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Enigmatic Diphyllatea eukaryotes: culturing and targeted PacBio RS amplicon sequencing reveals a higher order taxonomic diversity and global distribution

  • The Correction to this article has been published in BMC Evolutionary Biology 2018 18:118



The class Diphyllatea belongs to a group of enigmatic unicellular eukaryotes that play a key role in reconstructing the morphological innovation and diversification of early eukaryotic evolution. Despite its evolutionary significance, very little is known about the phylogeny and species diversity of Diphyllatea. Only three species have described morphology, being taxonomically divided by flagella number, two or four, and cell size. Currently, one 18S rRNA Diphyllatea sequence is available, with environmental sequencing surveys reporting only a single partial sequence from a Diphyllatea-like organism. Accordingly, geographical distribution of Diphyllatea based on molecular data is limited, despite morphological data suggesting the class has a global distribution. We here present a first attempt to understand species distribution, diversity and higher order structure of Diphyllatea.


We cultured 11 new strains, characterised these morphologically and amplified their rRNA for a combined 18S–28S rRNA phylogeny. We sampled environmental DNA from multiple sites and designed new Diphyllatea-specific PCR primers for long-read PacBio RSII technology. Near full-length 18S rRNA sequences from environmental DNA, in addition to supplementary Diphyllatea sequence data mined from public databases, resolved the phylogeny into three deeply branching and distinct clades (Diphy I – III). Of these, the Diphy III clade is entirely novel, and in congruence with Diphy II, composed of species morphologically consistent with the earlier described Collodictyon triciliatum. The phylogenetic split between the Diphy I and Diphy II + III clades corresponds with a morphological division of Diphyllatea into bi- and quadriflagellate cell forms.


This altered flagella composition must have occurred early in the diversification of Diphyllatea and may represent one of the earliest known morphological transitions among eukaryotes. Further, the substantial increase in molecular data presented here confirms Diphyllatea has a global distribution, seemingly restricted to freshwater habitats. Altogether, the results reveal the advantage of combining a group-specific PCR approach and long-read high-throughput amplicon sequencing in surveying enigmatic eukaryote lineages. Lastly, our study shows the capacity of PacBio RS when targeting a protist class for increasing phylogenetic resolution.


Diphyllatea is a protist group that holds a deep and distinct position in the eukaryote tree; dependent on the position of the root, it may represent one of the earliest diverging eukaryotic lineages [1,2,3,4,5]. Currently, only a few species are described using traditional microscopic methods. Initially, the class Diphyllatea and the order Diphylleida were proposed to encompass the biflagellate Diphylleia rotans and the quadriflagellate Collodictyon triciliatum [6]. However, revisions of the systematic classification changed this class to include the species Sulcomonas lacustris and several older synonyms (e.g. C. sparseovacuolatum for C. triciliatum and Aulacomonas submarina for D. rotans) [7, 8]. Currently, based on morphological features, with only 18S rRNA provided from D. rotans, Diphyllatea is proposed to consist of the three genera Collodictyon, Diphylleia (not to be confused with the homonym in Botanical nomenclature) and Sulcomonas [9, 10], with the first two constituting the order Diphylleida and the third family Sulcomonadidae. The three-representative species (C. triciliatum, D. rotans and S. lacustris) have been previously investigated by light and electron microscopy [8, 11,12,13,14,15,16]. They share a heart- or egg-shape form and possess a ventral groove [12, 14, 17], more or less dividing the body longitudinally. The size range of the identified species is variable (15–60 μm length for Collodictyon, 20–25 μm length for Diphylleia and 8–20 μm length for Sulcomonas).

As the description of species diversity and the erection of the whole taxonomic unit of Diphyllatea were based on microscopic observations, one could expect that sequencing surveys of environmental DNA would detect a larger number of cryptic species. On the contrary, excluding the original D. rotans 18S rRNA (AF420478) from Brugerolle et al. 2002, only a single partial 18S rRNA sequence of Diphyllatea has been reported from a Tibetan freshwater lake (AM709512), and until now, no Diphyllatea have been classified from other water samples [18]. It is known that environmental PCR using group-specific primers can effectively amplify the diversity of some unicellular eukaryotes [19,20,21], but such an approach has never before been applied to Diphyllatea. Hence, its diversity may currently be underestimated. Accordingly, the know geographical distribution of the class, based on molecular data, is currently limited to China, France and Norway, with less geographic resolution at lower taxonomical levels [1, 8, 18]. Though, morphological data seemingly suggests a possible global distribution of C. triciliatum [11, 14, 22,23,24].

Thus, the objective of this study is to investigate possible cryptic diversity and distribution of Diphyllatea by firstly studying the morphology of novel cultured strains, and secondly by the amplification and phylogenetic inference of Diphyllatea rRNA from marine and freshwater samples. Additional database mining will allow for the confirmation of the classes diversity and distribution.

To achieve a robustly resolved phylogeny that will allow us to infer the relationships within Diphyllatea, long rRNA sequence reads are essential. For this reason, we targeted Diphyllatea environmental DNA and sequence near full-length 18S rRNA gene amplicons with PacBio RSII technology.

Recently, eukaryotic diversity studies have used Illumina (predominantly MiSeq) technology for sequencing rRNA amplicons. As Illumina has a restricted read length, diversity studies have been limited to an amplicon maximum of approximately 450 bp. A result of this being that studies have either focused on short hypervariable regions of 18S rRNA [25,26,27], ITS [28, 29], or 28s rRNA [30, 31]. These regions, despite being variable, sometimes lack enough sequence variation to be able to divide some genera to the species level. Further, focusing on separate, non-overlapping rRNA regions makes it difficult to study amplicons in a comparative phylogenetic context. Conversely, the study of long amplicons has traditionally involved cloning and Sanger sequencing [32,33,34], a time-consuming and costly method when high depth is desired. The Pacific Bioscience (PacBio) RS sequencing platform offers an alternative to short Illumina reads by providing long (> 20 kb) sequencing reads. PacBio RS also represents an alternative to cloning and Sanger sequencing for longer rRNA amplicons. To date, PacBio RS has mainly been applied to genome and more recently transcriptome sequencing [35,36,37,38]. However, a few studies have shown the platforms viability for studying 16s rRNA diversity of prokaryotes [39, 40], and more recently eukaryotic rRNA amplicons [41, 42]. Though at present, no studies have applied PacBio to sequence targeted 18S rRNA amplicons of lengths > 1000 bp.


Culture isolation and maintenance

Asian strains of Diphyllatea were established by a single-cell isolation method from localities in Japan, Thailand and Vietnam (Table 1). The isolated strains from Asia were inoculated into the freshwater medium URO [43] with endogenous cyanobacteria (Microcystis, strain no. NIES-44) as food and established as cultures. The investigated Norwegian strain of Collodictyon triciliatum (i.e. strain Å85) was a clonal isolate (from a single-cell) from Lake Årungen initially cultured on WC-medium [44] with the cryptomonad Plagioselmis nannoplanktica or a strain of the green alga Chlorella as food [14]. Subsequently, all cultures were kept in BG11 ½ medium [45], with Microcystis strain CYA-43 provided by the Norwegian Institute of Water Research (NIVA– All cultures were grown using the following conditions: 17 °C, 250 μMol m− 1 s− 1 of daylight-type fluorescent light at a 14/10 (L/D) cycle.

Table 1 Sampling locations for cultured Diphyllatea-like organisms and environmental DNA


Light microscopy of the 11 Diphyllatea was conducted using a Nikon Diaphot inverted microscope. Differential interference contrast (DIC) micrographs and video of Diphyllatea cells were taken using a Nikon D- series digital camera (D1 and D300S) connected to a screen. Electron microscopy (EM) was done by the negative staining of whole cells, after drop fixation on grids by osmium vapour [14].

DNA isolation, PCR and sequencing

DNA was isolated from 50 ml of each culture by pelleting cells by centrifugation at 500 x g and 4 °C for 5 minutes, followed by standard CTAB chloroform/isoamylalcohol extraction and subsequent ethanol precipitation [46]. A ~6.3 kb region of the rRNA operon, covering the 18S, ITS1, 5.8S, ITS2 and 28S regions, was amplified as one continuous fragment with the forward primer NSF83 and the reverse primer LR11 (Table 2) utilizing Phusion High-Fidelity DNA polymerase, 35 cycles and a 50 °C annealing (ThermoFisher). The single ~6.3 kb PCR products were cleaned using Chargeswitch PCR Clean-up kit (ThermoFisher) and then Sanger sequenced (GATC Biotech, Germany) as separate fragments, utilizing primers outlined in Additional file 1: Table S2. Additional sequencing primers were designed using Primaclade [47]. The separate fragments were subsequently quality checked and assembled using the Phred/Phrap/Consed package [48] under default settings. Additional manual editing of the 11 contigs was performed in Mesquite v3.1 [49].

Table 2 List of primers used in this study

Primer design and specificity confirmation

For optimal primer design with high specificity to the Diphyllatea clade, all available orthologous Diphyllatea sequences were used for alignment construction; Å85 and KIVT02 rRNA were used as blastn queries to extract Diphyllatea sequences deposited in the NCBInr database using default parameters. Further, Diphylleia rotans NIES-3764 rRNA (isolated in Amakubo, Ibaraki prefecture, Japan), taken from an unconnected genome project, was additionally used as a query and included in subsequent analyses. The resulting sequences were aligned together with the 11 culture sequences using the MAFFT Q-INS-i method [50], considering secondary RNA structure (default parameters used). The alignment was then manually checked and edited using Mesquite v3.1 [49] before designing primers with Primaclade [47]. All potential primers were tested for specificity to the Diphyllatea clade by checking sequence identity against non-Diphyllatea sequences in the Silva rRNA database in addition to an rRNA alignment with a broad sample of eukaryotic taxa [51]. OligoCalc [52] was applied to check self-complementarity and calculate primer Tm. The Diphyllatea-specific primers with highest potential were utilized in PCRs to confirm amplification of Diphyllatea rRNA, with optimal annealing temperature being established, and the non-amplification of DNA template external to Diphyllatea (a DNA mix of 30 cultures held in our lab). Diphyllatea-specific rRNA 18S gene primers designed in this study are listed in Table 2.

Environmental DNA and confirmation of Diphyllatea

Environmental DNA was sampled from Lake Årungen by collecting and filtering two liters of surface water through a Whatman GF/C glass-fiber filter with an effective pore size of 1.2 μm prior to DNA isolation. Dr. David Bass (NHM) kindly provided supporting freshwater DNA samples (Table 1) from Borneo, South Africa, and the UK. Dr. Bente Edvardsen (UoO) in collaboration with BioMarKs [53], kindly provided marine DNA samples (Table 1) from Bulgaria, France, Italy, and Norway. Eukaryotic DNA was confirmed for all samples by PCR with a 55 °C annealing temperature, using the universal 18S rRNA primers NSF83 and 1528R (Table 2). Diphyllatea clade-specific PCR was subsequently performed on all environmental DNA samples targeting the 18S rRNA gene region with the primers Diphy257F and Diphy1881R (~1624 bp: see Table 2) with a 55 °C annealing temperature. Additionally, the annealing temperature for the Diphyllatea clade-specific PCR (Diphy257F - Diphy1881R) was lowered by 5 °C to allow primers to anneal to possible novel Diphyllatea template rRNA with lower sequence identity. Finally, for those environmental templates that gave no PCR product with the above primer pair, a pair with a lower specificity to the Diphyllatea clade was employed; Diphy453F and 1528R (~1697 bp: see Table 2), with a 55 °C annealing, amplifies a range of eukaryotes including Diphyllatea. A positive (Å85 and KIVT02 DNA) and negative control were employed for all PCRs. Positive amplicons were cleaned using Chargeswitch PCR Clean-up kit (ThermoFisher) or the Wizard SV gel and PCR clean-up system (Promega) and used for down-stream processing.

PacBio barcodes, library prep and amplicon sequencing

As a more economical and efficient alternative to cloning, PacBio RS II was employed to achieve higher sequencing depth of the long environmental rRNA amplicons. PCR primers with symmetric (reverse complement) PacBio barcodes (21 bp) were attached to the separate 18S rRNA gene amplicons by PCR: a 2μl 1:10 dilution of template DNA (18S rRNA gene amplicon) was used as input in a two-step PCR protocol using Phusion High-Fidelity DNA polymerase (ThermoFisher), with a 72 °C 90 s annealing and 20 cycles. The resulting PCR product was cleaned before successful attachment of PacBio barcodes was confirmed using Bioanalyzer (Agilent Technologies). A single SMRTcell was prepared and sequenced, multiplexing both the Diphy257F - Diphy1881R (~1624 bp) and the Diphy453F - 1528R (~1697 bp) amplicons (Table 3 and Additional file 1: Table S2). The Norwegian Sequencing Centre (NSC), Oslo, Norway, performed library preparation and sequencing. The Library was prepared using Pacific Biosciences 2 kb library preparation protocol, before sequencing with the PacBio RS II using P4-C2 chemistry. Filtering was performed using Reads of Insert protocol on the SMRT portal (SMRTAnalysis v2.2.0.p1 build 134,282). Default settings (Minimum number of passes = 1 and Minimum Predicted Accuracy = 0.9) were used.

Table 3 PCR and sequencing results for environmental 18S rRNA gene amplicons

Database-mining for marine Diphyllatea

To further investigate any cryptic presence of Diphyllatea in marine environments, publicly available databases were mined. The BioMarKs, Global Ocean Sampling (GOS), Tara oceans marine metagenome, and Tara oceans V9 databases were all queried for presence of Diphyllatea rRNA using the Diphylleia, KIVT02 and Å85 Collodictyon rRNA sequences. Further, the GOS and Tara oceans marine metagenome databases were queried with the 124 Collodictyon gene transcripts previously used to infer the phylogenetic placement of Diphyllatea [1]. It should be noted that the known C. triciliatum transcriptome reported in Zhao et al. 2012, was generated from the same Å85 strain represented in this study [1].

Clustering, alignment construction and phylogenetic analyses

PacBio sequencing reads were split into their respective samples and barcodes removed using the SMRT portal. Reads were subsequently filtered keeping a CCS read accuracy of 1.0 (high quality sequences constituting multiple read passes). CCS Reads lacking either the forward or reverse primer sequence were discarded. Reads were then clustered with a 98% identity threshold, utilizing the “-cluster-otus” command in Usearch v8.1 [54, 55]. The “-cluster-otus” command additionally removed possible chimeric reads from the dataset. Uncultured clones from the same locality, previously categorised as Diphyllatea, acquired from NCBInr, were also clustered at the same identity. Operational taxonomic unit (OTU) clustering was carried out in this study using a 98% clustering identity threshold that is more stringent than the more commonly used 97% threshold. OTU clustering at 97% has recently been shown to be too conservative for estimating diversity in microbial eukaryotes, merging different species in the same cluster [56, 57]. Further, a 97% clustering identity is usually applied to illumina amplicons when targeting variable rRNA regions [58], with a more stringent threshold being traditionally applied to longer read rRNA amplicons encompassing conserved and variable regions [56, 59]. Clusters (OTUs) were then queried with blastn against a private database on CLC main workbench 7 (Qiagen) containing a broad selection of eukaryotic 18S rRNA taxa, including Diphyllatea (Å85, Diphylleia rotans and KIVT02). OTU hits with an E-value of 0.0 to Diphyllatea were subsequently aligned to the previously constructed alignment using MAFFT “—add” with default parameters and manually refined with Mesquite v3.1 [49]. Phylogenetic placement of the OTUs was checked using RAxML (method described below), with only those clustering with the Diphyllatea clade and constituting > 1 read being kept for further analysis. Further, to check if a possible cryptic diversity was disregarded during filtering, the method was repeated on reads with a CCS accuracy < 1.0. After the removal of ambiguously aligned characters, using Gblocks with least stringent parameters [60], the final dataset consisted of 64 taxa and 3983 characters. The alignment (both masked and unmasked) has been made freely available through the authors’ ResearchGate pages (

Maximum likelihood phylogenetic analyses were carried out using the GAMMA-GTR model in RAxML v8.0.26 [61]. The topology with the highest likelihood score of 100 heuristic searches was chosen. Bootstrap values were calculated from 500 pseudo-replicates. Bayesian inferences were performed using MrBayes v3.2.2 [62], applying the GTR + GAMMA+Covarion model. Two independent runs, each with three cold and one heated Markov Chain Monte Carlo (MCMC) chains, were started from a random starting tree. The MCMC chains lasted for 40,000,000 generations with the tree sampled every 1000 generations. The posterior probabilities and mean marginal likelihood values of the sampled trees were calculated after the burn-in phase, which was determined from the marginal likelihood scores of the initially sampled trees. The average split frequencies of the two runs were < 0.01, indicating the convergence of the MCMC chains.

To investigate any possible topological effect of inferring taxa with missing sequence data, a secondary alignment constituting the 18S rRNA was constructed (64 taxa and 1575 characters). This was inferred, as previous, and the topological congruence of the ingroup taxa with that of the larger rRNA dataset was tested using the Icong index ( [63]. Topologies were more congruent than expected by chance (Icong = 2.69 & P-value = 6.93e-12), rejecting any negative effect of inferring taxa with missing sequence data. As such, only the result for the larger rRNA analysis is presented (Fig. 3), with the 18S rRNA tree supplied as Supporting material (Additional file 1: Figure S2).


Cultured Diphyllatea show a Collodictyon morphology

Our survey of the diversity of Diphyllatea generated 10 new strains from Japan, Thailand and Vietnam, which complemented the Norwegian Collodictyon strain already established (Table 1). Light microscope observations of all isolates showed a congruent morphology to Collodictyon by sharing an egg- or heart-like body and four isomorphic flagella (Fig. 1). All cultured strains were compared with the diagnoses of currently recognised species of Diphyllatea and assigned to the morphospecies C. triciliatum [11]. The swimming cells have a slow and relaxed movement, while rotating, driven by flagella (Fig. 1b, d, e, i, j and Additional file 2: Video S1). They have the ability to cling to the surface of the culture dish by a cytoplasmic veil and pseudopodia (i.e. an amoeboid property) within or from the sulcus (Fig. 1c, h and Additional file 3: Video S2). Observations of live cells show the central cytoplasm contains a few large or small vacuoles. Some of the vesicles contain food particles (i.e. Microcystis strain CYA 43) at various stages of digestion (Fig. 1a and g). All studied strains can form a ventral furrow or groove that extends dorsally, dividing the cell into two parts (Fig. 1d and i), but this is a non-permanent structure during the cell cycle. Emergence of a long groove may be exclusive to cells that are starting or initiating cell division. Furthermore, we uncovered thick-walled resting stages or cysts, with two long gelatinous filaments (Fig. 1f), similar to earlier descriptions of Collodictyon resting spores [64]. The resting stage was only observed in the Å85 culture, with more microscopy work needed to reveal if this feature is common among Diphyllatea species.

Fig. 1

DIC Micrographs of newly cultured Diphyllatea-like organisms (Asian strains) and C. triciliatum (strain Å85). a KIVTT01. b KIINB. c KIKNR01. d KIVTT02. e KIKNR02. f Å85. g KIVT04. h Å85. i Å85. j KIVT01; scale bar 10 μm. Diphy II is represented in (h & i), whilst Diphy III is represented in (a-e), (g & j). Swimming cells are represented in (b, d, e, i and j). Amoeboid property represented in (c and h). Cell digestion shown in (a and g). Ventral furrow or groove depicted in (d and i). The resting stage or cyst is shown in (f) and is a phase contrast image

Electron microscopy of the negatively stained Collodictyon cells showed identical and smooth flagella lacking hairs or tomentum (Fig. 2), and that the periplast is hyaline and even. Other sub-cellular ultrastructures were difficult to identify; the cell is highly fragile and easily disrupted in the electron microscopy fixation process [14].

Fig. 2

Electron micrographs of the flagella of C. triciliatum (strain Å85). a Four flagella and the membranes of flagella; b tip of flagellum

Diphyllatea is divided into three higher order groups (Diphy I – III)

The rRNA fragments of ~6.3 kb for all 11 Collodictyon cultures were successfully amplified, sequenced and assembled (Accessions MF039356-MF039367).

With the inclusion of Diphylleia rotans rRNA (MF039365) the Diphyllatea class was divided into three ribotype groupings based on sequence length and indels; the amplified fragment ranged from ~5.8 kb in Diphylleia rotans, here named Diphy I (calculated from genome sequence), ~5.9 kb in Å85 and KIVT03, here named Diphy II, to ~6.3 kb in KIINB, KIKNR01, KIKNR02, KIKNR03, KIVT01, KIVT02, KIVT04, KIVTT01 and KIVTT02, here named Diphy III. As such, the three groups (Diphy I, II and III) had a 69–79% pairwise identity over the amplicon length, and a 73–86% pairwise identity for the 18S rRNA gene.

Diphyllatea diversity in natural samples

To investigate the diversity of the class further we designed new Diphyllatea-specific primer pairs and applied these to environmental DNA samples from various habitats. The presence of 18S rRNA was confirmed in all environmental samples using the universal eukaryote primers NSF83 - 1528R. The Diphyllatea-specific primer pair Diphy257F - Diphy1881R, designed in this study, successfully amplified 18S rRNA from four of eight environmental freshwater samples (Table 3). The primer pair with lower specificity to known Diphyllatea 18S rRNA, Diphy453F – 1528R, successfully amplified template from a further three of the freshwater samples (Table 3).

Sequencing these environmental amplicons on a SMRTcell confirmed Diphy257F - Diphy1881R successfully amplified targeted 18s rRNA from Diphyllatea, whilst Diphy453F – 1528R was unsuccessful in amplifying Diphyllatea template (Table 3). Pacbio CCS reads were filtered and clustered at a 98% identity threshold before being aligned with the Diphy I-III 18s – 28s rRNA fragments previously amplified (see alignment and Fig. 3). The freshwater samples BOR41 and Årungen both showed the presence of Diphy I and II sequences. It should be noted that the Årungen Diphy II PacBio OTU and the clonal Å85 Sanger sequence shared a 100% identity over sequence length. Only Diphy I sequence data was observed in the BOR42 and BOR43 samples, though this is a likely result of limited sequencing depth. None of our new environmental 18S rRNA gene amplicons (MF039351–55) showed similarity to the Diphy III sequence. No additional sequences were obtained that clustered external to the three Diphyllatea groupings already confirmed (Diphy I-III). Only a single Diphyllatea OTU for each clade was recovered from the individual environmental samples using a 98% clustering identity threshold (Fig. 3). A such a more relaxed threshold would not have affected the recovered diversity.

Fig. 3

The rRNA phylogeny of Diphyllatea. The topology was reconstructed with the GAMMA-GTR model in RAxML v8.0.26. and inferred with 64 taxa and 3983 characters. The inference has been collapsed at varying taxonomic levels for easier visualisation, with blue representing the in-group. The numbers on the internal nodes are ML bootstrap values (BP, inferred by RAxML v8.0.26. under then GAMMA-GTR model) and posterior probabilities (PP, inferred by MrBayes v3.2.2 under the GTR + GAMMA+Covarion model), ordered; RAxML/MrBayes. Black circles indicate BP > 90% and PP 1.00, values with BP < 50% are not shown. Asterisk (*) denotes environmental OTUs sequenced in this study, with “N” representing the number of reads included in each OTU. § depicts rRNA from cultured Diphyllatea amplified in this study. The clonal Å85 Sanger sequence and Årungen PacBio OTU are represented as a single taxon as they shared a 100% identity. Abbreviations for countries: CN = China, FR = France, JP = Japan, MY = Malaysia, NL = Netherlands, NO = Norway, TH = Thailand, and VN = Vietnam. See Additional file 1: Figure S2 for 18S rRNA inference of Diphyllatea

The new primers Diphy257F and Diphy1881R therefore provide a promising tool for future investigations of the Diphyllatea diversity. It should be noted, however, that even though Diphyllatea 18S rRNA was successfully amplified, the new primers also amplified a putative protein-coding gene (4-diphospocytidyl-2C-methyl-D-erythritol kinase) from a possible novel brackish Actinobacteria (MF039368) in two samples (BOR41 and BOR43). As these sequences were not 18S rRNA, and obviously of prokaryote origin, they were discarded.

Diphyllatea unconfirmed in marine habitats

To date, Diphyllatea species have only been observed in freshwater environments, including an estuary of a freshwater river [13]. As the new PCR primers successfully amplify Diphyllatea 18S rRNA from environmental samples, we used them to investigation a possible cryptic diversity in marine environments. However, while the marine DNA samples were of good quality and previously used for large surveys of protist diversity [53], we were unable to amplify Diphyllatea 18S rRNA (Table 3) using the Diphy257F - Diphy1881R primer pair. Applying less stringent PCR conditions (i.e. lowering annealing temperature from 55 °C to 50 °C) had no effect on this result. As previous, and in an attempt to amplify novel Diphyllatea template rRNA with lower sequence identity, the primer pair Diphy453F - 1528R was used, successfully amplifying product from three of the four marine DNA samples (Table 3). However, once these environmental amplicons had been sequenced on a SMRTcell, filtered, and clustered, none of the 192 OTUs they represented had an affinity to Diphyllatea (see Table 3 and Additional file 1: Figures S2 and S4).

In our search for marine Diphyllatea sequences, we complemented our PCR and sequencing approach by searching public sequence databases. Despite querying four of the largest sequence databases (BioMarKs, GOS, Tara oceans marine metagenome, and Tara oceans V9) for the presence of Diphyllatea rRNA and two databases (GOS and Tara oceans marine metagenome) with 124 Collodictyon gene transcripts [1], we were unable to identify any marine Diphyllatea-like sequences. Instead, we identified 30 freshwater 18S rRNA sequences in the NCBInr database additional to the known Diphylleia rotans sequence from France (AF420478) and the uncultured Collodictyonidae sequence from Tibet (AM709512): 18 sequences (KC575460–76, KC575502) were from Lake Fuxian SW China, 2 sequences (JF774996, JF775022) from Rhine river water, Netherlands, and 10 sequences (GU970557–59, 61, 62, 64, 66, 69, 72, 73) from sewage water, Netherlands. All showed highest pairwise affinity to Diphy I (Fig. 3).

Phylogeny and diversity of the class Diphyllatea

Using all generated and acquired sequences in phylogenetic reconstruction (Fig. 3) resulted in a monophyletic Diphyllatea grouping with full bootstrap support (BS) and posterior probability (PP). Further, Diphyllatea formed a fully supported (100 BS / 1.00 PP) clade with Rigifila ramosa and Micronuclearia podoventralis (order Rigifilda) [5, 9].

Sequences within Diphyllatea (Fig. 3) were divided into three clades, all fully supported. Two of these include the previously known genera Diphylleia and Collodictyon, here marked Diphy I and II respectively. Furthermore, and most importantly, the tree reveals a new Diphyllatea clade distinct from the previous two. The new clade, here named Diphy III, branches off as a sister clade to Diphy II with full support, though both clades represent species with a comparable Collodictyon morphology. All 11 cultured strains are placed within Collodictyon (Diphy II and III); two placing within Diphy II (Å85 and KIVT03), and the remaining nine within Diphy III (KIINB, KIKNR01, KIKNR02, KIKNR03, KIVT01, KIVT02, KIVT04, KIVTT01 and KIVTT02).

To increase phylogenetic resolution of the ingroup, the phylogeny was additionally inferred without outgroup taxa (Additional file 1: Figure S3). This inference was equivalent to that of Fig. 1, with higher support for the observed branching patterns. The major difference between the two analyses was the separation of Diphy III strains into two supported clades.


Cultured Diphyllatea show a Collodictyon morphology

Diphyllatea, dependent on the position of the eukaryotic root, may represent one of the earliest branching eukaryote lineages, and as such is of pivotal importance for reconstructing eukaryotic evolution. Still, virtually nothing is known about the higher order phylogenetic structure, diversity and geographic dispersal of this deep lineage. Here we address these issues by combining culturing, rRNA sequencing of new strains and targeted 18S rRNA PCR of natural samples sequenced with PacBio RS II technology.

Morphologically these isolates all seem to be strains of C. triciliatum or closely related species, supporting earlier studies that Diphyllatea encompasses a limited species number [8, 11,12,13]. Alternatively, a similar phenotype may represent multiple cryptic species with distinct genotypes (or ribotypes).

Diphyllatea unconfirmed in marine habitats

Altogether, our PCR amplification and database searches could only detect Diphyllatea in freshwater, suggesting that the class maybe restricted to freshwater habitats. Knowledge of Diphyllatea habitat preferences and distributions in environmental systems remains limited. Therefore, the development of targeted PCR approaches, presented here, can be useful in future studies on additional environments.

Phylogeny and diversity of the class Diphyllatea

As we show that the C. triciliatum morphospecies concept encompasses two distinct molecular clades within Diphyllatea, future microscopy work should establish what taxonomic levels these represent, and if possible, which is most congruent with the morphological description of the type species. The taxonomic rank Diphy I-III is not clear, but all groups contain higher diversity than earlier known, and several substructures that might constitute different sub-groups It should also be noted that Diphy III is likely to be a clade at least on the same taxonomic level as Diphy I and II. Considering the sequence divergence between Diphy II and III: Only 79% sequence identity was shared over the rRNA length, increasing to 85% for the more conserved 18S rRNA region, suggesting these clades are at least separate genera with a shared morphology. Another distinct pattern in the tree, is the placement of Diphylleia BOR41 environmental OTU, which placed as sister to Diphy I and excluded from this clade with almost full support (99/1.00), and 95 BS in Additional file 1: Figure S3, but still showed > 98% pairwise identity to the other OTUs in Diphy I, suggesting Diphylleia likely constitutes several uncharacterized cryptic species (Fig. 3 and Additional file 1: Figure S3).

Mapping the morphology to the tree shows that the quadriflagellate forms branch together as two main monophyletic groups (i.e. Diphy II and III), implying that Diphyllatea as a group is deeply divided into two clades composed of quadriflagellate or biflagellate (Diphy I) forms. As the flagella of Collodictyon occupy the same position as the basal body in a pre-division stage of Diphylleia [6], and the cyst stage has two long gelatinous filaments [64], it could be hypothesised that the two forms represent different life-stages of the same species. However, no biflagellate stage was observed for our Diphy II and III cultures, with the phylogeny consistently separating the biflagellate Diphylleia from the two clades of quadriflagellate Collodictyon species. Hence, the morphological change in Diphyllatea has most likely occurred early in the history of the group. Dependent on the final position of the eukaryote root, this event may represent one of the most ancient morphological innovations known among eukaryotes.

Currently, available sequence data suggests a single biflagellate clade (Diphy I). However, additional sequence data is needed to confirm that Sulcomonas lacustris and possible cryptic Diphyllatea species place within the Diphy I clade.

To further understand the evolution of Diphyllatea, the ancestral form and its relationship within Sulcozoa, the genomes of multiple species are essential. For this reasoning, we are currently completing the annotation of genomes from each of the three Diphyllatea clades, in addition to that of Rigifila ramosa (Rigifilda).

A global distribution of Diphyllatea

The substantial increase in Diphyllatea sequence data presented, allows, for the first time, conclusions to be drawn as to the extent and ecological role of the class and genera therein.

The Diphy I clade (Fig. 3), representing the biflagellate cell-type, constituted sequences from Borneo, China, France, Japan, Netherlands and Norway, including the previously reported ribotypes from Tibet (China) and Clermont-Ferrand (France) [6, 18]. In addition to the localities above, Diphylleia has also be reported in Saudi Arabia [15], suggesting a global distribution of the genus.

The Diphy II clade constituted sequences from Borneo and Norway, from both culture and environmental samples. The Diphy III clade, in contrast, constituted only cultured sequence data from Asia (Japan, Thailand and Vietnam) with no environmental Diphyllatea amplicons having an affinity to this clade. Collodictyon, the quadriflagellate form (represented in Diphy II and III clades; Fig. 3), has been previously described from the island of Bombay and later in central Europe, Spain and Norway [11, 14, 23, 24]. The quadriflagellate morphotype has additionally been reported in North America [11, 22, 23], and more recently South America; from multiple freshwater localities in Uruguay: La Oriental, Maldonado (34°34’S 55°15’W), Tala, Canelones (34°20’S 55°45’W), and Picada Varela, San José River, San José (34°19’S 56°42’W). Accompanying video is available through (uuvb3eUZUQ8, AsY8s-HnTMQ, M8tAf3KoDQM and k88LsRcEXmg). As only morphological data is presented, in the reports above, we are unable to establish if these morphotypes represent Diphy II and/or III, however it does confirm a global distribution of the Collodictyon morphotype and accordingly the Diphyllatea class.

Interestingly, all environmental sequence data for Diphyllatea deposited in public databases were only related to the Diphy I clade. The reason for this pattern is unlikely a PCR primer bias, as the used primers show full match to all three Diphy groups. It may rather indicate higher abundance of Diphy I in the sampled localities or could reflect different habitat preferences among the three Diphy groups.

PacBio SMRT sequencing of targeted Diphyllatea amplicons

The PacBio RS sequencing platform has been previously used to study 16S [39, 40] and more recently 18S rRNA gene amplicons [41, 42]. Jones and Kustka sequenced the V7–9 region of 18S rRNA to answer questions about total eukaryotic diversity from marine samples [41]. Tedersoo et al., targeted the V4 (18S) - D3 (28S) region focusing on total eukaryotic and fungal diversity from soil samples, confirming PacBio as an alternative for metabarcoding of organisms with low diversity for reliable identification and phylogenetic approaches [42]. In contrast to these studies, which surveyed a broader eukaryotic diversity, our goal was a targeted 18S rRNA approach. Our result demonstrates PacBio RS as an efficient and economical alternative to the traditional cloning and Sanger method for sequencing long rRNA amplicons [32,33,34]; A single SMRT cell gave 6310 total reads of insert (Additional file 1: Table S2), which constituted 1741 high quality sequences (CCS = 1) and 281 OTUs. To achieve a comparable number of sequences via cloning and Sanger sequencing would be a tedious exercise, at an approximate cost 30× higher than that of the PacBio RS method (based on CCS = 1 result).

The major advantage of PacBio RS for the study eukaryotic of diversity is read length, which allows for higher phylogenetic resolution. Additionally, long-reads allow short-read amplicon datasets from different rRNA regions to be “scaffolded” and inferred in parallel, further increasing resolution. However, PacBio RS does have a high error rate, ~15% with the P4-C2 chemistry due to the random addition of incorrect nucleotides [65]. To overcome the random error rate, DNA is ligated into SMRT bells; circular DNA fragments that allow multiple sequence passes, a process termed Circular Consensus Sequencing (CCS), and further accounted for with a sequence analysis pipeline. Our results demonstrate an analysis pipeline as essential for the removal of sequencing errors that can affect variability and show the Årungen PacBio OTU and the clonal Å85 Sanger sequence to be 100% identical over sequence length. Additionally, chimeras, that increase proportionally with amplicon length [42, 66] can give an overestimation of diversity; Of the 1741 high quality sequences, 186 (11.44%) were identified as chimeric using Uchime (Additional file 1: Table S2). The high level of chimeric sequences identified was surprising, with only a 1–2% chimera level previously reported [39, 65] by “misligation” of SMRTbell adaptors in the PacBio library preparation. The observed chimera level is therefore attributed to PCR artefacts; It has been proposed that > 45% of reads in some datasets are chimeric [66,67,68], with experiments showing that > 30% of chimeras can be attributed to PCR [69]. Formation of PCR chimeras increases with amplicon length, a result of template switching [66], as such filters to identify and remove long-read amplicon chimeras (i.e. Uchime) are paramount. It is difficult to ascertain if the observed chimeras are a result of the original 18S rRNA amplification or the subsequent PCR to attach symmetric PacBio barcodes. It is possible, however to reduce the former by decreasing amplification cycles [70], and eradicate the latter by barcode ligation or the sequencing of separate samples, instead of multiplexing. It has been previously reported that Uchime fails to identify all long-read amplicon chimeras [39], though we found no evidence supporting this in our dataset.

In agreement with previous studies [41, 42], we find that long-read PacBio RS sequencing provides high phylogenetic resolution for eukaryotic diversity studies. Further, PacBio will improve with technological and chemical developments, allowing for longer and more accurate reads with higher output [39], with the recent release of PacBio Sequel confirming [42, 71]. Understanding PacBio biases will allow for improved bioinformatic pipelines, and as such phylogenetic inferences [39]. It should be noted that Oxford Nanopore sequencing platform has recently been applied to 16S rRNA gene amplicons [72], and may offer an alternative for the study of eukaryotic diversity with long-reads.


In this study, the application of culturing Diphyllatea protists in parallel with Sanger sequencing the partial rRNA operon from multiple strains, reveals two quadriflagellate ribotypes despite only a single morphotype being observed. Further, the inference of Diphyllatea cultured sequences with that of database orthologues and environmental amplicons infers a greater Diphyllatea diversity than previously known, recovering three clearly phylogenetically separated groupings (Diphy I, II, and III). The substantial addition of sequence data, in this study, resolves relationships between genera. We show a split between the Diphy I and Diphy II + III clades corresponding to a morphological division of Diphyllatea into bi- and quadriflagellate cell forms. The altered Diphyllatea morphology most likely occurred early in the history of the group and may represent one of the most ancient morphological innovations known among eukaryotes. Furthermore, environmental sequences and database mining show a global distribution of Diphyllatea with a dispersal restricted to freshwater habitats.

Our results suggest that combining culture methods with a group-specific PCR approach and long-read sequencing is invaluable for understanding the diversity and distribution of protist lineages, in particular Diphyllatea, and their ecological importance in aquatic systems. Here we provide the tools to uncover the true diversity of this class.

Lastly, our study shows the capacity of PacBio RS when employing a targeted approach for increasing phylogenetic resolution of a protist class. Although caution needs to be observed when analysing reads, to avoid a chimeric overestimation of diversity, the platform offers major economical and efficiency gains over traditional cloning and Sanger sequencing methods, something that will improve with technological advances.

Change history

  • 03 August 2018

    In the original publication of this article [1] there was an error in an author name. In this correction article the correct and incorrect name are indicated.



Bootstrap support


Circular consensus sequencing


Differential interference contrast


Electron microscopy


Global ocean sampling


Markov Chain Monte Carlo


Natural History Museum, London


Norwegian Institute for Water research


Norwegian Sequencing Centre


Operational taxonomic unit


Pacific Bioscience


Polymerase Chain Reaction


Posterior probability


University of Oslo


  1. 1.

    Zhao S, Burki F, Bråte J, Keeling PJ, Klaveness D, Shalchian-Tabrizi K. Collodictyon—An Ancient Lineage in the Tree of Eukaryotes. Mol Biol Evol. 2012;29(6):1557-68.

  2. 2.

    Brown MW, Sharpe SC, Silberman JD, Heiss AA, Lang BF, Simpson AGB, Roger AJ. Phylogenomics demonstrates that breviate flagellates are related to opisthokonts and apusomonads. Proc R Soc B Biol Sci. 2013;280(1769):20131755.

    Article  Google Scholar 

  3. 3.

    Burki F, Kaplan M, Tikhonenkov DV, Zlatogursky V, Minh BQ, Radaykina LV, Smirnov A, Mylnikov AP, Keeling PJ. Untangling the early diversification of eukaryotes: a phylogenomic study of the evolutionary origins of Centrohelida, Haptophyta and Cryptista. Proc R Soc B Biol Sci. 2016;283(1823):20152802.

    Article  Google Scholar 

  4. 4.

    Zhao S, Shalchian-Tabrizi K, Klaveness D. Sulcozoa revealed as a paraphyletic group in mitochondrial phylogenomics. Mol Phylogenet Evol. 2013;69(3):462–8.

    PubMed  CAS  Article  Google Scholar 

  5. 5.

    Brown MW, Heiss AA, Kamikawa R, Inagaki Y, Yabuki A, Tice AK, Shiratori T, Ishida K-I, Hashimoto T, Simpson AGB, et al. Phylogenomics places orphan Protistan lineages in a novel eukaryotic super-group. Genome Biol Evol. 2018;10(2):427–33.

    PubMed  PubMed Central  Article  Google Scholar 

  6. 6.

    Brugerolle G, Bricheux G, Philippe H, Coffea G. Collodictyon triciliatum and Diphylleia rotans (=Aulacomonas submarina) form a new family of flagellates (Collodictyonidae) with tubular mitochondrial cristae that is phylogenetically distant from other flagellate groups. Protist. 2002;153(1):59-70.

  7. 7.

    Brugerolle G, Patterson DJ. A cytological study of Aulacomonas submarina Skuja 1939, a heterotrophic flagellate with a novel ultrastructural identity. Eur J Protistol. 1990;25(3):191–9.

  8. 8.

    Brugerolle G. Description of a new freshwater heterotrophic flagellate Sulcomonas lacustris affiliated to the Collodictyonids. Acta Protozool. 2006;45:175–82.

    Google Scholar 

  9. 9.

    Cavalier-Smith T. Early evolution of eukaryote feeding modes, cell structural diversity, and classification of the protozoan phyla Loukozoa, Sulcozoa, and Choanozoa. Eur J Protistol. 2013;49(2):115–78.

    PubMed  Article  Google Scholar 

  10. 10.

    Ruggiero MA, Gordon DP, Orrell TM, Bailly N, Bourgoin T, Brusca RC, Cavalier-Smith T, Guiry MD, Kirk PM. A higher level classification of all living organisms. PLoS One. 2015;10(4):e0119248.

    PubMed  PubMed Central  Article  Google Scholar 

  11. 11.

    Carter HJ. XXXII.—on the fresh- and salt-water Rhizopoda of England and India. In: Annals and Magazine of Natural History, vol. 15. UK: Taylor & Francis; 1865. p. 277–93.

  12. 12.

    Francé R. A Collodictyon triciliatum cart. Szervezete (Über den Organismus Collodictyon triciliatum cart). In: Termeszetrai füzetek. vol. 22. Budapest: Tabla; 1899. p. 1–26.

    Google Scholar 

  13. 13.

    Massart J. Recherches sur les organismes inférieurs. VIII.- sur la motilité des flagellates. Académie Royale d'e Belgique Bulletin de la Classe des. Sciences. 1920;5(6):116–41.

    Google Scholar 

  14. 14.

    Klaveness D. Collodictyon triciliatum H.J. Carter (1865) - a common but fixation-sensitive Algivorous flagellate from the Limnopelagial. Nord J Freshw Res. 1995;70:3–11.

    Google Scholar 

  15. 15.

    Mohamed ZA, Al-Shehri AM. Grazing on Microcystis aeruginosa and degradation of microcystins by the heterotrophic flagellate Diphylleia rotans. Ecotoxicol Environ Saf. 2013;96:48–52.

    PubMed  CAS  Article  Google Scholar 

  16. 16.

    Bo-Ra K, Shin-ichi N, Baik-Ho K, Myung-Soo H. Grazing and growth of the heterotrophic flagellate Diphylleia rotans on the cyanobacterium Microcystis aeruginosa. Aquat Microb Ecol. 2006;45(2):163–70.

    Google Scholar 

  17. 17.

    Wawrik F. Collodictyon Studien. Arch Protistenkunde. 1973;115:353–6.

    Google Scholar 

  18. 18.

    Wu QL, Chatzinotas A, Wang J, Boenigk J. Genetic diversity of eukaryotic plankton assemblages in eastern Tibetan Lakes differing by their salinity and altitude. Microb Ecol. 2009;58(3):569–81.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  19. 19.

    Bass D, Cavalier-Smith T. Phylum-specific environmental DNA analysis reveals remarkably high global biodiversity of Cercozoa (Protozoa). Int J Syst Evol Microbiol. 2004;54(6):2393–404.

    PubMed  CAS  Article  Google Scholar 

  20. 20.

    Potvin M, Lovejoy C. PCR-based diversity estimates of artificial and environmental 18S rRNA gene libraries. J Eukaryot Microbiol. 2009;56(2):174–81.

    PubMed  CAS  Article  Google Scholar 

  21. 21.

    Bråte J, Klaveness D, Rygh T, Jakobsen KS, Shalchian-Tabrizi K. Telonemia-specific environmental 18S rDNA PCR reveals unknown diversity and multiple marine-freshwater colonizations. BMC Microbiol. 2010;10(1):168.

    PubMed  PubMed Central  Article  Google Scholar 

  22. 22.

    Lackey JB. The plankton algae and Protozoa of two Tennessee rivers. Am Midl Nat. 1942;27(1):191–202.

    Article  Google Scholar 

  23. 23.

    Rhodes RC. Binary fission in Collodictyon tricilliatum. Berkeley: University of California; 1917.

    Google Scholar 

  24. 24.

    Sánchez JC, Cobelas MÁ, Sanjurjo MA. Lista florística y bibliográfica de los clorófitos (Chlorophyta) de la Península Ibérica, Islas Baleares e Islas Canarias. the University of California. Spain: Asociación Española de Limnología; 1998.

  25. 25.

    Bradley IM, Pinto AJ, Guest JS. Design and evaluation of Illumina MiSeq-compatible, 18S rRNA gene-specific primers for improved characterization of mixed phototrophic communities. Appl Environ Microbiol. 2016;82(19):5878–91.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  26. 26.

    de Vargas C, Audic S, Henry N, Decelle J, Mahé F, Logares R, Lara E, Berney C, Le Bescot N, Probert I, et al. Eukaryotic plankton diversity in the sunlit ocean. Science. 2015;348(6237)

  27. 27.

    Hugerth LW, Muller EEL, Hu YOO, Lebrun LAM, Roume H, Lundin D, Wilmes P, Andersson AF. Systematic design of 18S rRNA gene primers for determining eukaryotic diversity in microbial consortia. PLoS One. 2014;9(4):e95567.

    PubMed  PubMed Central  Article  Google Scholar 

  28. 28.

    Al-Bulushi IM, Bani-Uraba MS, Guizani NS, Al-Khusaibi MK, Al-Sadi AM. Illumina MiSeq sequencing analysis of fungal diversity in stored dates. BMC Microbiol. 2017;17(1):72.

    PubMed  PubMed Central  Article  Google Scholar 

  29. 29.

    Taylor DL, Walters WA, Lennon NJ, Bochicchio J, Krohn A, Caporaso JG, Pennanen T. Accurate estimation of fungal diversity and abundance through improved lineage-specific primers optimized for Illumina amplicon sequencing. Appl Environ Microbiol. 2016;82(24):7217–26.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  30. 30.

    Asemaninejad A, Weerasuriya N, Gloor GB, Lindo Z, Thorn RG. New primers for discovering fungal diversity using nuclear large ribosomal DNA. PLoS One. 2016;11(7):e0159043.

    PubMed  PubMed Central  Article  Google Scholar 

  31. 31.

    Mueller RC, Gallegos-Graves LV, Kuske CR. A new fungal large subunit ribosomal RNA primer for high-throughput sequencing surveys. FEMS Microbiol Ecol. 2016, 92(2):fiv153.

  32. 32.

    Bachy C, Dolan JR, López-García P, Deschamps P, Moreira D. Accuracy of protist diversity assessments: morphology compared with cloning and direct pyrosequencing of 18S rRNA genes and ITS regions using the conspicuous tintinnid ciliates as a case study. ISME J. 2013;7(2):244–55.

    PubMed  CAS  Article  Google Scholar 

  33. 33.

    Edgcomb V, Orsi W, Bunge J, Jeon S, Christen R, Leslin C, Holder M, Taylor GT, Suarez P, Varela R, et al. Protistan microbial observatory in the Cariaco Basin, Caribbean. I. Pyrosequencing vs sanger insights into species richness. ISME J. 2011;5(8):1344–56.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  34. 34.

    Thomas MC, Selinger LB, Inglis GD. Seasonal diversity of planktonic Protists in southwestern Alberta rivers over a 1-year period as revealed by terminal restriction fragment length polymorphism and 18S rRNA gene library analyses. Appl Environ Microbiol. 2012;78(16):5653–60.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  35. 35.

    Orr RJS, Rombauts S, Van de Peer Y, Shalchian-Tabrizi K. Erratum for Orr et al., Draft Genome Sequences of Two Unclassified Chitinophagaceae Bacteria, IBVUCB1 and IBVUCB2, Isolated from Environmental Samples. Genome Announcements. 2017;5(41).

  36. 36.

    Hoang NV, Furtado A, Mason PJ, Marquardt A, Kasirajan L, Thirugnanasambandam PP, Botha FC, Henry RJ. A survey of the complex transcriptome from the highly polyploid sugarcane genome using full-length isoform sequencing and de novo assembly from short read sequencing. BMC Genomics. 2017;18(1):395.

    PubMed  PubMed Central  Article  Google Scholar 

  37. 37.

    Kuo RI, Tseng E, Eory L, Paton IR, Archibald AL, Burt DW. Normalized long read RNA sequencing in chicken reveals transcriptome complexity similar to human. BMC Genomics. 2017;18(1):323.

    PubMed  PubMed Central  Article  Google Scholar 

  38. 38.

    Orr RJS, Rombauts S, Van de Peer Y, Shalchian-Tabrizi K. Erratum for Orr et al., Draft Genome Sequences of Two Unclassified Bacteria, Sphingomonas sp. Strains IBVSS1 and IBVSS2, Isolated from Environmental Samples. Genome Announcements. 2017;5(41).

  39. 39.

    Fichot EB, Norman RS. Microbial phylogenetic profiling with the Pacific biosciences sequencing platform. Microbiome. 2013;1(1):10.

    PubMed  PubMed Central  Article  Google Scholar 

  40. 40.

    Mosher JJ, Bernberg EL, Shevchenko O, Kan J, Kaplan LA. Efficacy of a 3rd generation high-throughput sequencing platform for analyses of 16S rRNA genes from environmental samples. J Microbiol Methods. 2013;95(2):175–81.

    PubMed  CAS  Article  Google Scholar 

  41. 41.

    Jones BM, Kustka AB. A quantitative SMRT cell sequencing method for ribosomal amplicons. J Microbiol Methods. 2017;135:77–84.

    PubMed  CAS  Article  Google Scholar 

  42. 42.

    Leho T, Ave T-K, Sten A. PacBio metabarcoding of Fungi and other eukaryotes: errors, biases and perspectives. New Phytologist. 2018;217(3):1370-85.

  43. 43.

    Kimura B, Ishida Y. Photophagotrophy in Uroglena americana, Chrysophyceae. Jpn J Limnol (Rikusuigaku Zasshi). 1985;46(4):315–8.

    Article  Google Scholar 

  44. 44.

    Guillard RRL, Lorenzen CJ. Yellow green algae with chlorophyllide C1,2. J Phycol. 1972;8(1):10–4.

  45. 45.

    Stanier RY, Kunisawa R, Mandel M, Cohen-Bazire G. Purification and properties of unicellular blue-green algae (order Chroococcales). Bacteriol Rev. 1971;35(2):171–205.

    PubMed  PubMed Central  CAS  Google Scholar 

  46. 46.

    Doyle JJ, Doyle JL. A rapid DNA isolation procedure for small quantities of fresh leaf tissue. Phytochemistry Bull Bot Soc Am. 1987;19:11–5.

    Google Scholar 

  47. 47.

    Gadberry MD, Malcomber ST, Doust AN, Kellogg EA. Primaclade - a flexible tool to find conserved PCR primers across multiple species. Bioinformatics. 2005;21(7):1263–4.

    PubMed  CAS  Article  Google Scholar 

  48. 48.

    Gordon D, Abajian C, Green P. Consed: a graphical tool for sequence finishing. Genome Res. 1998;8(3):195–202.

    PubMed  CAS  Article  Google Scholar 

  49. 49.

    Maddison WP, Maddison DR: Mesquite: a modular system for evolutionary analysis. Version 3.1; 2017.

  50. 50.

    Katoh K, Standley DM. MAFFT multiple sequence alignment software version 7: improvements in performance and usability. Mol Biol Evol. 2013;30(4):772–80.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  51. 51.

    Cavalier-Smith T, Chao EE. Phylogeny and evolution of Apusomonadida (Protozoa: Apusozoa): new genera and species. Protist. 2010;161(4):549–76.

    PubMed  Article  Google Scholar 

  52. 52.

    Kibbe WA. OligoCalc: an online oligonucleotide properties calculator. Nucleic Acids Res. 2007;35:W43–6.

    PubMed  PubMed Central  Article  Google Scholar 

  53. 53.

    Logares R, Audic S, Bass D, Bittner L, Boutte C, Christen R, Claverie J-M, Decelle J, Dolan John R, Dunthorn M, et al. Patterns of rare and abundant marine microbial eukaryotes. Curr Biol. 2014;24(8):813–21.

    PubMed  CAS  Article  Google Scholar 

  54. 54.

    Edgar RC. Search and clustering orders of magnitude faster than BLAST. Bioinformatics. 2010;26(19):2460–1.

    PubMed  CAS  Article  Google Scholar 

  55. 55.

    Edgar RC, Haas BJ, Clemente JC, Quince C, Knight R. UCHIME improves sensitivity and speed of chimera detection. Bioinformatics. 2011;27(16):2194-200.

  56. 56.

    Stoeck T, Bass D, Nebel M, Christen R, Jones MDM, Breiner H, Richards TA. Multiple marker parallel tag environmental DNA sequencing reveals a highly complex eukaryotic community in marine anoxic water. Mol Ecol. 2010;19(s1):21–31.

    PubMed  CAS  Article  Google Scholar 

  57. 57.

    Maritz JM, Rogers KH, Rock TM, Liu N, Joseph S, Land KM, Carlton JM. An 18S rRNA workflow for characterizing Protists in sewage, with a focus on zoonotic Trichomonads. Microb Ecol. 2017;74(4):923–36.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  58. 58.

    Wu L, Wen C, Qin Y, Yin H, Tu Q, Van Nostrand JD, Yuan T, Yuan M, Deng Y, Zhou J. Phasing amplicon sequencing on Illumina Miseq for robust environmental microbial community analysis. BMC Microbiol. 2015;15:125.

    PubMed  PubMed Central  Article  Google Scholar 

  59. 59.

    Senés-Guerrero C, Schüßler A. A conserved arbuscular mycorrhizal fungal core-species community colonizes potato roots in the Andes. Fungal Divers. 2016;77(1):317–33.

    Article  Google Scholar 

  60. 60.

    Talavera G, Castresana J. Improvement of phylogenies after removing divergent and ambiguously aligned blocks from protein sequence alignments. Syst Biol. 2007;56(4):564–77.

    PubMed  CAS  Article  Google Scholar 

  61. 61.

    Stamatakis A. RAxML-VI-HPC: maximum likelihood-based phylogenetic analyses with thousands of taxa and mixed models. Bioinformatics. 2006;22(21):2688–90.

    PubMed  CAS  Article  Google Scholar 

  62. 62.

    Huelsenbeck J, Ronquist F. MrBayes: Bayesian inference of phylogenetic trees. Bioinformatics. 2001;17:754–5.

    PubMed  CAS  Article  Google Scholar 

  63. 63.

    de Vienne DM, Giraud T, Martin OC. A congruence index for testing topological similarity between trees. Bioinformatics. 2007;23(23):3119–24.

    PubMed  CAS  Article  Google Scholar 

  64. 64.

    Mischke U. Influence of food quality and quantity on ingestion and growth rates of three omnivorous heterotrophic flagellates. Mar Microb Food Webs. 1994;8:125–43.

    Google Scholar 

  65. 65.

    Koren S, Schatz MC, Walenz BP, Martin J, Howard JT, Ganapathy G, Wang Z, Rasko DA, McCombie WR, Jarvis ED, et al. Hybrid error correction and de novo assembly of single-molecule sequencing reads. Nat Biotech. 2012;30(7):693–700.

    CAS  Article  Google Scholar 

  66. 66.

    Laver TW, Caswell RC, Moore KA, Poschmann J, Johnson MB, Owens MM, Ellard S, Paszkiewicz KH, Weedon MN. Pitfalls of haplotype phasing from amplicon-based long-read sequencing. Sci Rep. 2016;6:21746.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  67. 67.

    Ashelford KE, Chuzhanova NA, Fry JC, Jones AJ, Weightman AJ. New screening software shows that most recent large 16S rRNA gene clone libraries contain chimeras. Appl Environ Microbiol. 2006;72(9):5734–41.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

  68. 68.

    Huber T, Faulkner G, Hugenholtz P. Bellerophon: a program to detect chimeric sequences in multiple sequence alignments. Bioinformatics. 2004;20(14):2317–9.

    PubMed  CAS  Article  Google Scholar 

  69. 69.

    Wang GC, Wang Y. Frequency of formation of chimeric molecules as a consequence of PCR coamplification of 16S rRNA genes from mixed bacterial genomes. Appl Environ Microbiol. 1997;63(12):4645–50.

    PubMed  PubMed Central  CAS  Google Scholar 

  70. 70.

    Smyth RP, Schlub TE, Grimm A, Venturi V, Chopra A, Mallal S, Davenport MP, Mak J. Reducing chimera formation during PCR amplification to ensure accurate genotyping. Gene. 2010;469(1–2):45–51.

    PubMed  CAS  Article  Google Scholar 

  71. 71.

    Hebert PDN, Braukmann TWA, Prosser SWJ, Ratnasingham S, deWaard JR, Ivanova NV, Janzen DH, Hallwachs W, Naik S, Sones JE, et al. A Sequel to Sanger: amplicon sequencing that scales. BMC Genomics. 2018;19(1):219.

  72. 72.

    Ma X, Stachler E, Bibby K. Evaluation of Oxford Nanopore MinION sequencing for 16S rRNA microbiome characterization. bioRxiv. 2017.

  73. 73.

    Hendriks L, Goris A, Neefs JM, Van de Peer Y, Hennebert G, Dewachter R. The nucleotide-sequence of the small ribosomal-subunit RNA of the yeast Candida albicans and the evolutionary position of the Fungi among the eukaryotes. Syst Appl Microbiol. 1989;12(3):223–9.

    CAS  Article  Google Scholar 

  74. 74.

    Medlin L, Elwood H, Stickel S, Sogin M. The characterization of enzymatically amplified eukaryotic 16S-like rRNA-coding regions. Gene. 1988;71:491–9.

    PubMed  CAS  Article  Google Scholar 

  75. 75.

    Schmitt I, Crespo A, Divakar PK, Fankhauser JD, Herman-Sackett E, Kalb K, Nelsen MP, Nelson NA, Rivas-Plata E, Shimp AD, et al. New primers for promising single-copy genes in fungal phylogenetics and systematics. Persoonia. 2009;23:35–40.

    PubMed  PubMed Central  CAS  Article  Google Scholar 

Download references


We would like to thank Abel (UoO) for providing computing resources, in particular projects nn9244k and nn9404k. We thank the Norwegian Sequencing Centre (NSC) for providing advice related to PacBio sequencing and analysis. We are grateful to Dr. David Bass and Dr. Bente Edvardsen, representing Biomarks, for providing environmental DNA samples. The Norwegian Institute for Water research (NIVA) are acknowledged for providing the Microcystis strain CYA 43. We thank Katherine Schou and Dr. Anders Krabberød (UoO) for laboratory support and discussion in formulating this paper. Thanks, are given to Dr. Takashi Shiratori and Dr. Ken Ishida from the University of Tsukuba for providing the D. rotans strain for a separate genomic study. Finally, we thank two anonymous reviewers for comments that improved this publication.


This work has been supported by research grants from the Norwegian Research Council to R.J.S.O (project 230868) and the University of Oslo to K.S.-T. and D.K. The funding bodies had no role in the design of the study, collection, analysis, interpretation of data nor the writing of the manuscript.

Availability of data and materials

All sequences produced in this study have been deposited in the NCBInr database under the accessions MF039351-MF039368. In addition, the alignments used for phylogenetic inference (both masked and unmasked) and videos of Diphyllatea have been made freely available through the authors ResearchGate pages via the following links: and

Author information




Research conception and design: RJSO, KST; Data collection: RJSO, SZ, DK, AY, IK, MMW; Analysis and interpretation: RJSO, SZ, DK, KST; Drafting the paper: RJSO, SZ; Critical revision of the paper: RJSO, KST; Obtained funding: RJSO, KST. All authors read and approved the final manuscript.

Corresponding authors

Correspondence to Russell J. S. Orr or Kamran Shalchian-Tabrizi.

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The author name of Dr. Watanabe was incorrect in the original publication and has been updated. Details are available in the related correction article

Additional files

Video S1. Motile Collodictyon cell. With relaxed movement and rotation driven by flagella. Collodictyon Å85 strain is shown. Video is filmed using a Nikon D300S on a Nikon Diaphot inverted microscope. (M4V 3804 kb)

Video S2. Cytoplasmic veil and pseudopodia. A Collodictyon cell clinging to the surface of the culture dish by a cytoplasmic veil and pseudopodia (i.e. the amoeboid property). Collodictyon Å85 strain is shown. Video is filmed using a Nikon D300S on a Nikon Diaphot inverted microscope. (M4V 6311 kb)

Additional file 1:

Table S1. Sanger sequencing primers. Table S2. Sequencing results for environmental amplicons per barcode. Figure S1. PacBio sequencing results. Figure S2. The 18S rRNA phylogeny of Diphyllatea. Figure S3. The rRNA phylogeny of Diphyllatea excluding outgroup taxa. Figure S4. Total diversity of generated OTUs. (DOCX 1098 kb)

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Orr, R.J.S., Zhao, S., Klaveness, D. et al. Enigmatic Diphyllatea eukaryotes: culturing and targeted PacBio RS amplicon sequencing reveals a higher order taxonomic diversity and global distribution. BMC Evol Biol 18, 115 (2018).

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  • Diphyllatea
  • PacBio
  • rRNA
  • Phylogeny
  • Collodictyon
  • Amplicon