Abstract
Iris ruthenica Ker Gawl. and I. uniflora Pall. ex Link, which are rare and endangered species in Korea, possess considerable horticultural and medicinal value among Korean irises. However, discrimination of the species is hindered by extensive morphological similarity. Thus, the aim of the present study was to identify discriminating features by comparing the species’ complete plastid genome (i.e., plastome) sequences and micromorphological features, including leaf margins, stomatal complex distribution (hypostomatic vs. amphistomatic leaves), anther stomata density, and tepal epidermal cell patterns. Plastome comparison revealed slightly divergent regions within intergenic spacer regions, and the most variable sequences, which were distributed in non-coding regions, could be used as molecular markers for the discrimination of I. ruthenica and I. uniflora. Phylogenetic analysis of the Iris species revealed that I. ruthenica and I. uniflora formed a well-supported clade. The comparison of plastomes and micromorphological features performed in this study provides useful information for elucidating taxonomic, phylogenetic, and evolutionary relationships in Iridaceae. Further studies, including those based on molecular cytogenetic approaches using species specific markers, will offer insights into species delimitation of the two closely related Iris species.
Similar content being viewed by others
Introduction
Leaf, flower, and pollen micromorphology has been informative for resolving taxonomic problems in angiosperms across various taxonomic levels1,2,3,4,5,6,7. In particular, leaf epidermal stomata, orbicules, and pollen exine ornamentation characters have been shown to possess systematic values when examined using both light microscopy (LM) and scanning electron microscopy (SEM) and may further be utilized to test phylogenetic hypotheses8,9,10,11,12,13. However, despite an increasing number of the leaf, flower, pollen, and seed micromorphological studies in Iridaceae14,15,16,17,18,19,20,21, leaf margins, stomatal occurrence, and orbicular traits have not been considerably challenged for the taxonomic delineation of two closely related species, Iris ruthenica and I. uniflora. Therefore, understanding their micromorphology may shed light on their taxonomic relationships.
The chloroplast is an essential organelle for photosynthesis, starch and fatty acid biosynthesis, and carbon fixation22,23,24. The length of photosynthetic vascular plant plastomes ranges from 120 to 200 kb and possess a quadripartite structure, with one large single copy (LSC) region, one small single copy (SSC) region, and two inverted repeat (IR) regions. In general, angiosperm plastomes contain 110–130 genes, including approximately 80 protein-coding genes, 30 transfer RNA (tRNA) genes, and four ribosomal RNA (rRNA) genes22. These plastomes possess highly conserved structures and gene content and exhibit low variation when compared to nuclear and mitochondrial genomes. However, variable plastome size, gene content, IR expansion or contraction, and structural arrangement have been reported25,26. Plastome sequencing can be useful for species classification and identification and high-resolution phylogenetic analysis27,28. Facilitated by next-generation sequencing (NGS), plastome data are increasingly utilized for the investigation of phylogenetic relationships and for the development of DNA barcode markers for low-taxonomic-level identification and the discrimination of controversial taxa29,30,31. However, even though complete plastome data are available for a variety of Korean irises32,33, neither the detailed comparative analysis of Iris plastomes nor the combination of such analysis with micromorphological analysis has been conducted in the genus Iris as it has been in other taxonomic groups34,35,36.
The genus Iris L. contains approximately 300 perennial species, which are distributed in temperate regions across the Northern Hemisphere, as well as a large number of infraspecific taxa15,37,38,39. Based on recent molecular phylogenetic analyses, the genus has been divided into six subgenera40,41,42,43,44,45, including Iris L. subg. Limniris (Tausch) Spach ser. Ruthenicae Diels, which contains two species, I. ruthenica Ker Gawl. and I. uniflora Pall. ex Link37,45,46. Interestingly, both I. ruthenica and I. uniflora are rare or endangered in Korea (Fig. 1), owing to their similar pharmacological effect as the herbal medicines or because of their popularity as ornamentals47,48. However, even though the infrageneric classification of Iris based on chloroplast DNA sequence data remains somewhat controversial33,38,45, the monophyly of ser. Ruthenicae is strongly supported by molecular evidence (whole plastome sequences33), chromosome number46, and external morphology37, and the series can be easily distinguished from other series in the genus37. Iris ruthenica is arguably most closely related to I. uniflora due to their similar morphology37,47. Regarding the cytological features, the two species have consistent chromosome numbers (2n = 42), and similar genome sizes (2.42 pg/1C in I. ruthenica; 2.46 pg/1C in I. uniflora)46. However, despite of the economic significance of the two species, genomic resources for the ser. Ruthenicae are still limited. Interestingly, some taxonomists considered I. uniflora as a synonym of I. ruthenica due to their high morphological similarity37,49, and such an example can be found in other taxonomic groups in the genus Iris50. Thus, comparison of the genomic data and micromorphology of the two taxa is needed as indicated in recent studies41,44,46,51,52.
Accordingly, the aims of the present study were to (1) compare the macro/microscopic features of I. ruthenica and I. uniflora, (2) characterize and compare the complete de novo-assembled plastomes for both species, and (3) investigate the evolutionary relationships within Iris through phylogenetic analysis33.
Results
Leaf, flower, pollen, and orbicule morphological characters
The two species possessed similar floral traits (e.g., tepal color, shape, and size; Fig. 1 and Supplementary Fig. S1) and similar leaf epidermis, epidermal cell, and anticlinal wall shapes (Fig. 2). The leaf epidermis of both species consisted of long tabular cells, typically with elongated pavement cells (Fig. 2c,i), with undulate anticlinal walls (Fig. 2e,k) that were covered by either prominent (I. ruthenica; Fig. 2f) or weak (I. uniflora; Fig. 2l) epicuticular wax. However, the leaf margin of I. uniflora was clearly entire, whereas that of I. ruthenica was spiny with sharp stiff points (Fig. 2), and the leaves of I. ruthenica were hypostomatic (stomata are absent or extremely rare on the adaxial leaf surface while they are present on the abaxial leaf surface; Fig. 2c,d), whereas those of I. uniflora were amphistomatic (stomata are present on both adaxial and abaxial leaf epidermis; Fig. 2i–j). In addition, the width of guard cells ranged from 24.63–28.19 μm on the abaxial surfaces of I. ruthenica leaves and from 26.53–28.14 μm and 27.02–27.77 μm on the adaxial and abaxial surfaces of I. uniflora leaves, respectively (Tables 1, 2). SEM analysis revealed that stomata of both species were clearly sunken (Fig. 2f,l), and that they were all anomocytic lacking subsidiary cells, surrounded by four epidermal cells (Fig. 2d,i,j). Tepal epidermal cells had unicellular covered by a striated cuticle and slightly sunk stomata (Supplementary Fig. S1). Furthermore, the outer anther epidermal cells were polygonal in shape and covered by a striated cuticle in both species, I. ruthenica and I. uniflora (Fig. 3g,h,q,r). Both species possessed anthers with anomocytic stomata in the middle section, despite differences in stomatal density (Fig. 3h,r). The guard cell surfaces of I. uniflora were weakly wrinkled (Fig. 3i), whereas those of I. uniflora were smooth (Fig. 3s).
The pollen grains of both species were monads of 47.54–56.31 μm in polar length and 39.18–53.55 μm in equatorial diameter (Table 2). While both species yielded fertile pollen grains (Fig. 3a,k), sterile pollen grains were only found extremely rarely or absent in I. ruthenica (Fig. 3a–c), and, in Iris uniflora, sterile pollen grains were frequently encountered (Fig. 3j–l), which differed from the fertile pollen grains of both species in regard to equatorial width (Table 2), shape (subprolate to prolate, P/E = 1.19–1.49 vs. oblate-spheroidal to prolate-spheroidal, P/E = 0.94–1.12; Table 2), and exine ornamentation (irregularly microreticulate exine ornamentation vs. monosulcate with microreticulate ornamentation; Fig. 3c–d,l–n). The orbicules of both species were entirely fused with the inner locule anther wall, particularly at the tapetal membrane (Fig. 3f, p), and possessed almost identical morphology (i.e., density, size, shape, and surface details).
Plastome sequencing
Illumina MiSeq yielded 5.2 and 6.0 Gb raw paired-end (2 × 300 bp) reads for I. ruthenica and I. uniflora, respectively, and 2.8 and 4.5 Gb trimmed reads, thereby providing coverage of approximately 739.3 × and 1064.6 × , respectively (Supplementary Tables S6 and S7).
Plastome characteristics
Both plastomes exhibited the quadripartite structure typical of angiosperm taxa (Fig. 4), with total lengths of 152,275 and 152,282 bp, LSC region lengths of 82,301 and 82,307 bp, and SSC region lengths of 18,134 and 18,135 bp in I. ruthenica and I. uniflora, respectively, as well as an IR region of 25,920 bp in length in both species (Table 3, Supplementary Figs. S2–4). The plastome junction regions were validated through the generation of high-quality plastome sequences. The overall GC content of the two plastomes was 38.1%, with greater GC content in the IR regions of I. ruthenica and I. uniflora (43.3 and 43.2%, respectively) than in the LSC regions (36.3 and 36.3%) and SSC regions (32.2 and 32.1%). Both plastomes contained 115 genes (80 protein-coding, 4 rRNA, and 31 tRNA genes; Table 3), 18 intron-containing genes (16 with one intron and two with three introns), and duplicate genes (ndhB, trnI-GAU, and trnA-UGC) in the IR regions (Supplementary Table S9). Analysis of codon usage and anticodon recognition patterns indicated that the plastomes of I. ruthenica and I. uniflora contained 26,634 and 26,641 codons, respectively, and that leucine, isoleucine, and serine were the most abundant (Supplementary Fig. S2). Relative synonymous codon usage (RSCU) analysis indicated synonymous codon bias, with a high proportion of A or T in the third position. Most RSCU values indicated a similar pattern. RSCU values for arginine were usually high.
Plastome comparison
Plastome alignment revealed slight genomic variation, with intergenic regions being the most divergent. However, the plastomes generally formed a well-conserved collinear block (Supplementary Fig. S3), with a highly conserved structure. Nucleotide diversity analysis identified 14 regions with weak variation (Figs. 5, 6). The genes psbA and ycf1 yielded Pi values of 0.00188 and 0.00112, respectively. Most of the divergent regions were located in the LSC region (Pi = 0.00243). In particular, the trnK-matK, matK-trnK, and trnK-rps16 regions have shown consecutive nucleotide variations in the LSC region. The analysis of IR boundaries revealed that rpl22 was located in the LSC region of both species. The ycf1 and ndhA genes were located in the junction of SSC/IRb region. The rps19 gene, which was duplicated in the IR regions, was generally well-conserved. The ycf1 gene was located at the IRa/SSC and SSC/IRb junctions (Supplementary Fig. S4).
Phylogenic relationships among Iris species
The ML and BI topologies were highly congruent for the whole plastome and CDS datasets, and all but one lineage was strongly supported (ML > 95%, BI = 1.0). More specifically, the topologies were clearly divided into three major clades, which corresponded to the subgenera Limniris, Pardanthopsis, and Iris (Fig. 7). Most of the Iris species included in the present study were assigned to section Limniris, which is consistent with the Angiosperm Phylogeny Group (APG) IV classification system, except for I. tectorum53. Furthermore, a clade containing I. domestica and I. gatesii was clustered as a sister group to I. tectorum; I. ruthenica and I. uniflora formed a monophyletic clade (Fig. 7).
Discussion
Micromorphology
Iris ruthenica and I. uniflora are sister taxa within ser. Ruthenicae and, as such, share a variety of morphological characters, including creeping rhizomes, leaf shape and size, flower color, and fruit shape37. Indeed, due to their morphological similarity, the taxonomic status of the species has been controversial. For example, Zhao et al.37 suggested that I. uniflora be considered a subgroup of I. ruthenica, and Zheng et al.54 argued that morphological differences between the species are the result of environmental conditions (i.e., different habitats). However, in the present study, I. ruthenica and I. uniflora could be differentiated using a variety of micromorphological features, including stomatal complex distribution (hypostomatic leaves vs. amphistomatic leaves), slight differences in the protruded conical cells of leaf surfaces, pollen grain fertility (all fertile vs. both fertile and sterile), and anther stomata density.
The micromorphological analysis performed in the present study revealed that I. ruthenica and I. uniflora possess leaves with an irregular shape and sinuate anticlinal striation, as previously reported14,20,55. Because both leaf surface micromorphology and stomata have shown considerable variation in papillae, they are not taxonomically significant, as suggested by Wu and Cutler14 and other monocot species56,57. The papillae that cover stomata likely contribute to defense against unfavorable environmental conditions58 or attack by pathogens59. Papillae can also play an important role in light reflection, by preventing overheating60, and, as such, may be more correlated with environmental conditions than taxonomic status. Regardless of stomatal distribution, both species possessed anomocytic stomata (Table 2), which is likely the ancestral (plesiomorphic) condition among monocots61. The guard cell and genome sizes of the two Iris species included in the present study were not significantly distinct (Table 2; Choi et al.46), although it is well known that stomata size is positively correlated with genome size and that ploidy level changes in plants62,63,64.
With the exception of clear differences in pollen viability, the morphology (e.g., shape, size, exine pattern, and orbicule presence) of pollen in I. ruthenica and I. uniflora were not significantly different (Fig. 3). As I. uniflora was only found under low-temperature stress conditions, whereas I. ruthenica was widely distributed46,47,48, the occurrence of sterile pollen grains in I. uniflora might be affected by meiotic abnormalities with genetic constitution as reported in other cold regions65,66. Orbicules, also known as Ubisch bodies, are small sporopollenin particles that can be produced on the inner locule walls of anthers67 and that are, here, reported in I. ruthenica and I. uniflora for the first time. Even though orbicule morphology has been widely used to elucidate systematic and evolutionary relationships12,68,69, the occurrence of orbicules has, until now, only been reported in I. pallida Lam.70. Thus, further investigation of orbicule occurrence in the Iridaceae might yield a significant phylogenetic trait, as reported in other plant groups67,68,69,70,71,72. However, as with other morphological features of Iris taxa, such as tepal structure17, pollen morphology15,16,21,73,74,75, and seed microstructure18, the micromorphological features of either vegetative or reproductive organs are largely insufficient for reconstructing the taxonomic relationship of I. ruthenica and I. uniflora.
Plastome characterization and variation
The structures of the I. ruthenica and I. uniflora plastomes were similar to those of plastomes from other members of the Iridaceae32,33, with the typical quadripartite structure and LSC and SSC regions separated by IR regions. The plastomes of the Iris species contained 114 unique genes, and their gene order, GC content, genomic structure, and overall length (152,275 and 152,282 bp) were within the ranges previously described for Iris plastomes76.
The mVISTA results indicated that the Iris plastomes contained little variation and that genic regions were more conserved than IGS regions, which is consistent with angiosperm plastomes in general77,78,79. More specifically, the psbA, trnK-matK, matK-trnK, and trnK-rps16 regions were hotspots for genetic variation (Fig. 5), which indicated underlying evolution80,81,82,83 and value as molecular markers84,85. In terms of nucleotide diversity (Pi), most of the divergent regions were non-coding, which is consistent with previous reports86,87,88. Other plastomes were highly variable for the non-coding regions at psbA, trnK-matK, matK–trnK, and trnK-rps16 in the present study (Fig. 6). mVISTA and Pi analysis showed difference between I. ruthenica and I. uniflora at the plastome level. Furthermore, these regions will play an important role in the discrimination of I. ruthenica and I. uniflora, as well as other species within the Iridaceae.
IR contraction and expansion causes variation in the size of angiosperm plastomes89. Previous studies have reported extremely short IRs or the loss of IR regions and genes90,91. Compared to I. ruthenica, I. uniflora had a highly conserved IR length and gene positions. However, the rps19 genes of I. ruthenica and I. uniflora were located in the IRa region, and ycf1 was located in the IRa/SSC, region which overlapped with ndhF. Thus, the Iris plastome possessed an extended IR, as reported previously32,33.
Phylogenetic relationships in the Iridaceae
Plastid genome (i.e., plastome) sequences are valuable genomic resources for estimating phylogenetic relationships, particularly among closely related species and unresolved taxa4,27,31. The systematics of Korean irises have been widely discussed, and several molecular studies based on single molecular markers (e.g., psbA-trnH, trnL-F) and plastome structure have been performed in the past33,92. The topologies of phylogenetic trees based on whole plastome sequences in the present study are similar to those reported previously (Fig. 7, Supplementary Figs. S5–S7)33,41,45,52,92. In agreement with earlier results, I. ruthenica and I. uniflora were nested deeply within section Limniris ser. Ruthenicae. However, in the present study, the monophyly of section Limniris was compromised by the inclusion of I. tectorum (ser. Lophris), which was deeply nested with subgenera Pardanthopsis and Iris in both the ML and BI trees (Fig. 7). Due to insufficient taxonomic sampling, the results of the present study are not suitable for the discussion of inter-subgeneric relationships within Iris s.l. 44. Nevertheless, the present study provides important genetic resources for further studies within the genus, as well as micromorphological comparisons between two closely related species in a taxonomic context.
The results of the present study confirm that Iris section Limniris ser. Ruthenicae (formerly section Ioniris sensu Zhao et al.37) contains the two species, I. ruthenica and I. uniflora. Morphologically, I. uniflora is distinguished from I. ruthenica because of the presence of narrow leaves54, but the flowers of the species are difficult to distinguish. In Korea, I. ruthenica is widespread, while I. uniflora is restricted to alpine areas46,47,48. Based on the comparison of morphological and chloroplast genome data of the two species, it is doubtful whether I. ruthenica and I. uniflora can be recognized as independent species-level taxa, as suggested by Zheng et al.54. Thus, further studies on molecular and morphological analyses of the two species at population level are required to clarify the taxonomic status of the two taxa.
Conclusions
The present study provides detailed insights into the leaf and flower micromorphologies and plastome structures of the two closely related species I. ruthenica and I. uniflora. Micromorphological features, including leaf margins, stomatal complex distribution (hypostomatic vs. amphistomatic leaves), anther stomata density, and floral epidermis cell patterns, are somehow useful for distinguishing the taxa, despite that the drastic influences of environmental variation, especially climate factors (e.g., temperature and light intensity), may also contribute to the morphological variations. The plastome sequences of the two related species possessed similar genome lengths, gene numbers, and gene orientations. Most of the variable sequences, which were found in non-coding regions, could be used as molecular markers for the differentiation of I. ruthenica and I. uniflora, as well as other Iris taxa. Given the economic and ecological importance of Korean Iris species, the molecular phylogenetic studies can now prompt a search for diagnostic characters, such as general morphological and micromorphological traits, a necessary prerequisite for any systematic and taxonomic context. Further integrative analyses of plastome sequences and morphological data of the two species at population level as well as employing molecular cytogenetic approaches using species-specific satellite DNA as probes may also offer insights into the species delimitation of the two closely related Iris species.
Materials and methods
Taxon sampling
All plant materials were collected from natural populations in Korea (Table 1). Assoc.-Prof. Dr. Tae-Soo Jang and Dr. Soonku So formally identified all the samples. Considering the protection of Korean endangered plant resources, we only collected a small number of plant specimens with the approval and permission of the local authorities (collection permit nos. 2019–13 [JC532], 2019–14 [BKC939], 2019–20 [JCKC190507]; Table 1). To evaluate the consistency of morphological and micromorphological characters, living specimens were collected from multiple populations (three I. ruthenica specimens from three populations and three I. uniflora specimens from one population), and cultivated at Chungnam National University (Table 1). Meanwhile, for plastome sequencing, representative fresh leaves were collected from I. ruthenica and I. uniflora specimens (accession numbers: BKC939 and JCK2019-77, respectively; Table 1). Specific locality information including GPS coordinates, latitude, and longitude cannot be provided due to the endangered/rare status of the species in Korea. All voucher specimens were deposited in the Chungnam National University Herbarium (CNUK).
Micromorphological analysis
Fresh leaf and flower materials from all four Iris populations were preserved using a formalin-acetic acid-alcohol solution and dehydrated by soaking in an acetone series (50, 70, and 90%) for 30 min and absolute acetone for 1 h. The dehydrated materials were then immersed in carbon dioxide for critical point drying (EMCPD300, Leica Microsystems, Germany), coated using an ion-sputtering device (E-1010, Hitachi, Japan), and analyzed using scanning electron microscopy (SEM; S3000N, Hitachi, Japan), with an accelerating voltage of 20 kV and working distance of 9–15 mm, following Choi et al.5, as well as light microscopy (BX53F, Olympus, Japan), which was used to analyze the structure of leaf epidermal pavement cells and stomatal complexes, following Kim et al.7. At least 20 guard cells were examined on both adaxial and abaxial leaf surfaces from each sample as described by Choi et al.5. To measure the pollen viability of each species, 10 randomly selected anthers from each individual plant were placed in an aniline blue dye solution to distinguish fertile pollen grains as described by Jang et al.93. At least 20 sterile and fertile pollen grains from each sample were randomly selected for size measurements. Both leaf and pollen micromorphological characters were measured using MicroMeasure ver. 3.3 program following Jang et al.94. For SEM, imaging was performed for both the abaxial and adaxial leaf surfaces, as well as for both the inner and outer surfaces of the outer tepals, stamens, and pollen grains. Orbicules, which are cellular structures of sporopollenin particles produced by the secretory tapetum, were investigated in this study for the first time using SEM in the genus Iris.
Plastome sequencing and assembly
Total genomic DNA was extracted from freshly collected samples using the modified CTAB method95, and Illumina short-insert paired-end sequencing libraries (TruSeq DNA Nano kit, Illumina, San Diego, CA, USA) were constructed and sequenced using the Illumina MiSeq platform. For de novo plastome assembly, sequencing reads were trimmed and filtered using FastQC v0.11.796, and the resulting trimmed paired-end reads (Phred score ≥ 20) were assembled using Velvet 1.2.1097, with kmer values of 71, 91 101, and 111 to form large contigs. The Velvet contigs were then assembled into complete plastomes using the de novo assembly option in Geneious prime (https://www.geneious.com) and ordered using reference plastome sequences from I. gatesii (NC_024936), I. sanguinea (NC_029227), and I. missouriensis (NC_042827). Finally, the LSC/IR, IR/SSC, SSC/IR, and IR/LSC regions of the complete plastomes were validated using PCR-based sequencing. Primer information and sequence alignment results are listed in Supplementary Tables S1 and S2.
Plastome annotation and repeat sequence analysis
The I. ruthenica and I. uniflora plastomes were annotated using GeSeq98. Protein-coding sequences were manually curated and confirmed using Artemis99 and then checked against the NCBI protein database. tRNA genes were confirmed using tRNAscan-SE 1.21100, and IR region sequences were confirmed using IR finder and RepEx101. Finally, circular maps of the I. ruthenica and I. uniflora plastomes were generated using OGDRAW102.
For plastome comparison, GC content and relative synonymous codon usage (RSCU) were calculated using MEGA6103. The two plastomes were also compared using mVISTA in Shuffle-LAGAN mode, with I. ruthenica plastome as a reference, and nucleotide variation (Pi) among the plastomes, excluding regions of < 200 bp, was calculated using DnaSP version 6.1104. Each plastome was divided into genes, introns, and intergenic regions.
Plastome phylogenetic analysis
The plastome sequences of eight taxa, including six other taxa from the Iridaceae and the outgroup taxa Crocus cartwrightianus (NC_041459) and C. sativus (NC_041459), were obtained from NCBI GenBank (Supplementary Table S3), and two matrices, one of whole plastome sequences and another of 78 conserved protein-coding sequences (CDS), which excluded duplicate genes in the IR region, were generated using MAFFT ver. 7105; all ten plastome sequences were then manually adjusted using Bioedit106. For CDS analysis, the aligned CDS were extracted and concatenated using Geneious (https://www.geneious.com) and filtered to remove ambiguously aligned regions using GBLOCKS ver. 0.91b107. The best-fitting model for nucleotide substitution was determined using the Akaike Information Criterion (AIC) in JModeltest V2.1.10108 (Supplementary Table S4). Maximum likelihood (ML) analysis was performed using RaxML v8.0.5109, with 1000 bootstrap replicates and the GTR + I + G model, and Bayesian Inference (BI) analysis was performed using MrBayes 3.2.2110, with two independent runs and four simultaneous Markov Chain Monte Carlo runs of 5,000,000 generations each. The resulting trees were sampled every 100,000 generations, with the first 25% discarded as burn-in, and the 50% majority-rule consensus tree was visualized using Figtree V.1.4.2111, with posterior probability (PP) values estimated from trees sampled after the burn-in fraction was discarded.
Ethics approval
The experimental research and field studies on plants, including the collection of plant material, complied with relevant institutional, national, and international guidelines and legislation. The appropriate permissions and/or licenses for collection of plant were obtained for the study.
References
Magauer, M., Schönswetter, P., Jang, T.-S. & Frajman, B. Disentangling relationships within the disjunctly distributed Alyssum ovirense/A. wulfenianum group (Brassicaceae), including description of a novel species from the north-eastern Alps. Bot. J. Linn.Soc. 176(4), 486–505. https://doi.org/10.1111/boj.12214 (2014).
Klimko, M., Nowińska, R., Wilkin, P. & Wiland-Szymańska, J. Comparative leaf micromorphology and anatomy of the dragon tree group of Dracaena (Asparagaceae) and their taxonomic implications. Plant Syst. Evol. 304, 1041–1055. https://doi.org/10.1007/s00606-018-1530-3 (2018).
Montes, B. & Murray, M. G. Application of floral microcharacters to solving taxonomic problems in Argentinean species of the genus Senecio (Asteraceae, Senecioneae). Flora 244–245, 37–52. https://doi.org/10.1016/j.flora.2018.04.003 (2018).
Park, I. et al. Cuscuta species identification based on the morphology of reproductive organs and complete chloroplast genome sequences. Int. J. Mol. Sci. 20, 2726. https://doi.org/10.3390/ijms20112726 (2019).
Choi, B., Kim, S. Y. & Jang, T.-S. Micromorphological and cytological comparisons between Youngia japonica and Y. longiflora using light and scanning electron microscopy. Microscopy Res. Techn. 83, 1456–1463. https://doi.org/10.1002/jemt.23538 (2020).
Karaismailoğlu, M. C. & Güner, Ö. Trichome micromorphology of the genus Stachys sect. Fragilicaulis subsect. Fragilis and its taxonomic implicaitons. Plant Biosyst. 155(4), 833–847. https://doi.org/10.1080/11263504.2020.1801874 (2021).
Kim, H. et al. Micromorphological differentiation of Korean Disporum species using light and scanning electron microscopy. Microscopy Res. Techn. 84, 2614–2624. https://doi.org/10.1002/jemt.23812 (2021).
Moon, H.-K., Vinckier, S., Walker, J. B., Smets, E. & Huysmans, S. A search for phylogenetically informative pollen characters in the subtribe Salviinae (Mentheae: Lamiaceae). Int. J. Plant Sci. 169(3), 455–471. https://doi.org/10.1086/526463 (2008).
Moon, H.-K., Hong, S.-P., Smetes, E. & Huysmans, S. Phylogenetic significance of leaf micromorphology and anatomy in the tribe Mentheae (Nepetoideae: Lamiaceae). Bot. J. Linn. Soc. 160(2), 211–231. https://doi.org/10.1111/j.1095-8339.2009.00979.x (2009).
Moon, H.-K., Smets, E. & Huysmans, S. Phylogeny of tribe Mentheae (Lamiaceae): The story of molecules and micromorphological characters. Taxon 59(4), 1065–1076. https://doi.org/10.1002/tax.594007 (2010).
Tkach, N. et al. Molecular phylogenetics and micromorphology of Australasian Stipeae (Poaceae, Subfmaily Pooideae), and the interrelation of whole-genome duplication and evolutionary radiations in this grass tribe. Front. Pl. Sci. 11, 630788. https://doi.org/10.3389/fpls.2020.630788 (2021).
Oak, M.-K., Yang, S., Choi, G. & Song, J.-H. Systematic palynology in Korean Piperales with special focus on its exine surface ornamentation and orbicule morphology. Sci. Rep. 12, 4142. https://doi.org/10.1038/s41598-022-08105-3 (2022).
Song, Y.-X. et al. Evolution and taxonomic significance of seed micromorphology in Impatiens (Balsaminaceae). Front. Pl. Sci. 13, 835943. https://doi.org/10.3389/fpls.2022.835943 (2022).
Wu, Q.-G. & Cutler, D. F. Taxonomic, evolutionary and ecological implications of the leaf anatomy of rhizomatous Iris species. Bot. J. Linn. Soc. 90, 253–303. https://doi.org/10.1111/j.1095-8339.1985.tb00385.x (1985).
Goldblatt, P. & Le Thomas, A. Pollen apertures, exine sculpturing and phylogeny in Iridaceae subfamily Iridoideae. Rev. Palaeobot. Palynol. 75, 301–315. https://doi.org/10.1016/0034-6667(92)90022-9 (1992).
Mitić, B., Halbritter, H., Šoštarić, R. & Nikolić, T. Pollen morphology of the genus Iris L. (Iridaceae) from Croatia and surrounding area: Taxonomic and phylogenetic implications. Plant Syst. Evol. 299, 271–288. https://doi.org/10.1007/s00606-012-0720-7 (2013).
Guo, J. Comparative micromorphology and anatomy of crested sepals in Iris (Iridaceae). Int. J. Plant Sci. 176, 627–642. https://doi.org/10.1086/682135 (2015).
Wang, L. & Hasenstein, K. H. Seed coat stomata of several Iris species. Flora 224, 24–29. https://doi.org/10.1016/j.flora.2016.07.002 (2016).
Guo, J. & Wilson, C. A. Organization, available space and organ morphology within floral buds of Iris (Iridaceae). Flora 249, 67–76. https://doi.org/10.1016/j.flora.2018.10.001 (2018).
Choi, B., Ahn, Y.-E. & Jang, T.-S. Impications of foliar epidermal micromorphology using light and scanning electron microscopy: A useful tool in taxonomy of Korean irises. Microscopy Res. Techn. https://doi.org/10.1002/jemt.24108 (2022).
Choi, B., Ryu, J. & Jang, T.-S. Can pollen exine ornamentation contribute to species delimitation in Korean Iris L. taxa (Iridaceae)?. Palynology https://doi.org/10.1080/01916122.2022.2061064 (2022).
Wicke, S., Schneeweiss, G. M., Depamphilis, C. W., Muller, K. F. & Quandt, D. The evolution of the plastid chromosome in land plants: Gene content, gene order, gene function. Plant Mol. Biol. 76, 273–297. https://doi.org/10.1007/s11103-011-9762-4 (2011).
Bock, R. & Knoop, V. Genomics of Chloroplasts and Mitochondria (Springer, 2012).
Daniell, H., Lin, C. S., Yu, M. & Chang, W. J. Chloroplast genomes: Diversity, evolution, and applications in genetic engineering. Genome Biol. 17, 134. https://doi.org/10.1186/s13059-016-1004-2 (2016).
Wolfe, K. H., Li, W.-H. & Sharp, P. M. Rates of nucleotide substitution vary greatly among plant mitochondrial, chloroplast, and nuclear DNAs. Proc. Nat. Acad. Sci. USA 84, 9054–9058. https://doi.org/10.1073/pnas.84.24.9054 (1987).
Delannoy, E., Fujii, S., des Colas Francs-Small, C., Brundrett, M. & Small, I. Rampant gene loss in the underground orchid Rhizanthella gardneri highlights evolutionary constraints on plastid genomes. Mol. Biol. Evol. 28, 2077–2086. https://doi.org/10.1093/molbev/msr028 (2011).
Jansen, R. K. et al. Analysis of 81 genes from 64 plastid genomes resolves relationships in angiosperms and identifies genome-scale evolutionary patterns. Proc. Nat. Acad. Sci. USA 104, 19369–19374. https://doi.org/10.1073/pnas.0709121104 (2007).
Parks, M., Cronn, R. & Liston, A. Increasing phylogenetic resolution at low taxonomic levels using massively parallel sequencing of chloroplast genomes. BMC Biol. 7, 1–17. https://doi.org/10.1186/1741-7007-7-84 (2009).
Qiu, Y., Hirsch, C. D., Yang, Y. & Watkins, E. Towards improved molecular identification tools in fine fescue (Festuca L., Poaceae) turfgrasses: Nuclear genome size, ploidy, and chloroplast genome sequencing. Front. genet. 10, 1223. https://doi.org/10.3389/fgene.2019.01223 (2019).
Thode, V. A. & Lohmann, L. G. Comparative chloroplast genomics at low taxonomic levels: A case study using Amphilophium (Bignonieae, Bignoniaceae). Front. Plant sci. 10, 796. https://doi.org/10.3389/fpls.2019.00796 (2019).
Park, I., Song, J.-H., Yang, S. & Moon, B. C. Comparative analysis of Actaea chloroplast genomes and molecular marker development for the identification of authentic Cimicifugae Rhizoma. Plants 9, 157. https://doi.org/10.3390/plants9020157 (2020).
Lee, H.-J. et al. The complete chloroplast genome sequences of Iris sanguinea Donn ex Hornem. Mitochondrial DNA Part A 28, 15–16. https://doi.org/10.3109/19401736.2015.1106521 (2017).
Kang, Y. J. et al. Identification of plastid genomic regions inferring species identity from de novo plastid genome assembly of 14 Korean-native Iris species (Iridaceae). PLoS ONE 15, e0241178. https://doi.org/10.1371/journal.pone.0241178 (2020).
Zhang, C. Y. et al. Testing DNA barcoding in closely related groups of Lysimachia L.(Myrsinaceae). Mol. Ecol. Resour. 12, 98–108. https://doi.org/10.1111/j.1755-0998.2011.03076.x (2012).
Li, Y., Tong, Y. & Xing, F. DNA barcoding evaluation and its taxonomic implications in the recently evolved genus Oberonia Lindl.(Orchidaceae) in China. Front. Plant Sci. 7, 1791. https://doi.org/10.3389/fpls.2016.01791 (2016).
Li, Q.-J. et al. Efficient identification of Pulsatilla (Ranunculaceae) using DNA barcodes and micro-morphological characters. Front. Plant Sci. 10, 1196. https://doi.org/10.3389/fpls.2019.01196 (2019).
Zhao, Y.-T., Noltie, H. J. & Mathew B. Iridaceae. In Flora of China, 24 (eds Wu, Z.Y. & Raven, P.H.) 297–313 (Missouri Botanical Garden Press, 2000).
Wilson, C. A. Patterns of evolution in characters that define Iris subgenera and sections. Aliso 22, 425–433 (2006).
Guo, J. & Wilson, C. A. Molecular phylogeny of crested Iris based on five plastid markers (Iridaceae). Syst. Bot. 38, 987–995. https://doi.org/10.1600/036364413X674724 (2013).
Reeves, G. et al. Molecular systematics of Iridaceae: Evidence from four plastid DNA regions. Am. J. Bot. 88, 2074–2087. https://doi.org/10.2307/3558433 (2001).
Makarevitch, I., Golovnina, K., Scherbik, S. & Blinov, A. Phylogenetic relationships of the Siberian Iris species inferred from noncoding chloroplast DNA sequences. Int. J. Plant. Sci. 164, 229–237. https://doi.org/10.1086/346160 (2003).
Wilson, C. A. Phylogeny of Iris based on chloroplast matK gene and trnK intron sequence data. Mol. Phylogenet. Evol. 33, 402–412. https://doi.org/10.1016/j.ympev.2004.06.013 (2004).
Wilson, C. A. Subgeneric classification in Iris re-examined using chloroplast sequence data. Taxon 60, 27–35. https://doi.org/10.1002/tax.601004 (2011).
Mavrodiev, E. V., Martínez-Azorín, M., Dranishnikov, P. & Crespo, M. B. At least 23 genera instead of one: The case of Iris L. s.l. (Iridaceae). PLoS One 9, e106459. https://doi.org/10.1371/journal.pone.0106459 (2014).
Jiang, Y. L. et al. Phylogenetic analysis of Iris L. from China on chloroplast trnL-F sequences. Biologia 73, 459–466. https://doi.org/10.2478/s11756-018-0063-0 (2018).
Choi, B. et al. Genome size and chromosome number evolution in Korean Iris L. species (Iridaceae Juss.). Plants 9, 1284. https://doi.org/10.3390/plants9101284 (2020).
Lee, T. B. Colored Flora of Korea (Hyangmunsa, 2003).
Ahn, Y. S. Red data book of endangered vascular plants in Korea (5). (Nature & Ecology, 2012).
Dykes, W. R. The genus Iris (Cambridge University Press, 2012).
Crespo, M. B., Martínez-Azorín, M. & Mavrodiev, E. V. Can a rainbow consist of a single colour? A new comprehensive generic arrangement of the ‘Iris sensu latissimo’ clade (Iridaceae), congruent with morphology and molecular data. Phytotaxa 232(1), 78. https://doi.org/10.11646/phytotaxa.232.1.1 (2015).
Sim, J. K., Park, H. D. & Park, S. J. Phylogenetic study of Korean Iris (Iridaceae) based on nrDNA ITS sequences. Korean. J. Pl. Taxon. 32, 33–53. https://doi.org/10.11110/kjpt.2002.32.1.033 (2002).
Wilson, C. A. Phylogenetic relationships among the recognized series in Iris section Limniris. Syst. Bot. 34, 277–284. https://doi.org/10.1600/036364409788606316 (2009).
Chase, M. W. et al. An update of the Angiosperm Phylogeny Group classification for the orders and families of flowering plants: APG IV. Bot. J. Linn. Soc. 181, 1–20. https://doi.org/10.1111/boj.12385 (2016).
Zheng, Y., Meng, T., Bi, X. & Lei, J. Investigation and evaluation of wild Iris resources in Liaoning Province, China. Genet. Resour. Crop Evol. 64, 967–978. https://doi.org/10.1007/s10722-016-0418-8 (2017).
Rudall, P. Taxonomic significance of leaf anatomy in Australasian Iridaceae. Nord. J. Bot. 6, 277–289. https://doi.org/10.1111/j.1756-1051.1986.tb00879.x (1986).
Chaves, A. L. A., Chiavegatto, R. B., Gavilanes, M. L., Benites, F. R. & Techio, V. H. Effect of polyploidy on the leaf epidermis structure of Cynodon dactylon (L.) Pers.(Poaceae). Biologia 73, 1007–1013. https://doi.org/10.2478/s11756-018-0106-6 (2018).
Lima, J. F., Leite, K. R. B., Clark, L. G. & de Oliveira, R. P. Leaf micromorphology in Poaceae subtribe Olyrinae (Bambusoideae) and its systematic implications. Bot. J. Linn. Soc. 192, 184–207. https://doi.org/10.1093/botlinnean/boz071 (2020).
Rodriguez, H. G., Maiti, R. & Ch, A. K. Comparative anatomy of leaf lamina of twenty six woody species of Tamaulipan thornscrub from north eastern Mexico and its significance in taxonomic delimitation and adaptation of the species to xeric environments. Pak. J. Bot 49, 589–596 (2017).
Thordal-Christensen, H., Zhang, Z., Wei, Y. & Collinge, D. B. Subcellular localization of H2O2 in plants. H2O2 accumulation in papillae and hypersensitive response during the barley—powdery mildew interaction. Plant J. 11, 1187–1194. https://doi.org/10.1046/j.1365-313X.1997.11061187.x (1997).
Barthlott, W., Mail, M., Bhushan, B. & Koch, K. Plant surface: Structures and functions for biomimetic innovations. Nano-Micro Lett. 9, 23. https://doi.org/10.1007/s40820-016-0125-1 (2017).
Rudall, P. J., Chen, E. D. & Cullen, E. Evolution and development of monocot stomata. Am. J. Bot. 104, 1122–1141. https://doi.org/10.3732/ajb.1700086 (2017).
Beaulieu, J. M., Leitch, I. J., Patel, S., Pendharkar, A. & Knight, C. A. Genome size is a strong predictor of cell size and stomatal density in angiosperms. New. Phytol. 179, 975–986. https://doi.org/10.1111/j.1469-8137.2008.02528.x (2008).
Hodgson, J. G. et al. Stomatal vs. genome size in angiosperms: The somatic tail wagging the genomic dog?. Ann. Bot. 105, 573–584. https://doi.org/10.1093/aob/mcq011 (2010).
Veselý, P., Bureš, P., Šmarda, P. & Pavlíček, T. Genome size and DNA base composition of geophytes: The mirror of phenology and ecology?. Ann. Bot. 109, 65–75. https://doi.org/10.1093/aob/mcr267 (2012).
Kaur, D. & Singhal, V. K. Meiotic abnormalities affect genetic constitution and pollen viability in dicots from Indian cold deserts. BMC Plant Biol. 19, 10. https://doi.org/10.1186/s12870-018-1596-7 (2019).
Kiran, A. et al. Disruption of carbohydrate and proline metabolism in anthers under low temperature causes pollen sterility in chickpea. Environ. Exp. Bot. 188, 104500. https://doi.org/10.1016/j.envexpbot.2021.104500 (2021).
Galati, B. G. Advanced in Plant Reproductive Biology. In Ubisch bodies in angiosperms (eds Chauhann, M. R. & Pandey, A. K.) (Narendra Publishing House, 2003).
Huysmans, S., El-Ghazaly, G. & Smets, E. Orbicules in angiosperms: Morphology, function, distribution, and relation with tapetum types. Bot. Rev. 64, 240–272. https://doi.org/10.1007/BF02856566 (1998).
Verstraete, B., Groeninckx, I., Smets, E. & Huysmans, S. Phylogenetic signal of orbicules at family level: Rubiaceae as case study. Taxon 60, 742–757. https://doi.org/10.1002/tax.603010 (2011).
Ruggiero, F. & Bedini, G. Phylogenetic and morphologic survey of orbicules in angiosperms. Taxon 69, 543–566. https://doi.org/10.1002/tax.12281 (2020).
Huysmans, S., Verstraete, B., Smets, E. & Chatrou, L. W. Distribution of orbicules in Annonaceae mirrors evolutionary trend in angiosperms. Plant Ecol. Evol. 143, 199–211. https://doi.org/10.5091/plecevo.2010.438 (2010).
Lippi, M. M., Cimoli, F., Maugini, E. & Tani, G. A comparative study of the tapetal behaviour in male fertile and male sterile Iris pallida Lam. during microsporogenesis. Caryologia 47, 109–120. https://doi.org/10.1080/00087114.1994.10797288 (1994).
Song, J. H., Moon, H. K., Oak, M. K. & Hong, S. P. Phylogenetic evaluation of pollen and orbicule morphology in Rosaceae tribe Neillieae (subfamily Amygdaloideae). Bot. J. Linn. Soc. 183, 439–453. https://doi.org/10.1093/botlinnean/bow019 (2017).
Moon, H. K. The phylogenetic potential of orbicules in angiosperms. Korean J. Plant Taxon. 48, 9–23. https://doi.org/10.11110/kjpt.2018.48.1.9 (2018).
Dantas-Queiroz, M. V. & da Luz, C. F. P. Palynotaxonomy of Iridaceae Juss. from Goiás and Tocantins States. Brazil. Braz. J. Bot. 39, 689–707. https://doi.org/10.1007/s40415-015-0239-6 (2016).
Choi, T.-Y. et al. The complete chloroplast genome sequences of the Iris loczyi kanitz (Iridaceae). Mitochondrial DNA Part B 5, 2876–2877. https://doi.org/10.1080/23802359.2020.1790312 (2020).
Kelchner, S. A. The evolution of non-coding chloroplast DNA and its application in plant systematics. Ann. Mo. Bot. Gard. 87(4), 482–498. https://doi.org/10.2307/2666142 (2000).
Shaw, J., Lickey, E. B., Schilling, E. E. & Small, R. L. Comparison of whole chloroplast genome sequences to choose noncoding regions for phylogenetic studies in angiosperms: The tortoise and the hare III. Am. J. Bot. 94, 275–288. https://doi.org/10.3732/ajb.94.3.275 (2007).
Asaf, S. et al. Complete chloroplast genome of Nicotiana otophora and its comparison with related species. Front. Plant Sci. 7, 843. https://doi.org/10.3389/fpls.2016.00843 (2016).
Morton, B. R. & Clegg, M. T. A chloroplast DNA mutational hotspot and gene conversion in a noncoding region near rbcL in the grass family (Poaceae). Curr. Genet. 24, 357–365. https://doi.org/10.1007/BF00336789 (1993).
Maier, R. M., Neckermann, K., Igloi, G. L. & Kössel, H. Complete sequence of the maize chloroplast genome: Gene content, hotspots of divergence and fine tuning of genetic information by transcript editing. J. Mol. Biol. 251, 614–628. https://doi.org/10.1006/jmbi.1995.0460 (1995).
Huo, Y. et al. Complete chloroplast genome sequences of four Allium species: Comparative and phylogenetic analyses. Sci. Rep. 9, 1–14. https://doi.org/10.1038/s41598-019-48708-x (2019).
Song, Y., Zhang, Y., Xu, J., Li, W. & Li, M. Characterization of the complete chloroplast genome sequence of Dalbergia species and its phylogenetic implications. Sci. Rep. 9, 1–10. https://doi.org/10.1038/s41598-019-56727-x (2019).
Liu, L. et al. Chloroplast genome analyses and genomic resource development for epilithic sister genera Oresitrophe and Mukdenia (Saxifragaceae), using genome skimming data. BMC Genomics 19, 1–17. https://doi.org/10.1186/s12864-018-4633-x (2018).
Liu, H. et al. Genome comparison reveals mutation hotspots in the chloroplast genome and phylogenetic relationships of Ormosia species. Biomed Res. Int. 2019, 7265030. https://doi.org/10.1155/2019/7265030 (2019).
Wang, W. et al. DNA barcoding of the Lemnaceae, a family of aquatic monocots. BMC Plant Biol. 10, 1–11. https://doi.org/10.1186/1471-2229-10-205 (2010).
Schroeder, H. et al. Development of molecular markers for determining continental origin of wood from white oaks (Quercus L. sect Quercus). PloS one 11, e0158221. https://doi.org/10.1371/journal.pone.0158221 (2016).
Park, S., An, B. & Park, S. Reconfiguration of the plastid genome in Lamprocapnos spectabilis: IR boundary shifting, inversion, and intraspecific variation. Sci. Rep. 8, 1–14. https://doi.org/10.1038/s41598-018-31938-w (2018).
Zhitao, N. et al. Comparative analysis of Dendrobium plastomes and utility of plastomic mutational hotspots. Sci. Rep. 7, 1–11. https://doi.org/10.1038/s41598-017-02252-8 (2017).
Raubeson, L. A. et al. Comparative chloroplast genomics: Analyses including new sequences from the angiosperms Nuphar advena and Ranunculus macranthus. BMC Genomics 8, 1–27. https://doi.org/10.1186/1471-2164-8-174 (2007).
Smidt, E. D. C. et al. Characterization of sequence variability hotspots in Cranichideae plastomes (Orchidaceae, Orchidoideae). PLoS ONE 15, e0227991. https://doi.org/10.1371/journal.pone.0227991 (2020).
Wang, R.-J. et al. Dynamics and evolution of the inverted repeat-large single copy junctions in the chloroplast genomes of monocots. BMC Evol. Biol. 8, 1–14. https://doi.org/10.1186/1471-2148-8-36 (2008).
Jang, T.-S., Moon, H.-K. & Hong, S.-P. Sex expression, population structure, and floral dimorphism in a gynodioecious herb, Agastache rugosa (Lamiaceae) in Korea. Flora 215, 23–32. https://doi.org/10.1016/j.flora.2015.06.004 (2015).
Jang, T.-S. et al. Chromosomal diversification and karyotype evolution of diploids in the cytologically diverse genus Prospero (Hyacinthaceae). BMC Evol. Biol. 13, 136. https://doi.org/10.1186/1471-2148-13-136 (2013).
Allen, G. C., Flores-Vergara, M., Krasynanski, S., Kumar, S. & Thompson, W. A modified protocol for rapid DNA isolation from plant tissues using cetyltrimethylammonium bromide. Nat. Protoc. 1, 2320–2325. https://doi.org/10.1038/nprot.2006.384 (2006).
Andrews, S. FastQC: A quality control tool for high throughput sequence data. Version 0.11. 2. Website: http://www.bioinformatics.babraham.ac.uk/projects/fastqc (2010).
Zerbino, D. R. & Birney, E. Velvet: Algorithms for de novo short read assembly using de Bruijn graphs. Genome Res. 18, 821–829. https://doi.org/10.1101/gr.074492.107 (2008).
Tillich, M. et al. GeSeq–versatile and accurate annotation of organelle genomes. Nucleic Acids Res. 45, W6–W11. https://doi.org/10.1093/nar/gkx391 (2017).
Carver, T. et al. Artemis and ACT: Viewing, annotating and comparing sequences stored in a relational database. Bioinformatics 24, 2672–2676. https://doi.org/10.1093/bioinformatics/btn529 (2008).
Lowe, T. M. & Eddy, S. R. tRNAscan-SE: A program for improved detection of transfer RNA genes in genomic sequence. Nucleic Acids Res. 25, 955–964. https://doi.org/10.1093/nar/25.5.955 (1997).
Michael, D. et al. RepEx: A web server to extract sequence repeats from protein and DNA sequences. Comput. Biol. Chem. 78, 424–430. https://doi.org/10.1016/j.compbiolchem.2018.12.015 (2019).
Greiner, S., Lehwark, P. & Bock, R. OrganellarGenomeDRAW (OGDRAW) version 1.3. 1: Expanded toolkit for the graphical visualization of organellar genomes. Nucleic Acids Res. 47, W59–W64. https://doi.org/10.1093/nar/gkz238 (2019).
Tamura, K., Stecher, G., Peterson, D., Filipski, A. & Kumar, S. MEGA6: Molecular evolutionary genetics analysis version 6.0. Mol. Biol. Evol. 30, 2725–2729. https://doi.org/10.1093/molbev/mst197 (2013).
Rozas, J. et al. DnaSP 6: DNA sequence polymorphism analysis of large data sets. Mol. Biol. Evol. 34, 3299–3302. https://doi.org/10.1093/molbev/msx248 (2017).
Katoh, K., Misawa, K., Kuma, K. I. & Miyata, T. MAFFT: A novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Res. 30, 3059–3066 (2002).
Hall, T. A. BioEdit: A user-friendly biological sequence alignment editor and analysis program for Windows 95/98/NT. Nucleic Acid Symp. Ser. 41 (1999).
Castresana, J. Selection of conserved blocks from multiple alignments for their use in phylogenetic analysis. Mol. Bio. Evol. 17, 540–552. https://doi.org/10.1093/oxfordjournals.molbev.a026334 (2000).
Darriba, D., Taboada, G. L., Doallo, R. & Posada, D. jModelTest 2: More models, new heuristics and parallel computing. Nat. Methods 9, 772–772. https://doi.org/10.1038/nmeth.2109 (2012).
Stamatakis, A. RAxML version 8: A tool for phylogenetic analysis and post-analysis of large phylogenies. Bioinformatics 30, 1312–1313. https://doi.org/10.1093/bioinformatics/btu033 (2014).
Ronquist, F. et al. MrBayes 3.2: Efficient Bayesian phylogenetic inference and model choice across a large model space. Syst. Biol. 61, 539–542. https://doi.org/10.1093/sysbio/sys029 (2012).
Rambaut, A. FigTree v1. 4. Molecular evolution, phylogenetics and epidemiology. Edinburgh: University of Edinburgh, Institute of Evolutionary Biology (2012).
Acknowledgements
This work was financially supported by the National Research Foundation of Korea (NRF) funded by the Korea government (NRF-2018R1C1B6003170 and NRF-2021R1I1A2045820) to T.-S. Jang. We thank Sun-Yu Kim (Nakdonggang National Institute of Biological Resources), Sungyu Yang (Korea Institute of Oriental Medicine), Seon-Wook Im (National Park Services) and CNUK members for help in collecting materials for this study. We acknowledge the use of the scanning electron microscopy (SEM) by Dr. Jin-Hyub Paik and Mr. Changyoung Lee (Korea Research Institute of Bioscience and Biotechnology, Daejeon, Korea).
Author information
Authors and Affiliations
Contributions
B.C. and T.-S.J. designed and contributed to the original concept of the project. IP performed bioinformatics analysis and molecular experiments. B.C. and K.-C.S. performed DNA and PCR analysis. B.C., J.R., Y.-E.A., J.-H.S., and T.-S.J. performed micromorphological analysis. B.C., S.S., H.-H.M., and T.-S.J. collected and identified the plant materials. B.C., I.P., and T.-S.J. wrote the original draft preparation with revision and editing of the manuscript. All authors contributed to the article and approved the submitted version.
Corresponding author
Ethics declarations
Competing interests
The authors declare no competing interests.
Additional information
Publisher's note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary Information
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Choi, B., Park, I., So, S. et al. Comparative analysis of two Korean irises (Iris ruthenica and I. uniflora, Iridaceae) based on plastome sequencing and micromorphology. Sci Rep 12, 9424 (2022). https://doi.org/10.1038/s41598-022-13528-z
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41598-022-13528-z
This article is cited by
-
Evaluation of the genetic diversity and population structure of reticulated iris accessions in the Iraqi Kurdistan region using SCoT and SRAP markers
Genetic Resources and Crop Evolution (2024)
-
Does the evolution of micromorphology accompany chromosomal changes on dysploid and polyploid levels in the Barnardia japonica complex (Hyacinthaceae)?
BMC Plant Biology (2023)
Comments
By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.