- Open Access
Revisiting chloroplast genomic landscape and annotation towards comparative chloroplast genomes of Rhamnaceae
BMC Plant Biology volume 23, Article number: 59 (2023)
Massive parallel sequencing technologies have enabled the elucidation of plant phylogenetic relationships from chloroplast genomes at a high pace. These include members of the family Rhamnaceae. The current Rhamnaceae phylogenetic tree is from 13 out of 24 Rhamnaceae chloroplast genomes, and only one chloroplast genome of the genus Ventilago is available. Hence, the phylogenetic relationships in Rhamnaceae remain incomplete, and more representative species are needed.
The complete chloroplast genome of Ventilago harmandiana Pierre was outlined using a hybrid assembly of long- and short-read technologies. The accuracy and validity of the final genome were confirmed with PCR amplifications and investigation of coverage depth. Sanger sequencing was used to correct for differences in lengths and nucleotide bases between inverted repeats because of the homopolymers. The phylogenetic trees reconstructed using prevalent methods for phylogenetic inference were topologically similar. The clustering based on codon usage was congruent with the molecular phylogenetic tree. The groups of genera in each tribe were in accordance with tribal classification based on molecular markers. We resolved the phylogenetic relationships among six Hovenia species, three Rhamnus species, and two Ventilago species. Our reconstructed tree provides the most complete and reliable low-level taxonomy to date for the family Rhamnaceae. Similar to other higher plants, the RNA editing mostly resulted in converting serine to leucine. Besides, most genes were subjected to purifying selection. Annotation anomalies, including indel calling errors, unaligned open reading frames of the same gene, inconsistent prediction of intergenic regions, and misannotated genes, were identified in the published chloroplast genomes used in this study. These could be a result of the usual imperfections in computational tools, and/or existing errors in reference genomes. Importantly, these are points of concern with regards to utilizing published chloroplast genomes for comparative genomic analysis.
In summary, we successfully demonstrated the use of comprehensive genomic data, including DNA and amino acid sequences, to build a reliable and high-resolution phylogenetic tree for the family Rhamnaceae. Additionally, our study indicates that the revision of genome annotation before comparative genomic analyses is necessary to prevent the propagation of errors and complications in downstream analysis and interpretation.
Advances in high-throughput sequencing technologies have enabled sequencing of whole chloroplast genomes of numerous plant species on a massive scale. This has led to the broad use of chloroplast genomes in plant evolutionary studies to achieve phylogenetic resolution at the genus and species levels. The key benefits of using chloroplast genomes for phylogenetic research include their haploid state, uniparental inheritance, and high conservation of quadripartite structures. Here, large single-copy (LSC) and small single-copy (SSC) regions are separated by two inverted repeats (IRs: IRa and IRb), whose gene content and order are well conserved [1, 2]. Although variations in chloroplast genomes (for example, genome inversions, deletions, and insertions) rarely occur, small changes in their nature are remarkably informative for phylogenetic reconstruction. Moreover, the average size of chloroplast sequences (120,000–160,000 bp) and the average number of genes (110–130 genes) provide an adequate degree of amplitude and complexity to contain structural and point mutations for extensive evolutionary classification . Whole chloroplast genomes have therefore been successfully used to resolve the phylogenies of numerous plant species [3,4,5,6].
Short-read sequencing technologies, such as Illumina platforms, have been widely used in chloroplast genome studies because of their ability to rapidly produce large, high-accuracy datasets at low cost . However, genome assembly, particularly across two IRs, is challenging when only short reads are used, because the approximate sizes of IRs (10–30 kb ) are typically larger than the generated read length (50–400 bp ). Recent single-molecule sequencing platforms, such as Oxford Nanopore Technologies (ONT) and Pacific Biosciences (PacBio), can reportedly produce a single read of longer than 10 kb to 200 kb for a large chloroplast section [7, 8]. However, when compared to short-read technologies, the per-base error rate of long reads is relatively high (5–10% ). Thus, a combination of long- and short-read datasets is a promising solution that can be apply for chloroplast genomes. It has been reported that approximately 20x coverage of long- and short-read hybrid assemblies can generate a single contig of the entire chloroplast genome . Here, long reads are useful for elucidating chloroplast structure, whereas the few fragmented contigs and sequencing errors can later be polished using short reads owing to their higher accuracy . This is a good practice to obtain high quality genome sequences . Once chloroplast genomes are assembled, they are annotated to identify fundamental features such as protein-coding sequences, tRNA genes, rRNA genes, intergenic regions, and IRs. This process is usually performed using automated annotation tools, such as DOGMA , CpGAVAS  and GeSeq . However, most tools rely on existing genomes deposited in databases (such as GenBank ), which are not completely correct . Therefore, subsequent curation by domain experts is a prerequisite before downstream analysis. Using Rhamnaceae as an example, our study revealed the significance of revisiting genome annotation prior to comparative genomic analysis.
Rhamnaceae is a plant family comprising approximately 55 genera and 950 species, including trees, shrubs, climbers, and herbs [15,16,17]. It belongs to the order Rosales, and several members of the family Rhamnaceae are of great economic and medicinal values. Chinese jujube (Ziziphus jujuba Mill) and Indian jujube (Ziziphus mauritiana) fruits are economically important . Members of genus Hovenia are used for making fine furniture and musical instruments [18,19,20]. Other species, such as Hovenia dulcis , Ventilago species [22, 23] and Ziziphus species , possess medicinal properties. Naturally, Rhamnaceae species reside in many different habitats, ranging from tropical rain forests to moderately arid regions and from sea level to treelines. This family appears to have a high morphological and genetic diversity . The traditional classification of Rhamnaceae tribes relies on morphological features such as floral traits, fruit characteristics, and a few marker genes. Until recently, the basis of taxonomic classification has shifted towards phylogenomic analysis of complete chloroplast genomes. Of over 5300 plant chloroplast genomes, only 24 complete genomes from seven genera of the family Rhamnaceae, namely Berchemia, Berchemiella, Hovenia, Rhamnus, Spyridium, Ventilago, and Ziziphus, have been published (National Center for Biotechnology Information (NCBI) database on July 2021). Notably, only one genome of the Ventilago species from China, Ventilago leiocarpa Benth (V. leiocarpa), is available. In particular, the current Rhamnaceae phylogenetic tree constructed by Wang et al. (2021) contains 13 unique species from six genera (Berchemia, Berchemiella, Hovenia, Rhamnus, Spyridium, and Ziziphus), except for Ventilago . Another tree constructed by Lu et al. (2021) includes V. leiocarpa . However, only seven Rhamnaceae species have been analyzed. Hence, the phylogenetic relationships between Ventilago and other Rhamnaceae organisms remain inconclusive and require more representative species. Ventilago harmandiana Pierre (V. harmandiana) is a plant species of the genus Ventilago within the family Rhamnaceae, which is found across Asia, including China, India, Malaysia, Singapore, and Thailand [22, 28, 29]. Indeed, Ventilago consists of over 40 species, including medicinal plants with numerous therapeutic properties, such as cytotoxicity to cancer cells , antimicrobial activity  and anti-inflammatory effects, as examined in animal models [31, 32]. Our previous study indicated that pyranonaphthoquinones from the heartwood extract of V. harmandiana are promising compounds with cytotoxic and anti-inflammatory properties . Although it shows promise with regards to complementary or alternative therapy, it is yet to be investigated on a genomic level.
To extend the taxonomic coverage of the family Rhamnaceae, we reported the complete chloroplast genome of V. harmandiana using a hybrid assembly of ONT long reads and Illumina HiSeq short reads. We clustered Rhamnaceae members based on their codon usage and reconstructed the phylogenetic tree at low taxonomic levels using all published Rhamnaceae chloroplast genomes, along with the newly sequenced chloroplast genome of V. harmandiana. Notably, short-read sequencing technologies, such as Illumina HiSeq and MiSeq, are the primary platforms for generating DNA sequences for published Rhamnaceae chloroplast genomes. Moreover, there are differences in assembly techniques, annotation tools, choices of reference genomes, and hidden errors in computational prediction. Hence, all chloroplast genomes in this study underwent extensive curation, which included revision of gene locations, correction of gene sequences, and re-annotation of missing genes prior to comparative sequence analyses. This was done to ensure that the newly sequenced chloroplast genome of V. harmandiana and the reconstructed phylogenetic tree of Rhamnaceae were of high quality.
V. Harmandiana chloroplast genome structure and validation
A total of 11,004 raw long reads with an average length of 4231 bp and 636.3 million raw short reads with an average length of approximately 150 bp were generated from the ONT and Illumina HiSeq platforms, respectively. Initially, the size of the draft chloroplast genome based on the hybrid assembly using the long- and short-read datasets was 162,893 bp. A dot plot of the V. harmandiana chloroplast genome illustrates the presence of a quadripartite structure with the two IRs (Fig. 1A). However, no single ONT read fully covered either IR region. In addition, the sequence length of IRs was 13 bp different, and there were 45 mismatched nucleotide bases.
To ensure the correct assembly of the quadripartite structure of the V. harmandiana chloroplast genome, PCR amplification of DNA regions spanning the four IR boundaries was performed (see Additional file 2 Table S1 for primer sequences). Boundary A separates LSC and IRb, Boundary B separates IRb and SSC, Boundary C separates SSC and IRa, and Boundary D separates IRa and LSC (Fig. 1B). The approximate sizes of the amplicons in each DNA region were 951, 1189, 1035, and 1193 nucleotides (nt), respectively (Fig. 1C). Furthermore, the number of spanning reads in the four DNA regions was determined (Additional file 1 Fig. S1). There were only two long reads of size 21,340 and 33,928 nt, spanning across the SSC. The overall read length, which covered the four IR boundaries, varied. However, the number of spanning reads in each region did not differ significantly. In total, there were 252, 256, 244, and 226 reads spanning boundaries A, B, C, and D, respectively. In particular, most reads were spread within 3000 nt from the borders, consisting of 216, 228, 202, and 192 reads in boundaries A, B, C, and D, respectively. Reads longer than 3000 nt accounted for approximately 10% of the total reads (Boundary A = 36, B = 28, C = 42, and D = 34 reads). The longest read for each boundary was 8934, 13,250, 10,159, and 12,531 nt in length for boundaries A, B, C and D, respectively.
The 45 mismatched nucleotide bases between the IRs were then corrected using sequences obtained from Sanger sequencing (Fig. 1D). At this step, the chloroplast genome size was 162,898 bp. The lengths of both IRs were identical, with a size of 26,399 bp. Table 1 lists the 134 genes, including 89 protein-coding genes, 37 tRNA genes, and 8 rRNA genes, identified by automated gene prediction.
Revision of published chloroplast genomes: a case study in Rhamnaceae
Among the 24 Rhamnaceae chloroplast genomes from the NCBI database, we noticed that out of the total number of genes (between 121 and 131 genes), protein-coding genes (between 78 and 86 genes), and tRNA genes (between 34 and 37 genes) varied notably (Additional file 2 Table S2). In particular, the numbers of genes within the same species, such as B. wilsonii, H. acerba, H. dulcis, and Z. jujuba, were different. Moreover, seven protein-coding genes were found to differ between V. harmandiana and V. leiocarpa MT974496. We suspect that this was possibly a result of the usual imperfection in computational predictions , as well as mis-assembly. Therefore, all the chloroplast genomes in this study were extensively refined before further comparative genomic analysis. This was done to avoid propagation of errors that were inherited from the automated genome assemblies and annotation pipelines.
First, we identified annotation anomalies in the 26 published chloroplast genomes (Additional file 2 Table S3). These included unresolved open reading frames, unaligned coding sequences, and missing genes. Arabidopsis thaliana NC_000932 was used as a reference genome to manually correct gene locations, including for example, accD, some of the NADH dehydrogenase and photosystem genes, and unaligned gene sequences like psbL and rpl36. A missing gene was identified by local alignment with the coding sequence of the closest organism, that is, the same species or genus. Overall, the most missing genes were those in the IRa region, and the least missing ones were those in the SSC region. Most gene corrections were made to the B. wilsonii NC_043912 chloroplast genome, whereas the H. acerba MN794429, H. dulcis MT225403, and H. trichocarpa chloroplast genomes contained the highest number of missing genes.
The genes of the IRs were of particular interest. A comparison of gene content and arrangement in the IRs among all organisms revealed that they were highly conserved (Fig. 2A and Additional file 1 Fig. S2). In total, there were 20 copies of genes in the IRs. However, a complete collection of these genes has only been reported in the chloroplast genomes of B. wilsonii NC_043912 and V. harmandiana. In this study, the loss of a rps12 copy from the Z. jujuba MF781071 and F. religiosa chloroplast genomes was recovered by its counterpart. The absence of both copies of trnN-GUU in the R. crenata chloroplast genome was addressed by re-annotation using trnN-GUU of R. globosa chloroplast genome as a reference (Additional file 1 Fig. S2). rps19, ycf1, and ycf15 were absent in most organisms. Especially, rps19 was missing from IRa. The ycf1 gene was not annotated in IRb, whereas ycf15 copies in IRs were not reported in many organisms in this study.
Re-annotation and analysis of rps19 and ycf1 genes
In general, rps19 and ycf1 are located at the borders of the IR regions. In organisms such as C. sativa, all rps19 genes were found in IRb and IRa. The entire rps19 gene was found in the LSC of the R. crenata chloroplast genome, except for its copy in IRa. In other organisms, the IR boundaries were positioned in the coding regions of rps19 and ycf1. In other words, segments of rps19 spanned the LSC (Fig. 2B) and those of ycf1 were integrated into the SSC (Fig. 2C). In accordance with other studies, the contracting or expanding incidence of IR boundaries from or into adjacent single-copy regions leads to the presence of a truncated rps19 copy in IRa and a shortened ycf1 copy in IRb [24, 34]. In this study, size variations between the rps19 and ycf1 copies were commonly observed. The rps19 gene size in the LSC/IRb region was equal in every organism (279 bp), whereas the gene size of its copy in the IRa/LSC region ranged from 48 bp (in H. dulcis MN723868) to 240 bp (in Z. mauritiana and Z. spina-christi) (Fig. 2B). In case of ycf1, there was a short fragment of ycf1 located in the IRb/SSC region with an approximate size of 1102 bp, except for R. heterophylla, whose case the gene size was only 300 bp (Fig. 2C). The average size of the ycf1 large open reading frame in the SSC/IRa region was 5734 bp. The entire Ycf1 protein domain was identified in this region, although part of the domain was matched to the ycf1 pseudogene in the IRb/SSC (Additional file 1 Fig. S3).
In addition, we identified two incidents that could be a result of assembly errors in the R. crenata chloroplast genome. Here, the truncated ycf1 copy and ycf1 appear to contradict other organisms. In this instance, inversion of IRs and SSC in the R. crenata chloroplast genome was observed after alignment with the other Rhamnus species (Fig. 2D). Secondly, duplicated rps19 was completely lost from IRa. In addition, we identified a shift in the origin coordinates of the H. acerba MN794429 chloroplast genome (Additional file 1 Fig. S4). Here, the start coordinates were different from those of the rest of the organisms in this study. In particular, the first coordinate of the H. acerba MN794429 chloroplast genome began at the 5′ end of IRa, while the others began at the 5′ end of LSC.
Re-annotation and analysis of ycf15 and infA genes
Among the genes in the IRs, copies of ycf15 were absent in 74% of the organisms in this study. In particular, ycf15 copies were identified in seven Rhamnaceae chloroplast genomes, namely B. wilsonii NC_043912, H. acerba MN782301, H. dulcis MN723868, S. parvifolium, V. harmandiana, Z. jujuba MF781071, and Z. jujuba NC_030299. In case of the outgroup, there were originally two copies of ycf15 in the F. religiosa chloroplast genome. The gene size of ycf15 was 192 bp, containing no introns. Nonetheless, we were unable to predict the Ycf15 protein domain based on its protein sequence (YP_009349652). Additionally, ycf15 copies of C. sativa were retrieved from ycf15 pseudogenes of its closest species (C. sativa NC_026562). It appeared that the identified ycf15 carried in-frame stop codons, which matched the fragment of the Ycf15 domain.
Multiple sequence alignment was then performed to examine the characteristics of ycf15 among the seven Rhamnaceae species (Additional file 1 Fig. S5). First, we located a missing T-base in both copies of the ycf15 gene of V. harmandiana. Interestingly, the ycf15 gene of B. wilsonii NC_043912 included an intervening sequence or a 278-bp intron, whereas in the rest of the species, ycf15 came in one piece. Moreover, the translated ycf15 of B. wilsonii NC_043912 showed a longer match with the Ycf15 domain fragment and showed a sequence match from the first amino acid onwards, unlike other organisms (Additional file 1 Fig. S5). This ycf15 annotation in Rhamnaceae appears dubious because of its ambiguous intron structure and protein domain matching.
At this step, ycf15 of N. tabacum Z00044 (tobacco) was chosen as a reference gene to revise the sequences of the previously identified ycf15. ycf15 of N. tabacum is present intact, and a full-length transcript has been reported in Schmitz-Linneweber’s study . Furthermore, the entire Ycf15 protein domain was detected in the protein sequence (CAA77386). Comparative sequence analysis revealed that the ycf15 genes of B. wilsonii NC_043912, H. acerba MN782301, H. dulcis MN723868, S. parvifolium, V. harmandiana, Z. jujuba MF781071, and Z. jujuba NC_030299, contained intervening sequences of sizes 278, 294, 294, 277, 278, 294, and 294 bp, respectively (Fig. 3A). Moreover, a common TA-gap was observed between the sequences. Similar results were observed when the ycf15 gene of Barbeya oleoides NC_040984 was re-annotated with the same reference (Additional file 1 Fig. S6). The chloroplast genome of Barbeya oleoides was used for genome mapping. Hence, it was skeptical whether the TA-gap was an indel mutation of Rosales lineages or an indel calling error of the genome mapping pipeline. Herein, the TA-gap in the V. harmandiana sequence was manually corrected, which could resolve the in-frame stop codon (Fig. 3B) and lead to the identification of the full-length Ycf15 domain. This indicated that the TA-gap was caused by an error in the genome mapping process, causing in-frame stop codons in the translated ycf15 genes.
The ycf15 gene of N. tabacum was used to re-annotate the missing ycf15 copies in the other organisms in this study. Common characteristics, including an intervening sequence and TA-gap, existed in all Rhamnaceae chloroplast genomes (Additional file 1 Fig. S7). In both C. sativa and F. religiosa chloroplast genomes, a portion of the ycf15 gene and TA-gap were detected (Additional file 1 Fig. S6). This part of the gene was in line with the second exon of the ycf15 in Rhamnaceae. However, it could be interpreted as a pseudogene because of the absence of an open reading frame. Therefore, further investigation is needed to confirm the existence and structure of ycf15 in both species.
The infA is a single-copy gene that has been lost in the chloroplast genomes of several species . In this study, infA was annotated in V. harmandiana along with five Ziziphus species (Z. jujuba KX266829, Z. jujuba KX266830, Z. jujuba MW160433, Z. mauritiana NC_037151, and Z. spina-christi NC_037152), with the exception of Z. incurva, Z. jujuba MF781071, and Z. jujuba NC_030299. The infA genes of Z. jujuba MF781071 and Z. jujuba NC_030299Z were entirely re-annotated using the infA sequence of Z. jujuba MW160433. In contrast, the infA gene of V. hamandiana was used as a reference to study the infA gene of V. leiocarpa. However, the discovered gene contained in-frame stop codons, possibly because of an A-indel error in the infA sequence of V. leiocarpa (Additional file 1 Fig. S8).
V. Harmandiana chloroplast genome features and content
A newly sequenced V. harmandiana chloroplast genome is proposed in this study. It has a circular quadripartite structure with a size of 162,904 bp (Fig. 4A). The LSC and SSC regions separated by a pair of IRs (the size of each IR being 26,401 bp) are 90,807 and 19,295 bp long, respectively (Additional file 2 Table S2). The chloroplast genome size of V. harmandiana is above the average size of Rhamnaceae chloroplast genomes (161,144 bp) and is 1024 bp larger than that of its closest species, V. leiocarpa. The GC content of V. harmandiana chloroplast genome is 36.60%, which is similar to that of H. dulcis NC_050971 and H. dulcis MN723868. However, it is slightly lower than the average GC content of Rhamnaceae (36.89%).
There are 134 genes in the V. harmandiana chloroplast genome, including 89 protein-coding genes, 37 tRNA genes, and 8 rRNA genes (Table 1). Among these, 94 genes are single-copy and 20 genes are duplicated in the IRs (Table 1). Table 2 lists the genes and their functions. Eighteen unique genes contain one intron, and the other two genes, namely ycf3 and clpP1, contain two introns. rps12 is a trans-spliced gene, one exon of which is in the LSC, and two copies of exons are in the IR regions (Fig. 4A). The matK gene resides in the intron of the trnK-UUU gene. The tRNA genes and codon patterns of all 20 amino acids were identified (Table 3). Among the three stop codons, namely TAA, TAG, and TGA, TAA is the most abundant. Apart from stop codons, codon usage analysis identified AAA (4.16%) and TGC (0.28%) as the most and least abundant codons, respectively (Fig. 4B and Table 3). On the other hand, the most and least abundant amino acids are leucine (10.51%) and cysteine (1.12%), respectively (Fig. 4C and Table 3).
Comparative sequence analysis unraveling the evolution of V. harmandiana
In total, this study included 25 chloroplast genomes from Rhamnaceae and two chloroplast genomes for the outgroup, including C. sativa from the family Cannabaceae and F. religiosa from the family Moraceae (Additional file 2 Table S2). Among the 25 chloroplast genomes of the Rhamnaceae family, eight were from the Ziziphus genus, including five from Ziziphus jujuba. Complete chloroplast genomes, LSC, SSC, and IR regions had average sizes of 161,144 bp, 89,136 bp, 19,109 bp, and 26,449 bp, respectively. The chloroplast genome and LSC sizes of H. dulcis NC_050971 were the largest, whereas those of V. harmandiana were the second largest. R. heterophylla had the smallest LSC, IR, and chloroplast genome sizes, but its SSC size was the largest. After revision of the chloroplast genomes in this study, the number of tRNA (37 genes) and rRNA (8 genes) genes was the same in all species. On an average, the total number of genes was 133. The number of genes in the R. crenata chloroplast genome was less than that in other organisms because the rps19 copy in the IRa was not detectable. As the infA gene was re-annotated, there were more protein-coding genes (89 genes) in both Ventilago species, and all Z. jujuba, Z. mauritiana, and Z. spina-christi chloroplast genomes, resulting in 134 genes in these species.
Codon and amino acid usage analyses were performed on 86 protein-coding genes of each chloroplast genome. Both copies of ycf15 and infA were excluded, as their ability to encode a functional protein remained doubtful [36, 37]. In addition, infA was found to be lost in several organisms. TAA (0.22% ± 0.084) was the preferred stop codon in Rhamnaceae. Apart from stop codons, AAA (4.12% ± 0.065) and TGC (0.28% ± 0.009) were the most and least abundant codons, respectively. On the other hand, the most and least abundant amino acids were leucine (10.51% ± 0.056) and cysteine (1.15% ± 0.015), respectively (Additional file 3 Table S5). PCA  was performed to observe codon usage patterns. Two Rhamnaceae groups, ziziphoid and rhamnoid, had distinct codon usage preferences (Fig. 5A). In particular, inter-group variation was clearly observed, while Rhamnaceae members were closely clustered within the same genus. However, H. acerba MN794429 and Z. jujuba NC_030299 were more distant from the other organisms in their genera. In this case, there were differences in gene size between Z. jujuba NC_030299 and the rest of Z. jujuba. These genes were the atpF, rpl16, rps16, and rps19 copies in IRa, ycf2, and both copies of ycf1. In particular, the atpF coding sequence of Z. jujuba NC_030299 was 42 bp longer than the other Z. jujuba. This was due to its shorter intergenic region than that of Z. jujuba (Additional file 1 Fig. S9A). Similarly, the divergent structure of the clpP gene was observed in H. acerba, with a 36 bp longer coding sequence in H. acerba MN794429 than that in H. acerba MN782301 (Additional file 1 Fig. S9B).
The phylogenetic trees of 78 orthologous proteins (Additional file 1 Table S4) were reconstructed using RAxML, ML, MP, and BI methods (Fig. 5B and Additional file 1 Fig. S10A-C). Additionally, the tree reconstructed from the orthologous genes using the RAxML method was observed (Additional file 1 Fig. S10D). The rps19 copy in the IRb and the long ycf1 copy in the IRa were included in the analysis; only one copy was applied for the other IR genes. To the best of our knowledge, this is the highest number of orthologs as well as organisms available to reconstruct the phylogenetic tree of the family Rhamnaceae. Overall, the reconstructed trees were topologically similar, with strong bootstrap values or Bayesian posterior probability (value close to 100) supporting the majority of nodes. The Rhamnaceae chloroplast genome sequences included in this study were from two groups (ziziphoid and rhamnoid), four tribes (Paliureae, Pomaderreae, Rhamneae, and Ventilagineae), and seven genera (Berchemia, Berchemiella, Hovenia, Rhamnus, Spyridium, Ventilago, and Ziziphus). Accordingly, the phylogenetic tree contained two large groups of ziziphoid and rhamnoid (Fig. 5B). The ziziphoid group included the tribes Pomaderreae and Paliureae, whereas the rhamnoid group included the tribes Rhamneae and Ventilagineae. This clustering was congruent with a tribal classification based on molecular markers, such as rbcL, trnL-F, and ITS regions [39, 40]. In the rhamnoid clade, V. harmandiana and V. leiocarpa formed a sister clade with Berchemia, Berchemiella, and Rhamnus. Both Berchemiella species were initially grouped into Berchemia berchemiifolia before being grouped into another Berchemia species. In addition, we resolved the phylogenetic relationships among the three Rhamnus species. Here, R. heterophylla was a sister to R. taquetii and clustered with R. globosa and R. crenata. In the ziziphoid clade, there were two groups of Ziziphus species, in which all five Z. jujuba clustered together and formed a sister clade to the one containing Z. mauritiana, Z. spina-christi, and Z. incurva. The recent phylogeny grouped H. acerba MN794429, H. dulcis MT225403, and H. trichocarpa into one clade , which further became a sister to H. acerba MN782301 in our tree.
Characteristics and comparisons of Rhamnaceae chloroplast genomes
Simple nucleotide repeats and long repeats
Among Rhamnaceae chloroplast genomes, the most abundant repeats were the mononucleotides (71.87%, Fig. 6A), and the most dominant SSR was AT-rich (Additional file 4 Table S6). Hexanucleotide repeats were found only in the genus Hovenia, R. heterophylla, R. taquetii, S. parvifolium, V. leiocarpa Z. spina-christi, and Z. incurva. The number of SSRs in the genus Ventilago was higher than that of the other Rhamnaceae (V. harmandiana = 167 SSRs and V. leiocarpa = 135 SSRs), while the Ziziphus and B. flavescens chloroplast genomes contained less than 100 SSRs (Additional file 1 Fig. S11A). Most SSRs were found in the LSC region, whereas the lowest proportion of SSRs were observed in the IRs (Additional file 1 Fig. S11B). Only 1.64% of SSRs were identified in the IR regions of V. harmandiana, which was less than the other Rhamnaceae. The long repeat analysis identified the palindromic repeat as a major long repeat type (48.9%) in Rhamnaceae (Fig. 6B). However, the number of the forward repeats was higher than the palindromic repeats in V. harmandiana and R. heterophylla chloroplast genomes, whereas the number of the forward and palindromic repeats in V. leiocarpa were equal (Additional file 1 Fig. S11C). Majorly, the long repeats located in the LSC and IR regions, and the lowest proportion was observed in the SSC (Additional file 1 Fig. S11D). However, a higher proportion of the long repeats were found in the SSC than the IRs for R. heterophylla. This was in relation to the finding of a very short ycf1 gene in R. heterophylla in the IR regions compared to the other Rhamnaceae.
RNA editing sites
On average, there were 160 RNA editing sites in the Rhamnaceae chloroplast genomes. The most RNA editing sites were found in R. crenata (174 sites), and the lowest number of RNA editing sites were observed in H. dulcis MN723868 and H. dulcis NC_050971 (153 sites, Fig. 6C). The rpoC2 and ycf2 genes of both H. acerba, H. dulcis MT225403 and H. trichocarpa contained the same number of RNA editing sites (16 sites). The rpoC2 gene contained the most RNA editing sites for the Ventilago (19 sites), while the most RNA editing sites were found in the ycf2 gene for the other of the Rhamnaceae. Here, 21 RNA editing sites were observed in the ycf2 gene of R. crenata. In Rhamnaceae chloroplast genomes, most of the RNA editing resulted in the conversion of serine to leucine (Additional file 5 Table S7). For the Ventilago, the second-most conversion was from alanine to valine.
Substitution rates and nucleotide diversity
The Ka/Ks ratio represents selective pressure, which Ka/Ks < 1.0 for purifying, Ka/Ks = 1.0 for neutral, and Ka/Ks > 1.0 for positive selection . For the Rhamnaceae chloroplast genomes, the Ka/Ks ratios of most genes were less than 1.0, meanwhile, those of the clpP and rpoC1 genes were more than 1.0 (Additional file 6 Table S8), indicating both genes had undergone positive selection. Specifically, the Ka/Ks values of the clpP gene were higher than 1.0 by comparing V. harmandiana to the other Rhamnaceae, except for V. leiocarpa (Fig. 7 and Additional file 7 Table S9). The rps16 and rpl23 genes had the Ka/Ks > 1.0 in the Ventilago compared to the Ziziphus and the Hovenia, respectively (Fig. 7). The rpoC1 and ycf1 were less than 1.0 in the Ventilago compared to the Ziziphus (Fig. 7). The positive selection was observed in the rps4, rpl20 and ycf4 when comparing between both Ventilago. The nucleotide diversity (π) of the Rhamnaceae orthologous genes ranged from 0.002 to 0.069 with an average diversity of 0.026 (Additional file 6 Table S8). The rpl22 and ndhB exhibited the highest and lowest nucleotide diversity, respectively. In particular, the π values of 31 genes (39.7% of the protein-coding genes) were higher than the average. Those genes were, for instance, the rpl22, ycf1, clpP, and matK, of which the π values were greater than 0.05. Whereas the relatively low π values (π < 0.01) were observed among the ndhB, petG, psbJ, psbL, psbZ, rpl2, rps7, ycf2, psbJ, petG, and ycf2 genes.
Even though genome assembly using a combination of long and short reads achieves higher accuracy than that using long or short reads alone, additional experiments and post-processing of the draft assembly are still necessary [7, 42]. In this study, we highlight the importance of these factors in improving the accuracy of genome assembly. Using the newly sequenced chloroplast genome of V. harmandiana as a case study, the genome was subjected to extensive investigation and manual correction to ensure high quality and validity. Generally, the presence of a circular DNA structure and two identical IRs within chloroplast genomes is a key challenge for automated genome assemblies . In our case, there were no long ONT reads covering the entire IR region. However, the absolute chloroplast structure of V. harmandiana was confirmed by PCR amplification of specific DNA regions, together with the number of spanning reads over the IR boundaries. Frequent errors in the ONT reads due to long homopolymer stretches and base modification  were polished by short reads. The remaining errors required amendment after genome assembly [7, 45, 46]. Therefore, per-base mismatches between the IRs in the V. harmandiana chloroplast genome were corrected using highly accurate reads from Sanger sequencing. Our findings suggest that major challenges in genome assemblies can be overcome by complementing traditional approaches.
The availability of big data-sharing resources, such as the NCBI database, offers new opportunities to conduct various studies on genomic data. Nevertheless, it is unlikely that all published genomes were entirely assembled and annotated to a high standard. This is because of the usual imperfection of computational tools, lack of standardized bioinformatics workflows, and uncorrected errors in existing genomes [14, 33, 47]. In this study, we extensively revised the annotation of the published chloroplast genomes of family Rhamnaceae, as unrevealed errors would complicate the subsequent evolutionary analysis of Rhamnaceae species. Interestingly, we identified annotation anomalies in all the published chloroplast genomes covered in this study. These included inconsistent intron splice sites of the same gene in the same species, in-frame stop codons within coding sequences, and missing genes.
Missing IR genes, including rps19, ycf1, and ycf15, were of particular interest. A copy of either rps19 or ycf1 was often misannotated. As the rps19 and ycf1 genes are located at the borders of the IR regions, this could possibly be a result of incomplete genome assembly. In addition, the observed size variations between the rps19 and ycf1 copies are considered to be a result of the contraction or expansion of the IR regions . We observed high variation in the ycf1 gene as well as the existence of a large open reading frame. Therefore, ycf1 has been proposed as a DNA barcode for species identification [48, 49]. Moreover, a different orientation of SSC was observed in the R. crenata chloroplast genome. This could be either a genome assembly error or an existing form of heteroplasmy, as found in the chloroplast genomes of some plants . Nonetheless, duplicated rps19 was completely lost from the IRa of the chloroplast genome. Short-read sequencing is the main sequencing platform used in the study on R. crenata . Furthermore, it is well known that IR assembly is particularly difficult when the IR size exceeds the read length . In this case, we speculated that it was a defect in genome assembly.
Another unusual finding in this study was the ycf15 gene. The possibility that ycf15 is a valid protein-coding gene has not yet been proclaimed. However, it has also been annotated in several flowering plants [35, 37]. Schmitz-Linneweber et al. (2001) reported two forms of the ycf15 gene: 1) they identified an intervening sequence of size 250–300 bp in the ycf15 of Arabidopsis thaliana, Spinacia oleracea, Zea mays, and Oenothera berteriana, and 2) they found intact ycf15 genes in the plastomes of Nicotiana tabacum, Cuscuta reflexa, and Epifagus virginiana . It initially appeared that intact ycf15 was the major gene structure among the Rhamnaceae members in this study. However, a different assumption was made based on interclade sequence matching and protein domain analysis. Moreover, the presence of an in-frame stop codon was possibly due to a TA-indel error in the second exon of ycf15, because the full-length Ycf15 protein domain was discovered after manual correction of the TA-indel error in V. harmandiana. Meanwhile, the truncated Ycf15 domain on the C-terminal side is present in other organisms. Additional evidence (such as intron information) to train gene prediction pipelines and extrinsic analysis (such as protein domain prediction) can be used to aid gene annotation. After revision of the chloroplast genomes in this study, the results showed that the numbers of protein-coding genes, tRNA genes, and rRNA genes, were similar.
The phylogeny of Rhamnaceae was then re-evaluated based on the revised chloroplast genomes. Rhamnaceae is a large plant family with a high level of morphological and genetic diversity. Previously, the classification of Rhamnaceae relied on fruit characteristics, resulting in the delimitation of two large heterogeneous tribes. The revision of tribal classification, as well as the study of taxonomic relationships between Rhamnaceae and other families (Barbeyaceae, Dirachmaceae, Elaeagnaceae, Moraceae, Rosaceae, Ulmaceae, and Urticaceae), is based on rbcL and trnL-F plastid genes combined with morphological information [15, 40]. Molecular phylogenetic analysis revealed 11 tribes  and three major groups of Rhamnaceae: ziziphoid, rhamnoid, and ampelozizyphoid groups [15, 16]. The majority of Rhamnaceae species belong to ziziphoid and rhamnoid groups . Although rbcL and trnL-F sequence data have been used for intrafamilial and suprageneric phylogenetic studies , more genetic information is needed for a better resolution of Rhamnaceae phylogeny. In particular, the combination of the trnL-F region of chloroplast DNA and the nuclear ribosomal DNA internal transcribed spacer (ITS) regions has been used to study Rhamnaceae tribes and genera [39, 51, 52]. These studies largely support the taxonomic study by Richardson et al.  and successfully validate controversial genera such as Rhamnus and Frangula. However, the phylogenetic relationships of polyphyletic genera (for example, Ziziphus) and genera without assigned tribes, remain unresolved by using only a few marker genes. Moreover, incongruence between genes can be observed by using too few genes, which makes phylogenetic reconstruction more error prone . More genetic data are therefore urgently needed.
The phylogenetic trees of Rhamnaceae have been built based on whole chloroplast genomes. However, the use of highly conserved and varied loci in phylogenetic studies requires consideration. Highly conserved genetic information usually resolves higher levels of phylogenetic trees (for example, family and genus) than highly variable genetic information. Conversely, the inclusion of exceptional insertions or deletions in the phylogenetic analysis could result in bias clustering towards a specific taxon. Therefore, orthologous identification was performed prior to phylogenetic reconstruction in this study. The phylogenetic tree at low taxonomic levels of Rhamnaceae was reconstructed using 78 orthologous protein-coding genes from 25 Rhamnaceae members and two organisms for the outgroup. As a greater number of Rhamnaceae species were included in the analysis, our phylogenetic tree added up the coverage of phylogenetic relationships between Rhamnaceae species to that of other studies [20, 24, 54, 55]. Furthermore, the clusters of Rhamnaceae organisms based on codon usage were in line with the molecular phylogenetic tree. Minor deviations of Z. jujuba NC_030299 and H. acerba MN794429 from their ziziphoid groups were observed based on codon usage. This could be a result of the imprecise prediction of intron-splice sites. Further investigation is needed to resolve the unaligned genes in both the Z. jujuba and H. acerba chloroplast genomes.
Additionally, the SSRs were reported as informative DNA markers to differentiate organisms at the lower taxonomic levels because of the high length variation and polymorphism [56, 57]. These regions were successfully used for the analysis of intraspecific genetic variation in the Ziziphus  and ginsengs . Consistently, we found the proportion of SSRs in each chloroplast region was different between species, but it was fairly similar within the same species, such as B. wilsonii, H. acerba and Z. jujuba. Moreover, because short polyadenine (polyA) or polythymine (polyT) repeats are the main component of SSRs in chloroplast genomes , the most dominant A/T motifs may contribute to overall high AT content of the Rhamnaceae chloroplast genomes. RNA editing is the modification of the transcripts that is observed in viruses and various eukaryotes including plants . Our study found that most of the RNA editing sites led to the conversion of serine to leucine, which is in accordance with the general characteristic of RNA editing in higher plants [61, 62]. Besides, the number of predicted editing sites was similar among closely related species. The analysis of nucleotide substitution of the orthologous genes reflected the high conservation of the chloroplast genomes, as most genes were strongly subjected to purifying selection in the evolutionary process. However, the clpP gene was strongly subjected to positive selection, and had relatively high nucleotide diversity. This could infer that the gene could be important in the adaptive evolution of the Rhamnaceae. The positive selection of the clpP in several plant lineages was found to be involved in repeated duplication .
Our study shows that genomic information at both the DNA and protein levels could support a tribal classification of Rhamnaceae and could clarify the phylogeny at low taxonomic levels. The completeness of the genomes is a basic requirement for subsequent comparative genomic analyses. In this study, we also demonstrate that extensive corrections of genome sequences and revision of annotations are essential, as errors in existing DNA sequence data could propagate to newly sequenced genomes and lead to endless flaws in consecutive genomic analyses.
In this study, we made use of the key advantages of different DNA sequencing platforms, to congregate the entire chloroplast genome of V. harmandiana and to ensure its high quality. In particular, ONT long reads were used to generate a draft assembly, and Illumina HiSeq short reads were integrated to polish the genome. Moreover, we demonstrated that a combination of PCR amplification, investigation of coverage depth, and Sanger sequencing for nucleotide base corrections could lead to elucidation of the complete chloroplast genome, even if the read length was shorter than the IR size. We then examined the features and content of the chloroplast genome.
Major gene functions of the V. harmandiana chloroplast genome, such as photosynthesis and genome replication, were as described in other plants. The reported chloroplast genome is not only a useful resource, but will also aid in the genetic exploration of this medicinal plant, as well as in the study of Rhamnaceae phylogeny. In this regard, we report the most complete phylogenetic tree of Rhamnaceae based on chloroplast genome information. It included a higher number of Rhamnaceae species than that in the dispersed phylogenetic relationships elucidated in other studies. However, during genome revision, we identified putative assembly errors and annotation anomalies in published chloroplast genomes of this family. This indicates the importance of revising the genome annotation prior to genomic analysis. Moreover, reviewing the completeness and correctness of the annotation before genome submission is superior. This is necessary to avoid the propagation of errors from reference genomes to newly assembled genomes, which could be carried on to downstream analysis and biological interpretation.
Plant material and sampling
Sample collection of V. harmandiana was permitted by the private land owner in Trang province, Thailand, Mr. Wanlop Pengphan. The collection of the V. harmandiana covering various plant parts for research and related purposes was done with the permission and supervision of the local authority. Plant samples were collected as previously described . Briefly, V. harmandiana leaves were collected in March 2019 in Trang Province, Thailand (lat. 7°47′12.8″ N, long. 99°30′55.0″ E; altitude 104 m a.s.l.). The collected samples were identified by the author, Dr. Narong Nuntasaen from Department of National Parks, Wildlife and Plant Conservation, Ministry of Natural Resources and Environment. All samples with the voucher specimen accession code, BKF no. 35203, were deposited at the Forest Herbarium, Department of National Parks, Wildlife and Plant Conservation in Bangkok, Thailand. The samples were immediately washed with tap water to remove dirt and kept on dry ice during transport to the laboratory. The samples were stored at − 80 °C until use.
The leaves were soaked in 0.05% Tween 20 to remove fungal spores and bacterial cells from their surfaces, and washed several times with distilled water. To extract DNA, 1 g of young leaves was ground to a fine powder using liquid nitrogen. Then, 7.5 ml of freshly prepared CTAB buffer (20 mM EDTA pH 8.0, 100 mM Tris-HCl pH 8.0, 1.5 M NaCl, 2% CTAB, 1% β-mercaptoethanol, 2% polyvinylpyrrolidone M.W. 10,000) was added, and incubated at 60 °C for 2 h with intermittent shaking every 10 min. The samples were centrifuged at 15,000 rpm for 30 min at room temperature and the aqueous phase was transferred to a new tube. Next, 1 V of phenol-chloroform-isoamyl alcohol (25:24:1) was added, inverted gently for 1 min, and centrifuged at 15,000 rpm for 15 min. This step was repeated using chloroform until the upper phase was translucent and no interphase protein appeared. The aqueous phase (upper phase) was transferred into a new tube without chloroform (lower phase). To precipitate the DNA, 2 V of isopropanol and 1/3 V of 3 M sodium acetate (pH 5.2) were added. The sample was then kept at − 20 °C for 1 h, followed by centrifugation at 15,000 rpm for 15 min. The DNA pellet was washed twice with 70% ethanol and absolute ethanol, and resuspended in TE buffer. DNA samples were supplemented with DNase-free RNase A (20 μg/ml) and incubated for 30 min at 37 °C to remove RNA. Finally, the DNA was re-purified using QIAGEN Genomic-tip 100/G (cat no.13343) according to the manufacturer’s protocol to obtain high-quality DNA (OD 260/280 and 260/230 of 2.0).
Chloroplast genome sequencing
MinION sequencing: To obtain the chloroplast sequencing reads, two library kits were used for DNA library preparation: the Rapid Barcoding Sequencing kit (SQK-RAD004, ONT, UK) and the 1D Genomic DNA sequencing kit (SQK-LSK109, ONT). A total of 500 ng of DNA was used for SQK-RAD004 input and 1500 ng was used for SQK-LSK109 input. We followed the protocol recommended by ONT, except for the DNA shearing step. Each DNA library was loaded onto an R9.4/FLO-MIN106 flow cell (ONT) on a MinION Mk1B for 48 h. Base-calling was performed using the local-based software GUPPY version v2.1.3 (ONT).
PromethION sequencing: To obtain the highest sequencing yield of long reads, the PromethION platform was selected for gDNA sequencing. The DNA library was prepared using SQK-LSK109 (ONT). A total of 2500 ng of DNA was used as input. The DNA library was loaded onto a PromethION flow cell (ONT) and incubated for 48 h. Base-calling was performed using the local-based software GUPPY version v2.1.3 (ONT).
A short-read high-throughput Illumina platform (HiSeq, Illumina, Inc., USA) was used to improve the accuracy of the final nanopore sequence. A TruSeq DNA polymerase chain reaction (PCR)-free library was prepared and 100-bp paired-end reads were generated.
The long- and short-read raw data of the chloroplast has been deposited in the Sequence Read Archive (SRA) repository, https://www.ncbi.nlm.nih.gov/sra/PRJNA906747.
Chloroplast genome assembly
Hybrid assemblies of ONT (combined reads from MinION and PromethION sequencing) and Illumina data were performed using default settings for circular chloroplast genomes. The ONT adapters in Nanopore reads were trimmed using Porechop v0.2.3 (https://github.com/rrwick/Porechop). The whole genome Nanopore reads with a mean quality score of 9 and a length of 1000 bases were retained from QC step using NanoFilt v2.5.0 . The high-quality reads were then mapped to the closely related species chloroplast genome of Barbeya oleoides NC_040984.1, to identify chloroplast reads using Minimap2 . To reduce complexity, all mapped reads were subjected to de novo assembly using Unicycler v0.4.7 . Six rounds of Pilon v1.23  polishing with Illumina data were applied iteratively on the circular draft chloroplast genome.
Validation of chloroplast inverted repeat regions
PCR amplification of DNA regions spanning over the four IR boundaries of the circular draft chloroplast genome was performed to determine the quadripartite structure of the V. harmandiana chloroplast genome (Fig. 1C and Additional file 1 Fig. S12). Primer sets were designed using the assembled sequences. Four pairs of PCR primers were designed to cover the LSC-IRb junction, IRb-SSC junction, SSC-IRa junction, and IRa-LSC junction (primers VharA–D, Additional file 2 Table S1 and Fig. 1B). Specific primers for the 18S rDNA gene (18S_FA: AAC CTG GTT CCT GCC AG and 18S_RB: TGA TCC TTC TGC AGG TTC AC) were used as positive controls . Five PCR reactions were performed, including reactions for the four boundaries and the positive control. Each PCR reaction mixture consisted of 0.2 μM of each primer, 200 μM of each dNTP, 1X of ThermoPol® Reaction Buffer (New England Biolabs, USA), 2.5 U of Taq DNA polymerase (New England Biolabs, USA), and 15 ng of the chloroplast DNA. PCR reaction mixtures were adjusted to a final volume of 50 μL using sterile nuclease-free water. The PCR conditions were as follows: initial denaturation at 95 °C for 5 min; 30 cycles of 95 °C for 5 min, 56 °C for 30 s, and 68 °C for 2 min; and final extension at 68 °C for 10 min. The amplicons were analyzed using 1.5% agarose gel electrophoresis with FluoroVue™ Nucleic Acid Gel Stain (SmoBio, Taiwan) and documented using G:BOX Chemi XRQ gel documentation (Syngene™, USA).
Local sequence alignment was conducted between IRb and reverse-complemented IRa (revIRa) to identify mismatched nucleotide bases between the IRs, and the correct bases were determined by Sanger sequencing. Fourteen primer pairs were designed to cover all 25 mismatched regions within the two IRs (primers VharIR1–14; Additional file 2 Table S1). Fourteen PCRs were performed using the same reaction components as described previously. The PCR conditions were as follows: initial denaturation at 95 °C for 5 min; 30 cycles of 95 °C for 5 min, 55 °C for 1 min, and 68 °C for 2 min; and final extension at 68 °C for 10 min. The PCR amplicons were purified using NucleoSpin Gel and PCR Clean-up (Macherey-Nagel, Germany), according to the manufacturer’s instructions. The purified amplicons were verified using gel electrophoresis and a NanoDrop spectrophotometer (Thermo Fisher, USA) before being sent for sequencing (Macrogen Inc., Republic of Korea). Nucleotide sequences were trimmed and manually edited using electropherograms. The edited sequences of each amplicon were aligned to the IRb and revIRa using Seaview version 5.0.5 , and the nucleotide sequences of both IRb and revIRa were manually corrected.
The GeSeq online tool  was used for annotation of the V. harmandiana chloroplast genome, and the OrganellarGenomeDraw (OGDRAW) tool  was used to draw the circular chloroplast gene map. The complete chloroplast genome of V. harmandianad has been deposited in the NCBI repository, https://www.ncbi.nlm.nih.gov/nuccore/MZ325585.
The complete chloroplast genomes of 24 Rhamnaceae members and two chloroplast genomes of Cannabis sativa cultivar Yoruba Nigeria and Ficus religiosa voucher Ronsted86, were retrieved from the NCBI database (Additional file 2 Table S2). C. sativa and F. religiosa were the outgroup in the phylogenetic analysis. The obtained sequence data, together with the V. harmandiana chloroplast sequence, were revised prior to further analysis. For the revision of published chloroplast genomes, the Muscle program  implemented in the SeaView software version 5.0.5  was used for multiple sequence alignment. Database searches were performed using the BLAST algorithm  within the NCBI database. Protein domain prediction was performed using the hmmscan program  in HMMER webserver version 2.41.2 .
Codon and amino acid usage analysis
The codon usage and amino acid preference of individual chloroplast genomes were calculated based on coding sequences using the CMG biotool . The results are illustrated in radar plots. Principle component analysis (PCA) was performed on the codon usage matrix to compare codon usage across different chloroplast genomes by using R programming language. The results were summarized in a two-dimensional plot of the first two principal components.
Phylogenetic analysis of orthologs
Seventy-eight orthologous proteins (Additional file 2 Table S4) were identified from 25 Rhamnaceae members and the outgroup, and were used in phylogenetic reconstruction. Amino acid sequence multiple alignments of individual orthologs were performed using the Muscle software version 5.1 . The aligned sequences were then trimmed and concatenated using trimAl version 1.2 . Phylogenetic analysis was performed using the randomized axelerated maximum likelihood (RAxML) method under raxmlGUI software environment version 2.0 , the maximum likelihood (ML), and the maximum parsimony (MP) method using MEGA software version 11 . Bootstrapping was performed 500 times to obtain the bootstrap confidence value of the tree branches. For Bayesian inference (BI) method, the best-fit model, JTT + F + I + G4 model, was computed by ModelFinder  in IQ-TREE version 2.2 . BI was performed on MrBayes version 3.2 with two independent Markov chain Monte Carlo (MCMC) runs. Each of four MCMC chains was run for 1000,000 generations and the first 25% of samples from the beginning of the chain were discarded as burn-in. All reconstructed trees were visualized with FIGTREE version 1.4.4 (http://tree.bio.ed.ac.uk/software/figtree/).
Comparative analysis of chloroplast genome features
Repeat structure analysis was performed to identify both simple sequence repeats (SSRs) and long repeats. The SSRs or microsatellites with motif sizes of one to six nucleotides were examined by MicroSAtellite (MISA) . The minimum number of repeats was defined as 10 for mononucleotides, five for dinucleotides, four for tri-nucleotides and three for tetra-, penta-, and hexa-nucleotides. The long repeat sequences were detected by REPuter program . The minimum repeat size was 30 bp, the maximum computed repeats was 90 bp and Hamming distance equal was set to three. The match directions for the long repeats include forward or direct, reverse, palindromic and complement matches.
RNA editing sites of protein-coding genes were predicted using the online Plant RNA Editing Prediction and Analysis Computer (PREPACT 3.0) [84, 85]. The prediction was performed on the BLASTX analysis mode using Cucumis sativus NC_007144 as a reference sequence.
Protein-coding sequences of individual orthologs were aligned by the online MUSCLE software (https://www.ebi.ac.uk/Tools/msa/muscle/)  prior to calculation of the synonymous (Ks) and non-synonymous (Ka) substitution rates and nucleotide diversity with DnaSP version 6.12.03 . The average Ka/Ks ratio of each gene was calculated to obtain the selection patterns of Rhamnaceae. Besides, the Ka/Ks values in V. harmandiana compared with those in the other Rhamnaceae were observed.
Availability of data and materials
The complete chloroplast genome of V. harmandianad has been deposited in the NCBI repository, https://www.ncbi.nlm.nih.gov/nuccore/MZ325585. The original contributions presented in the study can be found in the article and additional files, and further inquiries can be directed to the corresponding authors.
Palmer JD, Jansen RK, Michaels HJ, Chase MW, Manhart JR. Chloroplast DNA variation and plant phylogeny. Ann Missouri Bot Garden. 1988;75:1180–206.
Cronn R, Liston A, Parks M, Gernandt DS, Shen R, Mockler T. Multiplex sequencing of plant chloroplast genomes using Solexa sequencing-by-synthesis technology. Nucleic Acids Res. 2008;36(19):e122.
Liu Q, Li X, Li M, Xu W, Schwarzacher T, Heslop-Harrison JS. Comparative chloroplast genome analyses of Avena: insights into evolutionary dynamics and phylogeny. BMC Plant Biol. 2020;20(1):406.
Lloyd Evans D, Joshi SV, Wang J. Whole chloroplast genome and gene locus phylogenies reveal the taxonomic placement and relationship of Tripidium (Panicoideae: Andropogoneae) to sugarcane. BMC Evol Biol. 2019;19(1):33.
Li DM, Zhao CY, Liu XF. Complete chloroplast genome sequences of Kaempferia Galanga and Kaempferia Elegans: molecular structures and comparative analysis. Molecules. 2019;24(3):474.
Huo Y, Gao L, Liu B, Yang Y, Kong S, Sun Y, et al. Complete chloroplast genome sequences of four Allium species: comparative and phylogenetic analyses. Sci Rep. 2019;9(1):12250.
Wang W, Schalamun M, Morales-Suarez A, Kainer D, Schwessinger B, Lanfear R. Assembly of chloroplast genomes with long- and short-read data: a comparison of approaches using Eucalyptus pauciflora as a test case. BMC Genomics. 2018;19(1):977.
Giordano F, Aigrain L, Quail MA, Coupland P, Bonfield JK, Davies RM, et al. De novo yeast genome assemblies from MinION, PacBio and MiSeq platforms. Sci Rep. 2017;7(1):3935.
Jenjaroenpun P, Wongsurawat T, Pereira R, Patumcharoenpol P, Ussery DW, Nielsen J, et al. Complete genomic and transcriptional landscape analysis using third-generation sequencing: a case study of Saccharomyces cerevisiae CEN.PK113-7D. Nucleic Acids Res. 2018;46(7):e38.
Wyman SK, Jansen RK, Boore JL. Automatic annotation of organellar genomes with DOGMA. Bioinformatics. 2004;20:3252.
Liu C, Shi L, Zhu Y, Chen H, Zhang J, Lin X, et al. CpGAVAS, an integrated web server for the annotation, visualization, analysis, and GenBank submission of completely sequenced chloroplast genome sequences. BMC Genomics. 2012;13:715.
Tillich M, Lehwark P, Pellizzer T, Ulbricht-Jones ES, Fischer A, Bock R, et al. GeSeq - versatile and accurate annotation of organelle genomes. Nucleic Acids Res. 2017;45(W1):W6–W11.
Benson DA, Cavanaugh M, Clark K, Karsch-Mizrachi I, Lipman DJ, Ostell J, et al. GenBank. Nucleic Acids Res. 2013;41:D36–42.
Tonti-Filippini J, Nevill PG, Dixon K, Small I. What can we do with 1000 plastid genomes? Plant J. 2017;90(4):808–18.
Richardson JE, Fay MF, Cronk QC, Bowman D, Chase MW. A phylogenetic analysis of Rhamnaceae using rbcL and trnL-F plastid DNA sequences. Am J Bot. 2000;87(9):1309–24.
Richardson JE, Chatrou LW, Mols JB, Erkens RH, Pirie MD. Historical biogeography of two cosmopolitan families of flowering plants: Annonaceae and Rhamnaceae. Philos Trans R Soc Lond Ser B Biol Sci. 2004;359(1450):1495–508.
Christenhusz MJM, Byng JW. The number of known plants species in the world and its annual increase. Phytotaxa. 2016;261(3):20.
Medan D, Schirarend C. Rhamnaceae. In: Kubitzki K, editor. Flowering plants · Dicotyledons: Celastrales, Oxalidales, Rosales, Cornales, Ericales. Berlin, Heidelberg: Springer; 2004. p. 320–38.
Li M, Ye X, Bi H. Characterization of the complete chloroplast genome of two Hovenia species (Rhamnaceae). Mitochondrial DNA Part B. 2020;5(2):1731–2.
Zhang L, Mao R, Bi H, Shen J, Wang Y, Li M. Characterization of the complete chloroplast genome of Hovenia acerba (Rhamnaceae). Mitochondrial DNA B Resour. 2020;5(1):934–5.
Meng X, Tang GY, Zhao CN, Liu Q, Xu XY, Cao SY. Hepatoprotective effects of Hovenia dulcis seeds against alcoholic liver injury and related mechanisms investigated via network pharmacology. World J Gastroenterol. 2020;26(24):3432–46.
Lin LC, Chou CJ, Kuo YC. Cytotoxic principles from Ventilago leiocarpa. J Nat Prod. 2001;64(5):674–6.
Panthong K, Hongthong S, Kuhakarn C, Piyachaturawat P, Suksen K, Panthong A, et al. Pyranonaphthoquinone and anthraquinone derivatives from Ventilago harmandiana and their potent anti-inflammatory activity. Phytochemistry. 2020;169:112182.
Huang J, Chen R, Li X. Comparative analysis of the complete chloroplast genome of four known Ziziphus species. Genes (Basel). 2017;8(12):340.
Kang KB, Ernst M, van der Hooft JJJ, da Silva RR, Park J, Medema MH, et al. Comprehensive mass spectrometry-guided phenotyping of plant specialized metabolites reveals metabolic diversity in the cosmopolitan plant family Rhamnaceae. Plant J. 2019;98(6):1134–44.
Wang J, Yang S. The complete chloroplast genome of Rhamnus crenata Siebold & Zuccarini (Rhamnaceae). Mitochondrial DNA Part B, Resources. 2021;6(9):2489–90.
Lu X, Luo Q, Qin Y, Yan Q, Guo S. The complete chloroplast genome sequence of Ventilago leiocarpa Benth. Mitochondrial DNA Part B. 2021;6(3):736–7.
Cahen D, Utteridge TMA. Three new species of Ventilago (Rhamnaceae) from South-East Asia. Phytotaxa. 2017;307(3):2017.
Limjiasahapong S, Kaewnarin K, Jariyasopit N, Hongthong S, Nuntasaen N, Robinson JL, et al. UPLC-ESI-MRM/MS for absolute quantification and MS/MS structural elucidation of six specialized Pyranonaphthoquinone metabolites from Ventilago harmandiana. Front Plant Science. 2021;11(2038):602993.
Azizah M, Pripdeevech P, Thongkongkaew T, Mahidol C, Ruchirawat S, Kittakoop P. UHPLC-ESI-QTOF-MS/MS-based molecular networking guided isolation and Dereplication of antibacterial and antifungal constituents of Ventilago denticulata. Antibiotics (Basel). 2020;9(9):606.
Lin C-C, Lin W-C, Chang C-H, Namba T. Antiinflammatory and hepatoprotective effects of Ventilago leiocarpa. Phytother Res. 1995;9(1):11–5.
Panthong A, Kanjanapothi D, Taesotikul T, Phankummoon A, Panthong K, Reutrakul V. Anti-inflammatory activity of methanolic extracts from Ventilago harmandiana Pierre. J Ethnopharmacol. 2004;91(2–3):237–42.
Schrimpe-Rutledge AC, Jones MB, Chauhan S, Purvine SO, Sanford JA, Monroe ME, et al. Comparative omics-driven genome annotation refinement: application across Yersiniae. PLoS One. 2012;7(3):e33903.
Ma Q, Li S, Bi C, Hao Z, Sun C, Ye N. Complete chloroplast genome sequence of a major economic species, Ziziphus jujuba (Rhamnaceae). Curr Genet. 2017;63(1):117–29.
Schmitz-Linneweber C, Maier RM, Alcaraz JP, Cottet A, Herrmann RG, Mache R. The plastid chromosome of spinach (Spinacia oleracea): complete nucleotide sequence and gene organization. Plant Mol Biol. 2001;45(3):307–15.
Millen RS, Olmstead RG, Adams KL, Palmer JD, Lao NT, Heggie L, et al. Many parallel losses of infA from chloroplast DNA during angiosperm evolution with multiple independent transfers to the nucleus. Plant Cell. 2001;13(3):645–58.
Shi C, Liu Y, Huang H, Xia E-H, Zhang H-B, Gao L-Z. Contradiction between plastid gene transcription and function due to complex posttranscriptional splicing: an exemplary study of ycf15 function and evolution in angiosperms. PLoS One. 2013;8(3):e59620.
van den Berg RA, Hoefsloot HC, Westerhuis JA, Smilde AK, van der Werf MJ. Centering, scaling, and transformations: improving the biological information content of metabolomics data. BMC Genomics. 2006;7:142.
Hauenschild F, Matuszak S, Muellner-Riehl AN, Favre A. Phylogenetic relationships within the cosmopolitan buckthorn family (Rhamnaceae) support the resurrection of Sarcomphalus and the description of Pseudoziziphus gen. Nov. TAXON. 2016;65(1):47–64.
Richardson J, Fay M, Cronk Q, Chase M. A revision of the tribal classification of Rhamnaceae. Kew Bull. 2000;55:311.
Kimura M. The neutral theory of molecular evolution and the world view of the neutralists. Genome. 1989;31(1):24–31.
Kang H-I, Lee HO, Lee IH, Kim IS, Lee S-W, Yang TJ, et al. Complete chloroplast genome of Pinus densiflora Siebold & Zucc. And comparative analysis with five pine trees. Forests. 2019; 10(7);600.
Hunt M, Silva ND, Otto TD, Parkhill J, Keane JA, Harris SR. Circlator: automated circularization of genome assemblies using long sequencing reads. Genome Biol. 2015;16(1):294.
Wick RR, Judd LM, Holt KE. Performance of neural network basecalling tools for Oxford Nanopore sequencing. Genome Biol. 2019;20(1):129.
Scheunert A, Dorfner M, Lingl T, Oberprieler C. Can we use it? On the utility of de novo and reference-based assembly of Nanopore data for plant plastome sequencing. PLoS One. 2020;15(3):e0226234.
Laehnemann D, Borkhardt A, McHardy AC. Denoising DNA deep sequencing data-high-throughput sequencing errors and their correction. Brief Bioinform. 2016;17(1):154–79.
Gruenstaeudl M, Gerschler N, Borsch T. Bioinformatic workflows for generating complete plastid genome sequences-an example from Cabomba (Cabombaceae) in the context of the Phylogenomic analysis of the water-lily clade. Life (Basel). 2018;8(3):25.
Neubig KM, Whitten WM, Carlsward BS, Blanco MA, Endara L, Williams NH, et al. Phylogenetic utility of ycf1 in orchids: a plastid gene more variable than matK. Plant Syst Evol. 2009;277(1):75–84.
Dong W, Xu C, Li C, Sun J, Zuo Y, Shi S, et al. ycf1, the most promising plastid DNA barcode of land plants. Sci Rep. 2015;5(1):8348.
Wang W, Lanfear R. Long-reads reveal that the chloroplast genome exists in two distinct versions in Most plants. Genome Biol and Evol. 2019;11(12):3372–81.
Bolmgren K, Oxelman B, Generic limits in Rhamnus L. s.l. (Rhamnaceae) inferred from nuclear and chloroplast DNA sequence phylogenies. TAXON. 2004;53(2):383–90.
Hauenschild F, Favre A, Salazar GA, Muellner-Riehl AN. Analysis of the cosmopolitan buckthorn genera Frangula and Rhamnus s.l. supports the description of a new genus, Ventia. TAXON. 2016;65(1):65–78.
Williams AV, Miller JT, Small I, Nevill PG, Boykin LM. Integration of complete chloroplast genome sequences with small amplicon datasets improves phylogenetic resolution in Acacia. Mol Phylogenet Evol. 2016;96:1–8.
Xie Y, Wang Z, Jiang X, Zhang X. The complete chloroplast genome of Rhamnus globosa (Rhamnaceae). Mitochondrial DNA B Resour. 2020;5(3):2830–1.
Zhang Y, Hu G, Mao W, Dong N, Chen B, Pan Q. Chloroplast genome sequence of the wild Ziziphus jujuba Mill. var. spinosa from North China. Mitochondrial DNA B Resour. 2021;6(2):666–7.
Zong D, Gan P, Zhou A, Li J, Xie Z, Duan A, et al. Comparative analysis of the complete chloroplast genomes of seven Populus species: insights into alternative female parents of Populus tomentosa. PLoS One. 2019;14(6):e0218455.
Rogalski M, do Nascimento Vieira L, Fraga HP, Guerra MP. Plastid genomics in horticultural species: importance and applications for plant population genetics, evolution, and biotechnology. Front. Plant Sci. 2015;6:586.
Dong W, Liu H, Xu C, Zuo Y, Chen Z, Zhou S. A chloroplast genomic strategy for designing taxon specific DNA mini-barcodes: a case study on ginsengs. BMC Genet. 2014;15:138.
Kuang DY, Wu H, Wang YL, Gao LM, Zhang SZ, Lu L. Complete chloroplast genome sequence of Magnolia kwangsiensis (Magnoliaceae): implication for DNA barcoding and population genetics. Genome. 2011;54(8):663–73.
Mower JP. The PREP suite: predictive RNA editors for plant mitochondrial genes, chloroplast genes and user-defined alignments. Nucleic Acids Res. 2009;37:W253.
Tang D, Wei F, Kashif MH, Munsif F, Zhou R. Identification and analysis of RNA editing sites in chloroplast transcripts of kenaf (Hibiscus cannabinus L.). 3 Biotech. 2019;9(10):361.
Javaid N, Ramzan M, Khan IA, Alahmadi TA, Datta R, Fahad S, et al. The chloroplast genome of Farsetia hamiltonii Royle, phylogenetic analysis, and comparative study with other members of clade C of Brassicaceae. BMC Plant Biol. 2022;22(1):384.
Erixon P, Oxelman B. Whole-gene positive selection, elevated synonymous substitution rates, duplication, and indel evolution of the chloroplast clpP1 gene. PLoS One. 2008;3(1):e1386.
De Coster W, D'Hert S, Schultz DT, Cruts M, Van Broeckhoven C. NanoPack: visualizing and processing long-read sequencing data. Bioinformatics. 2018;34(15):2666–9.
Li H. Minimap2: pairwise alignment for nucleotide sequences. Bioinformatics. 2018;34(18):3094–100.
Wick RR, Judd LM, Gorrie CL, Holt KE. Unicycler: resolving bacterial genome assemblies from short and long sequencing reads. PLoS Comput Biol. 2017;13(6):e1005595.
Walker BJ, Abeel T, Shea T, Priest M, Abouelliel A, Sakthikumar S, et al. Pilon: an integrated tool for comprehensive microbial variant detection and genome assembly improvement. PLoS One. 2014;9(11):e112963.
Medlin L, Elwood HJ, Stickel S, Sogin ML. The characterization of enzymatically amplified eukaryotic 16S-like rRNA-coding regions. Gene. 1988;71(2):491–9.
Gouy M, Guindon S, Gascuel O. SeaView version 4: a multiplatform graphical user interface for sequence alignment and phylogenetic tree building. Mol Biol Evol. 2010;27(2):221–4.
Greiner S, Lehwark P, Bock R. OrganellarGenomeDRAW (OGDRAW) version 1.3.1: expanded toolkit for the graphical visualization of organellar genomes. Nucleic Acids Res. 2019;47(W1):W59–64.
Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32(5):1792–7.
Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215(3):403–10.
Finn RD, Clements J, Eddy SR. HMMER web server: interactive sequence similarity searching. Nucleic Acids Res. 2011;39:W29–37.
Potter SC, Luciani A, Eddy SR, Park Y, Lopez R, Finn RD. HMMER web server: 2018 update. Nucleic Acids Res. 2018;46(W1):W200–W4.
Vesth T, Lagesen K, Acar O, Ussery D. CMG-biotools, a free workbench for basic comparative microbial genomics. PLoS One. 2013;8(4):e60120.
Edgar RC. MUSCLE v5 enables improved estimates of phylogenetic tree confidence by ensemble bootstrapping. BioRxiv. 2021;2021:449169.
Capella-Gutierrez S, Silla-Martinez JM, Gabaldon T. trimAl: a tool for automated alignment trimming in large-scale phylogenetic analyses. Bioinformatics. 2009;25(15):1972–3.
Edler D, Klein J, Antonelli A, Silvestro D. raxmlGUI 2.0: a graphical interface and toolkit for phylogenetic analyses using RAxML. Methods Ecol Evol. 2021;12(2):373–7.
Tamura K, Stecher G, Kumar S. MEGA11: molecular evolutionary genetics analysis version 11. Mol Biol Evol. 2021;38(7):3022–7.
Kalyaanamoorthy S, Minh BQ, Wong TKF, von Haeseler A, Jermiin LS. ModelFinder: fast model selection for accurate phylogenetic estimates. Nat Methods. 2017;14(6):587–9.
Minh BQ, Schmidt HA, Chernomor O, Schrempf D, Woodhams MD, von Haeseler A, et al. IQ-TREE 2: new models and efficient methods for phylogenetic inference in the genomic era. Mol Biol Evol. 2020;37(5):1530–4.
Beier S, Thiel T, Munch T, Scholz U, Mascher M. MISA-web: a web server for microsatellite prediction. Bioinformatics. 2017;33(16):2583–5.
Kurtz S, Choudhuri JV, Ohlebusch E, Schleiermacher C, Stoye J, Giegerich R. REPuter: the manifold applications of repeat analysis on a genomic scale. Nucleic Acids Res. 2001;29(22):4633–42.
Lenz H, Rudinger M, Volkmar U, Fischer S, Herres S, Grewe F, et al. Introducing the plant RNA editing prediction and analysis computer tool PREPACT and an update on RNA editing site nomenclature. Curr Genet. 2010;56(2):189–201.
Lenz H, Hein A, Knoop V. Plant organelle RNA editing and its specificity factors: enhancements of analyses and new database features in PREPACT 3.0. BMC Bioinformatics. 2018;19(1):255.
Madeira F, Pearce M, Tivey ARN, Basutkar P, Lee J, Edbali O, et al. Search and sequence analysis tools services from EMBL-EBI in 2022. Nucleic Acids Res. 2022;50(W1):W276–9.
Rozas J, Ferrer-Mata A, Sanchez-DelBarrio JC, Guirao-Rico S, Librado P, Ramos-Onsins SE, et al. DnaSP 6: DNA sequence polymorphism analysis of large data sets. Mol Biol Evol. 2017;34(12):3299–302.
We thank Dr. Visanu Wanchai for technical assistance with codon usage calculations.
This study was also supported by Mahidol University, Grant No. (IO) R016420001 (to SK). This study received funding from the NSRF via the Program Management Unit for Human Resources & Institutional Development, Research, and Innovation [grant number B16F640099]. We acknowledge the support from the Center of Excellence for Innovation in Chemistry (PERCH-CIC), Ministry of Higher Education, Science, Research, and Innovation, Thailand. This work supported by the National Institute of General Medical Sciences of the National Institutes of Health (P20GM125503 to IN).
Ethics approval and consent to participate
Sample collection of V. harmandiana was permitted by the private land owner in Trang province, Thailand, Mr. Wanlop Pengphan. The collection of the V. harmandiana covering various plant parts for research and related purposes was done with the permission and supervision of the local authority. The collected samples were identified by the author, Dr. Narong Nuntasaen from Department of National Parks, Wildlife and Plant Conservation, Ministry of Natural Resources and Environment. All samples with the voucher specimen accession code, BKF no. 35203, were deposited at the Forest Herbarium, Department of National Parks, Wildlife and Plant Conservation in Bangkok, Thailand. Experimental research and field studies on plants (either cultivated or wild), including the collection of plant material, must comply with relevant institutional, national, and international guidelines and legislation.
Consent for publication
The authors declare that there is no conflict of interest.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Additional file 1: Figure S1.
The number of spanning reads over the IR boundaries. (A) Boundary A locates between LSC and IRb. (B) Boundary B locates between IRb and SSC. (C) Boundary C locates between SSC and IRa. (D) Boundary D locates between IRa and LSC. The number of ONT reads spanning over the four IR boundaries at different distances (nt) from the boundaries are illustrated as bar charts. Large single-copy (LSC); inverted repeats (IRs) and small single-copy (SSC). Figure S2. Comparative gene arrangement in IR regions of Rhamnaceae, C. sativa and F. religios. Each box represents a gene. The rps19 and ycf1 genes (bold and underline) are located at the borders of IR regions. A missing gene that was re-annotated is highlighted in red. A gene in LSC is represented by an orange box. A gene in IR is in a blue box and a gene in both LSC and IR regions is in a white box. The C. sativa NC_027223 and F. religiosa NC_033979 are the outgroup of phylogenetic analysis. Reversed inverted repeat (revIR). Figure S3. Domain analysis of Ycf1 protein sequences. The full-length colored bar represents the presence of an entire Ycf1 domain. A shorter colored bar within the grey bar indicates the matching part of the domain. A truncated domain is shown by a jagged edge. The number indicates the amino acid length. Ycf1 copy in IRb (ycf1_IRb) and ycf1 gene in IRa (ycf1_IRa). Figure S4. A shift in the origin of H. acerba MN794429 chloroplast genome and correction. Suggested origin is presented in red color. Figure S5. Multiple alignment of the ycf15 gene sequences and matching domain fragments. This figure shows the alignment of the deposited ycf15 DNA sequences from six Rhamnaceae organisms and the ycf15 sequence of V. harmandiana. The predicted Ycf15 domain of each ycf15 is illustrated on the right column. A missing T-base from the ycf15 sequence of V. harmandiana is pointed out by an arrow. The full-length colored bar represents the presence of an entire Ycf15 domain. A truncated omain is shown by a jagged edge. The number indicates the amino acid length. Only the ycf15 copy in IRb is shown, as its copy in IRa is identical. Figure S6. Re-annotation of the ycf15 gene in Barbeya oleoides NC_040984 and the outgroup. The alignment of the ycf15 gene sequences of Barbeya oleoides, C. sativa and F. religiosa to the ycf15 gene sequence of N. tabacum Z00044 is illustrated. The TA-gap is pointed out by a black arrow. The predicted Ycf15 domain of each ycf15 is illustrated on the right column. The full-length colored bar represents the presence of an entire Ycf15 domain. A truncated domain is shown by a jagged edge. The number indicates the amino acid length. Only the ycf15 copy in IRb is shown, as its copy in IRa is identical. Figure S7. Re-annotation of the ycf15 gene in Rhamnaceae. (A) The alignment of the reference gene sequence to the first exon and (B) to the second exon of the ycf15 gene in Rhamnaceae organisms. The figure shows the multiple sequence alignment using N. tabacum Z00044 as a reference to re-annotate the ycf15 gene of the organisms in this study. TA-gaps in the ycf15 sequences of the Rhamnaceae are pointed out by a black arrow. The predicted Ycf15 domain of each ycf15 is illustrated on the right column. The full-length colored bar represents the presence of an entire Ycf15 domain. A truncated domain is shown by a jagged edge. The number indicates the amino acid length. Only the ycf15 copy in IRb is shown, as its copy in IRa is identical Figure S8. Re-annotation of infA gene in V. leiocarpa. (A) The alignment of infA DNA sequences between V. harmandiana and V. leiocarpa. A-gap is pointed out by an arrow. (B) Comparing amino acid sequences of the infA between V. harmandiana and V. leiocarpa. A dashed line (−) indicates a stop codon. Figure S9. Comparisons of the atpF and clpP gene structures. (A) Comparing the atpF gene structure of Z. jujuba species. (B) Comparing the clpP gene structure of H. acerba species. A blue box represents a coding region and the red wavy line represents an intergenic region. The base position of the atpF in Z. jujuba NC_030299 and the clpP in H. acerba MN794429 is used as a reference for each gene. Figure S10. Phylogenetic trees of Rhamnaceae reconstructed from the orthologous proteins (A) using ML method, (B) using MP method, (C) using BI method and (D) the tree reconstructed from the orthologous genes using RAxML method. Different colors correspond to tribes labelled in square brackets. The outgroup branch is not colored. Two major groups of Rhamnaceae: ziziphoid and rhamnoid are presented on the rightmost text. A number in each tree indicates the ML bootstrap value, the MP bootstrap value, the posterior probability of BI, the ML bootstrap value, respectively. Figure S11. Characteristics and comparisons of Rhamnaceae chloroplast genome features. (A) Comparison of the SSR types. (B) Distribution of SSRs in LSC, SSC and IR regions. (C) Comparison of the long repeat types. (D) Distribution of long repeats in LSC, SSC and IR regions. The total number of SSRs and long repeat sequences in each species is in the parenthesis. Figure S12. The original image of gel in Fig. 1C before cropping and inverting color.
Additional file 2: Table S1.
List of primers. Table S2. List of 25 Rhamnaceae complete chloroplast genomes and the outgroup for the phylogenetic analysis. Table S3. List of re-annotated genes. Table S4. List of orthologous genes for phylogenetic reconstruction.
Additional file 3: Table S5.
Codon usage of 86 protein-coding genes of each chloroplast genome.
Additional file 4: Table S6.
SSRs of 25 Rhamnaceae chloroplast genomes.
Additional file 5: Table S7.
Changes of amino acids from RNA editing
Additional file 6: Table S8.
The Ka/Ks ratio values and nucleotide diversity of protein-coding genes of the Rhamnaceae
Additional file 7: Table S9.
The Ka/Ks ratio comparisons with V. harmandiana
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.
About this article
Cite this article
Wanichthanarak, K., Nookaew, I., Pasookhush, P. et al. Revisiting chloroplast genomic landscape and annotation towards comparative chloroplast genomes of Rhamnaceae. BMC Plant Biol 23, 59 (2023). https://doi.org/10.1186/s12870-023-04074-5
- Ventilago harmandiana
- Chloroplast genome
- Plant genomics
- Natural product
- Genome assembly
- Genome annotation
- Oxford Nanopore technologies