinus = 1,192 Mb, Sciaenidae = 753 Mb, Perciformes = 919 Mb; Gregory, 2001). The paired-end reads obtained with the MiSeq run were merged using FLASH source code (Magoč & Salzberg, 2011) and their quality was checked in FastQC (Andrews, 2010); the first 10 bp were trimmed in Geneious v 9.0 (Kearse et al., 2012).

From the NGS data we looked for sequences longer than 300 bp that contained a microsatellite repeat that would be suitable for primer design. These sequences were checked for microsatellite motifs and forward and reverse primers were designed using the software QDD2 beta (Meglécz et al., 2010). Sequences with target microsatellites and primers were then filtered according to the following criteria: only pure repeats were selected; all dinucleotide repeats were excluded; repeats greater than eight were selected; loci with a predictive target sequence length above 300 bp were selected; primers with a distance less than 20bp from the repeat sequence were excluded; and the PCR primers with a PCR_PRIMER_ALIGNSCORE equal or above 6 were excluded to discard primers with high alignment scores to the amplicon. A unique pair of primers was selected for each locus. The PCR predicted sequences for all the loci were imported into Geneious v 9.0 and blasted (MEGABLAST) against the NCBI GenBank database to check if the microsatellites fell into coding regions. Sequences that would be homologous to any other NCBI sequence likely to be functional were excluded. All the primers were blasted against their original genomic database built using the NGS reads. Only microsatellites with primers that had one hit across the whole genome were kept for further steps to increase the chance of each primer to amplify a unique sequence. As a final check point before wet laboratory work and to make sure each pair of primers bound to the 5′ and 3′ ends of a unique sequence containing a microsatellite we selected, containing microsatellites sequences and pairs of primers were mapped de novo. For each species, we selected the 48 microsatellites that contained the best quality repeats with the highest number of tri- tetra- or penta-nucleotide repeats possible and with no small dinucleotide repeats between the primer and the microsatellite sequence to avoid any noise that may interfere with scoring genotypes.

Forward primers were tagged on the 5′ end with the universal CAG sequence (5′-CAGTCGGGCGTCATCA-3′). Inclusion of the 5′-tail will allow use of a CAG-tagged universal primer in the PCR that is fluorescently labeled for detection on the sequencing machine (Schuelke, 2000). Additionally, a pig-tail (5′-GTTTCTT-3′) was added to the 5′ end of the reverse primers to increase the accuracy of genotyping and ensure the consistency of the amplicon size (Brownstein, Carpten & Smith, 1996). The resulting 48 pairs of primers were synthetized by Integrated DNA Technologies (

Loci and primers testing

For each species, the 48 pairs of primers were tested over a set of genomic DNA extracted from eight individuals of the target species. The fluorescent dye labelling of PCR fragments in one reaction was performed with three primers. Amplification reactions were carried out in a 8.8 µL volume comprising 1 µL of DNA, 4.84 µL of 2× Bioline Taq Mastermix, 4.4 pmol of locus-specific forward CAG-tagged primer, 22 pmol of locus-specific reverse pig-tail-tagged primer and 22 pmol of universal CAG primer labeled with a 6-FAM fluorescent dye. The heating cycle parameters used for amplification were 95 °C for 3 min, 37 cycles of denaturation at 94 °C for 15 s, annealing for 15 s at 57 °C and elongation at 72 °C for 60 s. A final extension at 72 °C for 30 s was performed. Post-amplification, the PCR products were diluted with water 1:20. We added 2 µL of these diluted PCR products to 10 µL of Hi-Di formamide (ABI) and 0.05 µL of GenScan-500 LIZ (ABI) size standard. Samples were denatured at 95 °C for 3 min and sized on the ABI 3730xl capillary sequencer (Applied Biosystems, Carlsbad, California, USA) using the conditions set down by the manufacturer. Chromatograms were analysed using Geneious v 9.0 (Kearse et al., 2012).

Criteria used to select the best loci among the 48 tested for each species included the amplification success rate, peak intensity, the presence or absent of stutter peaks, the polymorphism of the loci, the number of alleles and heterozygosity. The best loci were individually tested against a further 23 samples of the target species.

Multiplex optimization of PCR

In order to reduce the cost and time of genotyping for further genetic studies, the newly designed microsatellites were combined into multiplex panels of 2–4 loci. The panels were set up based on the microsatellite allele-size range. The primers for all the loci of each panel were combined in a single PCR to allow the amplification of several microsatellite loci at the same time. When allele-size ranges overlapped, alternate dyes were employed to allow the discrimination of each locus on the chromatograms. Each of the four ABI dyes FAM, VIC, NED and PET were tailed with a unique M13 primer: M13F (5′-TTTCCCAGTCACGACGTTG-3′), M13V (5′-GCGGATAACAATTTCACACAGG-3′), M13N (5′-TAAAACGACGGCCAGTGC-3′) and M13P (5′-CACAGGAAACAGCTATGACC-3′). The 5′ end of the forward primer for the locus was synthetized with the corresponding M13 tail to allow fluorescent labeling of PCR product using a 3-primer PCR protocol as described above (Schuelke, 2000). Several multiplex trials were conducted to find the best combination of loci with the optimal concentration of primers and PCR parameters. Primer pairs that failed to amplify within a multiplex were removed from the panels and further optimization focused on the remaining primer pairs. For each species, the multiplex trials were all evaluated against eight samples that were the same for those used in the 23 samples above, allowing the consistency to be checked across the templates.

Genetic variability and population genetics

In order to test if the herein developed microsatellites would be useful to discriminate fish stocks across northern Australia we collected samples from two locations in the Northern Territory and one location in Western Australia and assayed their population structure. For each of the three species, samples were collected from Camden Sound (Western Australia, Australia), Wadeye (Northern Territory, Australia) close to the Western Australia border and Vanderlin Islands in the bottom of the Gulf of Carpentaria (Northern Territory, Australia) (Fig. 1). Fourteen L. johnii, eighteen P. diacanthus and twenty-eight L. laticaudis were collected from Camden Sound (Western Australia, Australia); twenty-nine L. johnii, twenty-five P. diacanthus and twenty-seven L. laticaudis were collected from Wadeye (Northern Territory, Australia); twenty-five L. johnii, twenty-nine P. diacanthus and twenty-nine L. laticaudis were collected from Vanderlin Islands (Northern Territory, Australia). All individuals were assayed as part of the multiplex panels or PCR pooled. The multiplex PCR were comprised of 2–5 µL of DNA depending on the samples (approximately 20 ng total), 8 µL of 2× Bioline Taq Mastermix and 4 µL of panel primer mix containing various quantities of primers as described in Table 1. Concentrations of the different primers were adjusted to obtain homogenous PCR products revealed by similar intensity chromatogram peaks for each of the dyes within each panel. The heating cycle parameters, sizing of the alleles and chromatogram analyses were conducted using the same method as stated above.

The obtained datasets were statistically evaluated. The potential for null alleles, large allele dropout and stuttering to interfere with scoring accuracy was evaluated for each microsatellite locus in each sample using Microchecker v.2.2.3 (Van Oosterhout et al., 2004). The software Arlequin (Excoffier & Lischer, 2010) was used to calculate the number of alleles (A), expected (He) and observed (Ho) heterozygosity and conduct exact tests of conformance of genotypic proportions to Hardy–Weinberg equilibrium expectations. Estimation of probability values (PHW) employed a Monte Carlo Markov Chain (MCMC) of 105 steps and 5 × 104 dememorization. Genotypic equilibrium between pairs of microsatellites (linkage disequilibrium) was tested in Arlequin with 10,000 permutations. Fixation indices (FST) between pairs of sample localities were estimated as implemented in Arlequin to identify possible spatial boundaries among sample locations.

Location of the three sampling sites across northern Australia.

Figure 1: Location of the three sampling sites across northern Australia.

Table 1:
Technical details on the multiplex polymerase chain reaction (PCR) and post-PCR pooled products of microsatellite loci in Lutjanus johnii, Protonibea diacanthus and Lethrinus laticaudis.
Included in the table are the multiplex PCR panels for L. johnii, P. diacanthus and post-PCR pooled products panels for L. laticaudis, primer mix quantities per reaction (µL) within each multiplex and fluorescent dye labels used for each locus in the PCR reactions.
Species Panel Microsatellite Quantity (µL) ABI dye
Lutjanus johnii 1 Luj094 0.2 FAM
Luj068 0.6 PET
Luj027 0.6 FAM
Luj076 0.6 VIC
2 Luj051 0.2 VIC
Luj090 0.4 FAM
Luj114 0.6 VIC
Luj091 0.6 PET
3 Luj072 0.7 FAM
Luj082 0.7 VIC
Protonibea diacanthus 1 Prd012 0.2 PET
Prd023 0.2 VIC
Prd044 0.2 FAM
Prd042 0.2 NED
2 Prd018 0.4 NED
Prd045 0.2 PET
Prd046 0.2 FAM
Prd020 0.2 PET
3 Prd036 0.2 VIC
Prd049 0.2 FAM
Prd024 0.2 PET
Lethrinus laticaudis 1 Lel033 NED
Lel012 PET
Lel040 VIC
Lel011 FAM
2 Lel032 NED
Lel028 PET
Lel041 VIC
Lel013 FAM
3 Lel036 NED
Lel039 PET
Lel044 VIC
Lel047 FAM
4 Lel027 FAM
DOI: 10.7717/peerj.2418/table-1


Primer mix for each locus is all initially made with 6 µL of forward (M13) primer (10 µM), 30 µL of reverse primer (10 µM), 30 µL of M13 labeled dye (10 µM) and 84 µL of water. The primer mixes of each panel are mixed in the proportion given in the table with water added to reach 4 µL.

Results and Discussion

The IonTorrent sequencing technology allowed the production of longer reads (range 8–620 bp) compared to the Illumina MiSeq that produced 300 bp reads fixed by the method. The paired-end reads of the MiSeq run were merged to increase their length to 300–575 bp and allow the detection of at least 300 bp length sequences that may contain a microsatellite locus. This resulted in 1,169,198 reads, which is less than what was used to select microsatellite loci in the first two species. The MiSeq run produced higher quality sequences than the IonTorrent (Phred score: 36 vs. 29). Quality profiles along the IonTorrent reads showed that the quality of the sequencing decreased with length meaning that the end of the longer reads (>325 bp) had a lower quality then at their start. QDD Pipe1 detected between 110,000 and 170,000 sequences containing a microsatellite sequence depending on the species (Table 2). This number was independent of the type of NGS platform used. From those sequences QDD Pipe2 removed the low complexity sequences (no BLAST to itself), putative minisatellites (short sequences of repeated nucleotides) and sequences that had BLAST hit to other sequences to only keep the singletons and unique consensus sequences. QDD Pipe3 designed primers for all QDD Pipe2 output reads. The resulting number of sequences that contained a microsatellite sequence and the corresponding primers were given in the final output of QDD pipeline, and varied between 20,000 and 30,000 depending on the species (Table 2). After applying the filtering criteria described previously, 97 potentially amplifiable microsatellite reads were found for P. diacanthus, 121 for L. johnii and 103 for L. laticaudis. From those microsatellite reads, we selected the ones with the smallest number of repeats but greater than eight and eliminated those with small repeats between the primer and the microsatellite to reach 48 microsatellite loci per species being ultimately tested in the laboratory.

Table 2:
Next-generation sequencing and bioinformatics details obtained from FastQC software (Andrews, 2010) and QDD pipeline (Meglécz et al., 2010) for Lutjanus johnii, Protonibea diacanthus and Lethrinus laticaudis.
Lutjanus johnii Protonibea diacanthus Lethrinus laticaudis
Genomic DNA extraction Qiagen DNeasy Qiagen DNeasy Salting out
NGS Technology IonTorrent | Ion318Chip IonTorrent | Ion318Chip Illumina® MiSeq
Library preparation Iron ExpressTM Iron ExpressTM
Type of reads Single reads Single reads Paired-end reads
Number of reads 1,374,891 1,587,789 2,800,640
Merged reads 1,169,198
Reads length 8–620 8–618 300
Merged reads length 300–575
% GC 41 42 39
Sequence quality < Phred 20 yes at positions >325 bp yes at positions >350 bp no
Per sequence quality—Phred score 29 29 36
Sequence length distribution peak at 350 bp peak at 350 bp plateau at 520–540 bp
QDD2 pipe 1—Sequence preparation and microsatellite detection
Number sequence length ≥80 bp 1,235,685 1,405,082 1,169,198
Number sequence with microsatellite 109,641 (8.9%) 167,702 (11.9%) 130,269 (11.1%)
QDD2 pipe 2—Sequence similarity detection
Total # input sequences 109,641 167,702 130,269
Numer of unique consensus sequences 18,978 N/A N/A
Number of singleton sequences 49,122 N/A N/A
Number of reads in output 68,100 63,789 69,714
QDD2 pipe 3—Primer design
Total number of input sequences 68,100 63,789 69,714
Total number of sequences with target MS 67,461 63,785 69,714
Total number of sequences with primers 29,485 20,233 19,867
Filtering QDD output
Total # input sequences 29,485 20,233 19,867
Total # sequences after filtering criteria 121 97 103
DOI: 10.7717/peerj.2418/table-2

The testing of 144 primer pairs resulted in the selection of 34 polymorphic loci that could be reliably scored and showed consistent amplification success. We selected a final set of 10 loci for L. johnii, 11 loci for P. diacanthus and 13 loci for L. laticaudis (Table 3). Multiplex panels of microsatellites were developed for the two species L. johnii and P. diacanthus, and the optimization of each panel resulted in the efficient assay and unambiguous scoring of microsatellites in the two species. Although the M13 labeling system worked very well for L. johnii and P. diacanthus it did not amplify successfully as part of PCR multiplexes for L. laticaudis. The reasons why it did not work well for this species are still unclear as the quality of the DNA was even across the three species and the same protocol was followed. However, in-house experiments showed that lengthening the labeled forward primer might facilitate the PCR reaction when multiplexing several loci. Direct labeling of the forward primer may also be another option for multiplexing a large number of loci. For L. laticaudis, the loci were all amplified in individual PCR with the CAG labeling system as described above. The resulting PCR products were then pooled according to the panels described in Table 1 before the ABI run.

Table 3:
Characteristics of the 34 microsatellite markers developed in Lutjanus johnii, Protonibea diacanthus and Lethrinus laticaudis.
Species Locus Primer sequences (5′–3′) (fluorescent label) Repeat motif GenBank accession no. n Allele size range (bp) #A HO HE PHW
Lutjanus johnii Luj027 F: CTGGGCCACACTGATAAAGC (FAM) (AGC)9 KX387441 68 152–179 8 0.309 0.306 0.606
Luj094 F: TCTCAGAGGGTTTGATGCAG (FAM) (AATC)9 KX387437 68 223–239 4 0.426 0.470 0.205
Luj076 F: CGGGTCGAGTCTGTTTGTGT (VIC) (AAG)15 KX387436 66 200–233 10 0.818 0.811 0.289
Luj068 F: CCTAGGGTGTCAGTGTCAGTCA (PET) (AAAG)20 KX387435 68 174–258 18 0.882 0.936 0.212
Luj090 F: ATCCTAATGCATCGTGCTTG (FAM) (AGC)17 KX387444 68 194–278 23 0.868 0.922 0.146
Luj051 F: TGCAGAGCAACAGAACAACAC (VIC) (ACTG)10 KX387440 67 172–192 6 0.687 0.596 0.377
Luj114 F: CCATAACTGCTGTTCTGTATCTGG (VIC) (AGC)9 KX387442 68 276–314 11 0.794 0.739 0.725
Luj091 F: TCATTCCCAGGAGCTCAAAT (PET) (ACAG)12 KX387438 64 219–279 12 0.813 0.782 0.499
Luj072 F: ACTCGAAGAACACAGCCCAC (FAM) (AGC)9 KX387443 65 192–204 5 0.738 0.675 0.052
Luj082 F: AAGTACATCGGAGGGCTGAG (VIC) (ACGAT)12 KX387439 65 220–275 12 0.800 0.833 0.548
Protonibea diacanthus Prd044 F: ACAAAGTTTCCTCCTCTGGC (FAM) (AAG)13 KX387452 71 181–211 11 0.746 0.804 0.324
Prd023 F: TCGTGTGAACACTTTGATGC (VIC) (ATC)11 KX387448 72 292–316 9 0.875 0.847 0.034
Prd042 F: TACCTTTGAGATGCGAGCG (NED) (AGC)12 KX387451 72 230–248 7 0.694 0.698 0.526
Prd012 F: AGGCTGTTTGAACTGCAGGG (PET) (AAAG)20 KX387445 64 195–271 19 0.828 0.898 0.324
Prd046 F: TCATCCTGAGTTTGTGCTGG (FAM) (AGC)9 KX387454 72 224–236 5 0.347 0.351 0.693
Prd018 F: ATGAACGGCATCAGTCAGC (NED) (ACAG)9 KX387446 68 179–207 8 0.662 0.784 0.008
Prd020 F: CAATGTTCTGCAAGAGCTGC (PET) (ATC)11 KX387447 71 189–216 10 0.746 0.713 0.837
Prd045 F: GTCTATCCATGTTCCAGCCC (PET) (ATCC)11 KX387453 64 279–309 8 0.672 0.639 0.400
Prd049 F: CCTTGTCCTCCTTTCAGGC (FAM) (ACC)9 KX387455 72 216–234 5 0.278 0.316 0.280
Prd036 F: TCACGTGAAGCGTCTACAGC (VIC) (AAG)12 KX387450 72 227–257 9 0.653 0.677 0.746
Prd024 F: AGAGTGTCCGAGTCCAGAGG (PET) (AAG)11 KX387449 72 199–217 6 0.736 0.683 0.892
Lethrinus laticaudis Lel011 F: CTGTCGGAGGTAAAGTGCG (FAM) (AGC)9 KX387422 84 237-285 11 0.655 0.660 0.251
Lel040 F: TGGTTGCAGACAACTGCC (VIC) (AGC)9 KX387431 84 171–216 14 0.821 0.825 0.367
Lel033 F: AGTGCGACAAAGAAATGGC (NED) (AGAT)16 KX387428 84 167–143 20 0.893 0.926 0.438
Lel012 F: GCGAGGGTCTGCTACTATAGGG (PET) (AAT)9 KX387423 76 246-334 22 0.711 0.846 0.005
Lel013 F: CCTGAACCTGGAGAACTCGG (FAM) (ATC)12 KX387424 82 242–287 10 0.744 0.829 0.150
Lel032 F: AAATCTGCATTATGAAATTGGC (NED) (AAAG)16 KX387427 83 173–233 16 0.867 0.883 0.209
Lel028 F: CAGTAGCTTTAATAGTTAGGCACCC (PET) (AAAG)13 KX387426 83 200–244 14 0.843 0.877 0.954
Lel027 F: CACTAAGGGTCCATGTTGCC (FAM) (AAT)22 KX387425 79 196–238 15 0.911 0.914 0.480
Lel044 F: TTCTACTTGACCCTGGTAGGC (VIC) (ATCC)11 KX387433 83 151–199 11 0.759 0.816 0.268
Lel039 F: CTTGTAGAGTGTCAACGAGGG (PET) (AAT)11 KX387430 80 196–214 9 0.700 0.764 0.747
DOI: 10.7717/peerj.2418/table-3


n is the sample size, #A is the number of alleles at each loci, HE is the expected heterozygosity, HO is the observed heterozygosity and PHW is the p-value of the exact tests of conformance of genotypic proportions to Hardy-Weinberg equilibrium expectations.

Genotypes from 10 microsatellites were obtained from multiplexed PCR for 68 individuals of L. johnii. There was 1.91 % missing data and the number of alleles for each locus varied between 4 and 23 (Table 3). Microchecker indicated the possible occurrence of null alleles at location Wa for locus Luj012 and at CS for locus Luj018 with possible stuttering or scoring errors for the latter. There were only 3/45 significant tests for linkage disequilibrium between pairs of loci (Luj094 × Luj051, Luj051 × Luj091 and Luj076 × Luj082) and there was no deviation from Hardy–Weinberg equilibrium (HWE) detected. Heterozygosity was moderate to high for all loci (mean overall loci 0.707 ± 0.200) and generally similar to expectations (around 0.7 for marine fish, DeWoody & Avise, 2000). Genotypes from 11 microsatellites were obtained from multiplexed PCR for 72 individuals of P. diacanthus. There was 2.77 % missing data and the number of alleles for each locus varied between five and 19 (Table 3). Microchecker indicated the possible occurrence of null alleles at location CS for locus Prd068 and at VI for locus Prd012. There were only 3/55 significant tests for linkage disequilibrium between pairs of loci (Prd046 × Prd018, Prd020 × Prd018 and Prd018 × Prd045) and overall deviations from Hardy–Weinberg equilibrium (HWE) were detected at two loci Prd023 (p-value = 0.034) and Prd018 (p-value = 0.008). Heterozygosity was variable and with an overall mean lower than for L. johnii (0.673 ± 0.185). Genotypes from 10 microsatellites were obtained from pooled post PCR products for 84 individuals of L. laticaudis as three of our developed microsatellites did not amplified consistently in all the samples. There was 2.61% missing data and the number of alleles for each locus varied between 9 and 22 (Table 3). Microchecker indicated the possible occurrence of null alleles at location CS for loci Lel033 and Lel012. There were 6/78 significant tests for linkage disequilibrium between pairs of loci (Lel040 × Lel012, Lel040 × Lel032, Lel011 × Lel027, Lel012 × Lel032, Lel012 × Lel013 and Lel028 × Lel027) and overall deviations from Hardy–Weinberg equilibrium (HWE) were detected at a single locus Lel012 (p-value = 0.005). Heterozygosity was high and with an overall mean higher than for the two other species (0.834 ± 0.078).

A pattern of genetic differentiation with low but significant population-pairwise FST (range 0.007–0.017) was observed in the three species (Table 4). These levels of differentiation are similar in magnitude to those reported for other marine fish species with potentially high gene flow (O’Reilly et al., 2004). The three species also presented different patterns of structure between the three locations. L. laticaudis presented pairwise differentiation between Western Australia location (CS) and the two other Northern Territory locations (VI and Wa). Similarly, P. diacanthus presented a structure between the two most distant populations of CS and VI whereas CS and Wa remained undifferentiated. By contrast, L. johnii did not present structure between Western Australia and Northern Territory. However, VI and Wa in the Northern Territory had a significant pairwise FST. Pairwise FST values were low in all comparisons for the three species (range 0.001–0.017) as commonly reported in marine species and, 4 out of 9 pairwise comparisons were significant meaning the microsatellites we developed can accurately detect population differentiation across Northern Australia and may be used for genetic structure studies and stock identification.

Table 4:
Pairwise FST estimates for Lutjanus johnii, Protonibea diacanthus, and Lethrinus laticaudis for three locations.
Estimates are based on 10 microsatellite data from 68 individuals of L. johnii, 11 microsatellite data from 72 individuals of P. diacanthus and 10 microsatellite data from 84 individuals of L. laticaudis among the three sampling locations Camden Sound (CS), Wadeye (Wa) and Vanderlin Islands (VI). The comparisons that differed significantly from zero (p < 0.05) are shaded in grey.
Lutjanus johnii Protonibea diacanthus Lethrinus laticaudis
FST p-value FST p-value FST p-value
Wa-CS 0.001 0.308 0.009 0.090 0.017 0.000
Wa-VI 0.007 0.043 0.007 0.069 0.007 0.069
CS-VI 0.006 0.148 0.014 0.013 0.009 0.017
DOI: 10.7717/peerj.2418/table-4


In conclusion, we applied the direct sequencing of a genomic library approach to develop microsatellite loci and it resulted in a significant reduction in laboratory effort compared to traditional protocols for microsatellite discovery (cloning and Sanger sequencing). Merged paired-end reads from the MiSeq platform demonstrated higher quality of reads than the IonTorrent single reads. From the 1–1.5 million raw reads, we selected a reduced number of loci to test (48) and successfully amplified satisfactory polymorphic loci for 10 to 13 of them depending on the species. However, the NGS data revealed the potential for hundreds to thousands of potentially amplifiable microsatellites to be discovered. The microsatellites characterized in this work will be available to explore the population genetics and stock structure of these highly valuable species.

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