Open Access

Nephroselmis viridis (Nephroselmidophyceae, Chlorophyta), a new record for the Atlantic Ocean based on molecular phylogeny and ultrastructure

  • Karoline Magalhães Ferreira Lubiana1Email author,
  • Sônia Maria Flores Gianesella2,
  • Flávia Marisa Prado Saldanha-Corrêa2 and
  • Mariana Cabral Oliveira1
Marine Biodiversity Records201710:5

DOI: 10.1186/s41200-017-0107-0

Received: 25 October 2016

Accepted: 19 January 2017

Published: 2 February 2017


Nephroselmis is composed by unicellular nanoplanktonic organisms, occurring predominantly in marine environments. Currently, 14 species are taxonomically accepted. Nephroselmis viridis was described in 2011 and strains were isolated from Indic and Pacific Oceans. Since then, it was not recorded in other places. A strain was isolated from coastal waters of Brazil by micropipetting and washing, and cultivated in f/2 medium for morphological observations (light, confocal, SEM and TEM) and molecular phylogeny inferences (maximum likelihood and Bayesian). The cells are asymmetrical, have two unequal flagella, one cup-shaped chloroplast with an eyespot, and a large starch covered pyrenoid. Chloroplast thylakoids intrude into the pyrenoid and organic scales cover all cell body and flagella. Molecular phylogeny (18S rRNA) clustered the isolated strain with other Nephroselmis viridis sequences, and the species is the sister of the N. olivacea, the type species of the genus. Morphology and molecular phylogeny corroborate the strain identification, and it is the first time this species is recorded in Brazil and in the Atlantic Ocean.


Brazilian coast 18S rRNA Strain isolation Morphology Biodiversity


Nephroselmis was described in 1879 by the typification of Nephroselmis olivacea Stein, and initially was allocated into Cryptophyceae (Parke and Rayns 1964). Further studies moved it to Chlorophyta, and Bourelly, in 1970, classified it as Prasinophyceae (Norris 1980). In the last decades, many studies taking into account molecular phylogeny have shown that Prasinophyceae is not monophyletic (Marin and Melkonian 2010; Marin and Melkonian 1994; Nakayama et al. 1998; Steinkotter et al. 1994). Hence, the class Nephroselmidophyceae (Nephrophyceae) was proposed to accommodate the genus (Cavalier-Smith 1993; Nakayama et al. 2007). This class seems to be an early derived clade of the core Chlorophyta (Daugbjerg et al. 1995; Nakayama et al. 1998; Steinkotter et al. 1994; Turmel et al. 2009; Turmel et al. 1999), keeping a high number of ancestral characters.

Currently, 14 species of Nephroselmis are taxonomically accepted (Guiry and Guiry 2016), and except for N. olivacea which is freshwater, all other species are brackish or marine. The nuclear gene coding for the ribosomal small subunit RNA (18S rDNA) is the most widely used molecular marker for this group (Bell 2008; Faria et al. 2012; Faria et al. 2011; Nakayama et al. 2007; Nakayama et al. 1998; Yamaguchi et al. 2011). However, sequences for just nine species of this molecular marker are available in Genbank, representing less than 65% of the genus biodiversity.

Nephroselmis viridis Inouye, Pienaar, Suda & Chihara was described in 2011 and strains were isolated from marine waters of Fiji, Japan and South Africa, in the Pacific and Indic Oceans (Yamaguchi et al. 2011). In the Atlantic Ocean, just five Nephroselmis species were recorded previously, vis., N. discoidea Skuja (Menezes and Bicudo 2008), N. fissa (Lackey 1940), N. minuta (N.Carter) Butcher (Butcher 1959; Domingos and Menezes 1998), N. pyriformis (N.Carter) Ettl (Bergesch et al. 2008; Moestrup 1983; Steinkotter et al. 1994), and N. rotunda (N.Carter) Fott (Bell 2008; Butcher 1959). Therefore, here we report for the first time the occurrence of N. viridis in Atlantic Ocean, isolated from the coast of Brazil, identified by molecular and microscopy tools.


Strain isolation and culturing conditions

The strain was isolated from a water sample collected in coastal area of Ubatuba, São Paulo, Brazil, close to Anchieta Island (23° 35.847′ S, 45° 01.70′ W), at a depth of 40 m. In the laboratory, a drop of the water sample was used to select the cell, which was transferred successively to sterile sea water drops until just the desired cell was present. Then, the cell was placed in 3 ml of medium, and after 1 month transferred to higher volume. The isolated strain is being maintained in f/2 medium (without Si stock solution) (Guillard and Ryther 1962), salinity 32–35, temperature 20 °C (±1), photoperiod of 12 h light/12 h dark, and 80 μE m−2.s−1 radiation. The strain is deposited in the Microorganisms Collection Aidar & Kutner from Oceanographic Institute, University of São Paulo (strain number BMAK193).

Morphological characterization

Cultures of 1–3 weeks old were used for morphological observations. Living and fixed cells (2% glutaraldehyde) were observed under light microcopy Leica DM 4000 B (Leica Microsystems, Wentzler, Germany), and confocal microscopy Zeiss LSM 440 Axiovent 100 (lp870/543 nm) (Carl Zeiss, Jena, Germany). For SEM and TEM, cultures were harvested by centrifugation (3 min, 100–150 g), and transferred for 90 min to a fixative solution (2% glutaraldehyde plus sodium cacodylate trihydrate 0.1 M, and sucrose 0.8 M buffer). For the SEM preparation, cells were washed in cacodylate plus-sucrose buffer, and then post-fixed in osmium tetroxide (1%) for 60 min. After that, the cells were washed again in buffer, and dehydrated in an ethanol series (70, 90, 95 and 100%). Finally, the sample was dried to critical point (Balzers CPD 030, Bal-Tec, Vaduz, Liechtenstein) and gold-coated (Balzers SCD 050) for visualization in Zeiss Sigma VP. For TEM, cells were dehydrated in an acetone series (50, 70, 95 and 100%), and after embed in Spurr resin. Lastly, thin sectioned, stained, and observed in Zeiss EM 900.

DNA extraction, amplification, sequencing and molecular phylogeny

Genomic DNA was extracted using NucleoSpin® Plant II kit (Macherey-Nagel, Düren, Germany), according to the manufactures instructions. PCRs of 18S (small ribosomal subunit), ITS 1 and 2 (internal transcribed spacers), 5.8S and partial 28S (large ribosomal subunit) rRNA were amplified with Platinum® Taq DNA polymerase kit (Invitrogen™, Carlsbad, USA) and purified with the GFX Illustra kit (GE Healthcare Life Sciences, Little Chalfont, Buckinghamshire, UK), both done in accordance with the manufactures instructions. PCRs programs and primers are available as Additional file 1. Terminator Cycle Sequencing Ready Reaction kit (Applied Biosystems™, Hammonton, NJ, USA) was used for sequencing reactions, and samples were sequenced using a 3730 DNA Analyzer (Applied Biosystems™, Hammonton, NJ, USA).

Sequences were assembled with Sequencher 4.7 software (Gene Codes Corporation, Ann Arbor, Michigan, USA), and were used to seek for other sequences in GenBank database. Thirty-four sequences were used in the matrix data (see Additional file 2). Four sequences of phylogenetically close species were used to root the tree (Pyramimonas aurea, Pseudoscourfieldia marina, and Pycnococcus provasolii). These sequences were chosen based on previous studies of Nephroselmis phylogeny (Faria et al. 2012; Faria et al. 2011; Nakayama et al. 2007; Yamaguchi et al. 2011). Introns were removed from the data. Dataset alignment was performed in AliView (Larsson 2014), using the Muscle algorithm (Edgar 2004). The appropriate evolution method was selected according to JModelTest 2.1.7 analysis (Darriba et al. 2012). Maximum likelihood (ML) phylogeny inference was performed in Garli (Bazinet et al. 2014) using 1000 bootstrap replicates (Felsenstein 1985), and two searches per run. MrBayes (Ronquist et al. 2012) was used to perform Bayesian analysis, with nodes confidence supported by posterior probability. Two runs were done consecutively, each one with 4 × 106 generations, four chains, and sampling at 100 generations. MrBayes generated 8 × 104 trees, whereas 6 × 104 were used to build the consensus tree (burn-in 2×104).





Genus Nephroselmis Stein 1878

Nephroselmis viridis Inouye, Pienaar, Suda & Chihara, 2011 (Fig. 1 and Yamaguchi et al. 2011)

Fig. 1

Nephroselmis viridis morphology by light and confocal microscopy. Scale bars represents 5 μm. a Living cell in bright field coiling the flagella around the body; b Living cell in duplication observed in bright field. c Fixed cell in phase contrast evidencing the flagella length and pyrenoid. d Chloroplast natural fluorescence evidencing the chloroplast sinus (arrow) and pyrenoid. e Chloroplast fluorescence and cell morphology showing disk-like structure (arrow). (F1) longer flagellum, (F2) shorter flagellum, (P) pyrenoid. (S) starch sheath

Fig. 2

Nephroselmis viridis morphology by electron microscopy. a SEM image showing cell surface and organic scales (Scale bar 1 μm). b TEM image of the ventral view a cell showing the right nucleus (Scale bar 1 μm). c TEM image form the right- anterior view evidencing the organellar placement (Scale bar 1 μm). d More detailed view of organellar arrangement (Scale bar 0.5 μm). (C) chloroplast, (D) disk-like structure, (F1) longer flagellum, (F2) shorter flagellum, (G) Golgi body, (M) mitochondria, (N) nucleus, (P) pyrenoid. (S) starch sheath, and (V) vacuoles


The cells decant on the flasks bottom and the color of the culture is green in exponential phase and become olive in stationary and senescent phases. Cells are flattened when observed in ventral view and almost symmetrical in lateral view, bean-shaped, ranging 5 to 7.5 μm in length and 5.5 to 9 μm width (Figs. 1 and 2). During the cellular cycle, cells enlarge becoming more rounded, and the first noticeable feature is the expansion of the pyrenoid. The cells reproduce by bisection in the longitudinal axis (Fig. 1b), and sexual reproduction was not observed. Two unequal heterodynamic flagella emerge from a frontal groove, ventrally located (Figs. 1a, c and 2a). The bigger flagellum (F1), ranged from 20 to 27 μm (3–4×), and the smaller flagellum (F2), ranged between 8.5 and 11.5 μm (1–1.5×) (Fig. 1d). The cells commonly coil both flagella around the body when resting (Fig. 1a). An unique green parietal cup-shaped chloroplast was located at cells dorsal face (Figs. 1a, c, d, e and 2c) which has an eyespot in the anterior/ventral face (not show in figures). The chloroplast has a large sinus in the ventral portion (Fig. 1d), and a big cup-shaped pyrenoid starch sheath is at the dorsal region (Figs. 1b, c and 2c). Thylakoids sheets penetrate the pyrenoid (Fig. 2c). A disc-like structure is located at the dorsal part of the cell (Figs. 1e and 2c). The nucleus is located in the right position, near the ventral face (Fig. 2b and c). A single reticulate mitochondrion (Fig. 2b) is situated in the inner part of the chloroplast cavity, and a high number of Golgi vesicles are visible (Fig. 2c and d).

Molecular phylogeny

The 18S rDNA of BMAK193 does not have introns. The sequences of ITS 1 and 2, 5.8S, and partial 28S rRNA obtained in this work were not used to infer phylogeny, due to few sequences of these markers in the Genbank for the genus and the absence for the species. In the alignment matrix of 18S rDNA, Nephroselmis viridis strains sequences are 100% identical (DNA matrix is available upon request). Maximum likelihood and Bayesian phylogenetic analysis clustered BMAK193 into Nephroselmis viridis strains (Fig. 3). It also pointed out that Nephroselmis is a monophyletic genus, and N. viridis is the sister group of the freshwater species N. olivacea.
Fig. 3

Nephroselmis maximum likelihood phylogeny tree inferred by 18S rRNA performed with 1000 bootstraps replicates in two consecutive runs. General time reversible with invariant sites (I = 0.6902) and gamma distribution rate (α = 0.6101) was the evolutionary substitution nucleotide model used (GTR + G + I, InL −5465.48501). Nodes supports are bootstrap/posterior probability. Branch width represents the node bootstrap support. Scale bar is the rate of nucleotide substitution per site


The cell measures of Nephroselmis viridis from the Atlantic Ocean, such as width and length of cell body and flagella, are exactly the same of the type described in Yamaguchi et al. (2011). Ultrastructural features observed also endorse the identification, such as the chloroplast form and location, the pyrenoid cup shaped and its starch sheath, the thylakoid sheets penetrating into the pyrenoid, the disk like structure, and the positions of the reticulate mitochondrion, nucleus, and Golgi apparatus. The shape and location of these organelles are the same as observed by Yamaguchi et al. (2011). However, the color of the cells and culture are different from the species description. The isolated strain is olive when in stationary and senescent physiological culture stage, different from the green color of the type.

The most common cell shape in Nephroselmis species is bean-shaped or semicircular, and symmetrical in anterior/posterior and right/left axis, as in N viridis (Faria et al. 2012; Faria et al. 2011; Yamaguchi et al. 2011). The cell and flagella size are overlapping in some Nephroselmis species. Another common feature widespread in this genus is coiling the flagella around the cell body when cells are resting (Faria et al. 2012; Faria et al. 2011; Suda 2003; Yamaguchi et al. 2011). For these reasons, N. viridis could be easily mistaken with N. rotunda in light microscopy investigation. Therefore, for reliable morphological identification ultrastructural information is need.

Molecular markers are more suitable for identification of species, once are less affected by erroneous or incomplete observations and morphological plasticity. The clustering of Nephroselmis viridis isolated from coastal waters of Brazil with other N. virids strains from Japan, Fiji and South Africa give a clear evidence that they are the same species. The 18S rDNA pointed out that Nephroselmis is a monophyletic genus, and N. viridis is the sister group of the freshwater species N. olivacea, as observed in previous studies (Faria et al. 2012; Faria et al. 2011; Marin and Melkonian 2010; Yamaguchi et al. 2011; Yoshii et al. 2005). The 18S rDNA of BMAK193 does not have introns, such as the strain isolated in Fiji (Fiji7). But, introns in the 18S rDNA are present in other two strains of N. viridis, NIES-486 and PS537, isolated from Japan (Yamaguchi et al. 2011).

Other species of Nephroselmis were detected in Brazilian coastal waters, such as N discoidea (Menezes and Bicudo 2008), N. minuta, (Domingos and Menezes 1998), and N. pyriformis (Bergesch et al. 2008). However, most of the studies performed in South Atlantic Ocean investigate the composition of diatoms and dinoflagellates (Garcia and Odebrecht 2012; Jardim and Cardoso 2013; Lubiana and Dias Júnior 2016, and others). Consequently, the biodiversity status is rarely updated for other groups, such as the chlorophytes.

The small cell size, the challenge of morphological identification, and the species tendency to reside in sediments makes Nephroselmis viridis detection difficult. However, the species geographic distribution ought to be worldwide, especially in tropical and temperate marine regions (Yamaguchi et al. 2011), such as coastal waters of Brazil. Therefore, using an integrate methodology with culturing, morphological description, and molecular phylogeny we contribute to the knowledge of the biodiversity of the Atlantic Ocean, presenting the first record of Nephroselmis viridis in coastal waters of Brazil.



Scanning electron microscopy


Transmission electron microscopy



We wish to thanks, André Nakasato, Willian da Silva Oliveira, and Rosario Petti for technical support. Also, Irwandro Pires and Waldir Caldeira from Electron Microscopy Laboratory of IB USP for the help with electron and confocal microscopes. Financial support was obtained from FAPESP (2010/50187-1), and CNPq scholarships to K. M. F. Lubiana (163070/2013-0), and to M.C. Oliveira (301491/2013-5).


FAPESP (2010/50 187-1), and CNPq scholarships to KMFL (163070/2013-0), and to MCO (301491/2013-5).

Availability of data and materials

The DNA sequence generated in this study are available in GENBANK repository, Reference number KU978910. The strain isolated in this study is available in Marine Microorganisms Collection Aydar & Kutner, Reference number BMAK193. The sequence data matrix are available under request to corresponding author. Other data used in this publication are available in Additional files.

Authors’ contributions

KL isolated the strain, obtained morphological and molecular data, and wrote the manuscript. SG assisted article composing. FSC did strain culturing for experiments. MCO draw the experiment, did the phylogenetic analysis, and assisted article composing. All authors read and approved the final manuscript.

Competing interests

The authors declare that they have no competing interests.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Not applicable.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

Laboratório de Algas Marinhas “Édson José de Paula”, Departamento de Botânica, Instituto de Biociências, Universidade de São Paulo
Departamento de Oceanografia Biológica, Instituto Oceanográfico, Universidade de São Paulo


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