Skip to main content

Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Growth and single cell kinetics of the loricate choanoflagellate Diaphanoeca grandis

Abstract

Choanoflagellates are common members of planktonic communities. Some have complex life histories that involve transitions between multiple cell stages. We have grown the loricate choanoflagellate Diaphanoeca grandis on the bacterium Pantoea sp. and integrated kinetic observations at the culture level and at the single cell level. The life history of D. grandis includes a cell division cycle with a number of recognisable cell stages. Mature, loricate D. grandis were immobile and settled on the bottom substratum. Daughter cells were ejected from the lorica 30 min. after cell division, became motile and glided on the bottom substratum until they assembled a lorica. Single cell kinetics could explain overall growth kinetics in D. grandis cultures. The specific growth rate was 0.72 day−1 during exponential growth while mature D. grandis produced daughter cells at a rate of 0.9 day−1. Daughter cells took about 1.2 h to mature. D. grandis was able to abandon and replace its lorica, an event that delayed daughter cell formation by more than 2 days. The frequency of daughter cell formation varied considerably among individuals and single cell kinetics demonstrated an extensive degree of heterogeneity in D. grandis cultures, also when growth appeared to be balanced.

Introduction

Diaphanoeca grandis is a marine/brackish water solitary loricate choanoflagellate with morphotypes distributed globally1. It has been observed year-round in temperate waters2,3,4 mostly suspended in the water column2 and most frequently near the coast4. Choanoflagellates are filter feeders and feed primarily on picoplankton such as smaller bacterial cells5,6,7. Along with other heterotrophic nanoflagellates these organisms play important roles in marine environments where they depress the concentration of bacteria in the water column8,9 and mediate the transfer of bacterial biomass to higher trophic levels of aquatic food webs10.

D. grandis belongs to the family Stephanoecidae and has characteristic choanoflagellate morphology (Fig. 1). The protoplast measures 4–6 μm and possesses a 9 μm long apical flagellum surrounded by a collar of approximately 50 microvilli3,11. The surrounding lorica measures approximately 16 × 28 μm and is built from approximately 120 silicate sticks (costal strips). The collar anchors the protoplast within the lorica. Part of the lorica is covered by a thin membranous veil consisting of a meshwork of microfibrils embedded in a matrix3,12. The flagellum generates a water flow through the collar where bacteria and other particles are captured (Fig. 1A). Water exits via the part of the lorica named the chimney3,13. In Stephanoecidae, the costal strips that are to be used by daughter cells to construct new lorica are synthesised by the parental protoplast prior to cell division and transported on the surface of the daughter cell when it leaves the parental lorica11,14. The specific growth rate of D. grandis3 and the related species, Stephanoeca diplocostata15 follows Monod type kinetics with suspended bacteria as the growth limiting food source. Cultivation of D. grandis have shown a maximum specific growth rate, μmax = 0.12 h−1 at 15 °C, a half-saturation constant, Kb = 2,400 bacterial cells (Pseudomonas sp.) per μL, and a maximal ingestion rate of approximately 40 Pseudomonas per h3,16.

Figure 1
figure1

Diaphanoeca grandis. (A) Wholemount (TEM), ba, bacteria; fl, flagellum; mv, microvilli collar; pr, protoplast. Fluid flow direction from lower left corner towards upper right corner. (B) Lorica with apical membranous veil (me) concealing collar and flagellum (SEM, fixed on 1 μm polycarbonate filter; hexamethyldisilazane dried). (C) (redrawn from Andersen3). Schematic drawing with flow lines (arrows) and transport of bacteria (black dots) to the microvilli collar.

The life history of D. grandis is shown in Fig. 2. The cell division cycle proceeds via a series of recognizable cell stages11. The specific growth rate will depend on the life time of each of the different cell stages. Cell division takes place within the parental lorica at intervals, τ1. Two protoplasts will then be present within the parental lorica for a period of time, τ2. Subsequently, one protoplast, named the daughter protoplast, leaves the parental lorica via the chimney (Fig. 2, Inset B) and spends a period of time, τ3 as a motile, non-loricate cell. The second protoplast, here named the mother protoplast, remains inside the parental lorica. Finally, the daughter cell spends a period of time, τ4 assembling a new lorica before it has matured. The protoplast may also leave its lorica after a time, τ5 and become motile for a period of time before it again assembles a new lorica. Microbial batch cultures often show an initial lag phase during which the cells adjust to novel conditions before growth commences. In Fig. 2, the time it takes from a cell is added with the inoculum and until it undergoes its first cell division and thereafter is recognized as a mature, loricate choanoflagellate is denoted τ0.

Figure 2
figure2

Diaphanoeca grandis life history. D. grandis added in inoculum until it has passed through first cell division, 0. Mature, loricate D. grandis, m. Dividing protoplast, d. Motile, non-loricate cell, n. Cell assembling new lorica, l. Empty lorica, e. Solid arrows indicate transitions between cell stages in the cell division cycle. Characteristic life times of different cell stages: Time until cells divide the first time, τ0. Time between cell divisions, τ1. Life time of stage with two protoplasts (mother and daughter) inside the lorica, τ2. Life time of motile, non-loricate cell stage, τ3. Time expenditure for assembly of new lorica, τ4. Dashed lines indicate protoplast abandoning its lorica and forming a motile cell that subsequently constructs a new lorica. Time span from protoplast went through its final cell division until it abandons its lorica, τ5. Inset A: Cell components of loricate D. grandis. Lorica, lo. Protoplast, pr. Collar, co. Flagellum, fl. Chimney, ch. Scale bar = 20 μm. Inset B. Dividing protoplast. Mother, mo, remains in parental lorica. Daughter, da, about to exit via the chimney, ch.

Choanoflagellates can be solitary as well as colonial and is the sister group to metazoans17. The two aloricate species, Monosiga brevicollis and Salpingoeca rosetta have been suggested as model organisms for the study of early animal evolution18,19. Both species have life histories that include several morphologically different cell stages18,20,21 and belong to the choanoflagellate order, Craspedida22. The loricate choanoflagellates belong to the second choanoflagellate order, Acanthoecida22. These may also have life histories that include more cell stages (Fig. 2) but only few studies have focussed on their growth kinetics, presumably because loricate choanoflagellates are difficult to bring into culture. A few species, including D. grandis have however been characterised from cultivation studies3,11,23. The purpose of this study is to integrate kinetic observations at the culture level with the kinetics of the different steps in the cell division cycle measured at the single cell level in order to develop a structured kinetic growth model for loricate choanoflagellates. Such an approach may deepen our understanding of the life history of D. grandis and qualify the interpretation of kinetic data from cultures of loricate choanoflagellates.

Methods and Materials

Sampling and isolation of Diaphanoeca grandis and Pantoea sp

Diaphanoeca grandis24 was isolated from a 5 L surface water sample April 10, 2016 from Mariager Fjord, Denmark (56°39′15.51″N 9°58′57.26″E) by the dilution culture method3. Serial dilution of enrichment cultures into autoclaved seawater (salinity = 10‰, temp. = 15 °C) containing wheat grains as feed for bacterial prey resulted in cultures that appeared to be free from other eukaryotic contaminants. These cultures were subsequently diluted in sterile seawater until a D. grandis concentration of approximately 1 μL−1 and transferred into a microtiter plate well (1 μL per well) containing 200 μL of sterile seawater enriched by 0.01 g L−1 of yeast extract as substrate for the bacterial population still present in the culture. After 1 week of incubation at 15 °C, each well was examined under the microscope. One isolate was selected for further studies and at 2–3 week intervals, this D. grandis isolate was transferred into new batch cultures at 15 °C in 10‰ autoclaved seawater supplemented by 0.01 g L−1 of yeast extract and named D. grandis MF2016-1. Other eukaryotes but D. grandis were not observed under the microscope.

A bacterium to be used as feed was isolated from a Diaphanoeca grandis wheat grain culture. First, the culture was diluted in sterile sea water until a bacterial concentration of 10 μL−1. Then, 20 μL was spread onto petri dishes (approximately 200 cells per petri dish) containing seawater autoclaved with 50 g L−1 of wheat grains. The medium was solidified by 10 g L−1 agar. The plates were incubated at 15 °C for 1 week, and individual bacterial colonies were isolated and transferred to sterile seawater enriched with 1 g L−1 of yeast extract. One bacterial isolate consisting of spherical or ellipsoid cells with a diameter of approximately 1 μm and a cell volume of approximately 0.7 μm3 (later identified as Pantoea sp.) grew as solitary, non-motile cells and supported growth of D. grandis. This bacterium was grown in batch cultures in an orbital shaking incubator at 15 °C until stationary phase was reached, where after the culture was harvested by centrifugation, re-suspended in sterile seawater, and used as sole prey for D. grandis cultures. This procedure minimized potential co-transfer of left-over components from the bacterial growth medium25.

Diaphanoeca grandis was identified based on its characteristic morphology combined with blastN analysis against the non-redundant database at NCBI26 after PCR amplification and partial sequencing of the silica transporter gene using the primer pair for D. grandis27. Pantoea sp. was identified by PCR amplification and partial sequencing followed by blastN analysis of the 16 S rDNA gene using the primer pair 27 F/1492 R for Pantooea sp.28. Experimental details were as described by Tophøj et al.25.

Population growth and grazing in batch cultures of Diaphanoeca grandis

Prior to growth and grazing experiments, Diaphanoeca grandis inocula were precultured on Pantoea sp. and 1–2 mL of these precultures were used to inoculate new D. grandis cultures at cell concentrations of 2–10 μL−1 in 50 mL of sterile seawater. Pantoea sp. was added at cell concentrations of 4,000–26,000 μL−1 as the sole feed. In addition were 50–100 unidentified bacteria μL−1 carried over with the inocula since 1,000–2,000 bacteria μL−1 remained in the precultures. The D. grandis cultures were grown in 100 mL conical glass flasks incubated at 15 °C with no stirring. Only when samples were taken 1–2 times per day, cultures were gently shaken to form a homogeneous suspension. Attempts were also made to grow D. grandis in suspension cultures stirred by an orbital shaker, a planktonic wheel, or by gentle sparging.

D. grandis and Pantoea sp. were simultaneously counted by flow cytometry in samples taken from the cultures. Cells were stained by addition of 1 μL acridine orange (Sigma-Aldrich) solution (1 mg L−1) to 1 mL of culture sample. After 5 min of incubation, cells were counted on a Cyflow Space flow cytometer (Sysmex Partec, Germany) equipped with a 480 nm blue laser. Concentrations of D. grandis, cf and Pantoea sp., cb were calculated from absolute counts of particles in 0.7 mL sample volume giving rise to simultaneous forward scatter, side scatter, and green fluorescence signals. D. grandis concentrations were also determined from microscopically counts in a 0.0025 mm3 hemocytometer (Thoma, Germany).

To identify the range of bacterial concentrations where D. grandis grow optimally, the specific growth rate, μ as function of bacterial concentration cb, was described by

$$\mu ={\mu }_{{\max }}(\frac{{c}_{b}}{{K}_{b}+{c}_{b}})(1-\frac{1}{1+{e}^{(E{C}_{50}-{c}_{b})\cdot H}})$$
(1)

that combines the Monod model with a sigmoidal dose-response curve (supersaturating bacterial concentrations may reduce the filtration rate of D. grandis3 and potentially also affect growth), where μmax is the maximal specific growth rate and Kb is a half-saturation constant. EC50 is the effective bacterial concentration at which the specific growth rate is reduced to half its maximal value. The coefficient H defines the steepness of the slope of the curve (additional details in Supplementary Information).

Single cell growth kinetics

Growth of Diaphanoeca grandis was also monitored at the single-cell level in the oCelloScope optical detection system (Biosense Solutions Aps, Denmark), which is an automatic digital microscope equipped with a 4x optical magnification (200x effective magnification)29,30. In the oCelloScope, D. grandis was grown in NUNCTM Edge 96-well plates (Thermo Scientific, USA) containing 200 μL of sterilised seawater (salinity = 10‰, temp. = 15 °C) and with Pantoea sp. as sole prey. To minimize evaporation, 8 mL of water was added to the surrounding plate-reservoir. D. grandis inocula and Pantoea sp. used as feed had been treated as described above, before being loaded into the microtiter plate (5 D. grandis μL−1 and 3,000–12,000 Pantoea sp. μL−1). After 1 hour of incubation to allow for sedimentation, focus and light intensity were manually adjusted for each well. Each scan at 1 min. interval (6 days total incubation) consisted of 15 separate raw images (with an image distance of 11.44 µM) and from these in-focus planes were automatically concatenated to form a series of images covering a 1,300 μm × 1,200 μm area. To preserve image quality, each frame was manually exported and subsequently imported into Fiji ImageJ ver. 2.0.0. The image stacks could be viewed as a film and allowed continuous surveillance of individual D. grandis for up to 6 days with recordings of several consecutive cell division cycles. From the image stacks, the characteristic life time, τ0 - τ5 of the different cell stages of individual D. grandis (Fig. 2) were determined.

The cell division cycle of D. grandis depicted in Fig. 2 was translated into a structured kinetic growth model, describing the number of cells, N in batch cultures of D. grandis

$$\frac{d{N}_{0}}{dt}=-\,{k}_{0}{N}_{0}$$
(2)
$$\frac{d{N}_{m}}{dt}={k}_{0}{N}_{0}+{k}_{4}{N}_{l}$$
(3)
$$\frac{d{N}_{d}}{dt}={k}_{0}{N}_{0}+{k}_{1}\frac{{c}_{b}}{{K}_{b}+{c}_{b}}{N}_{m}-{k}_{2}{N}_{d}$$
(4)
$$\frac{d{N}_{n}}{dt}={k}_{2}{N}_{d}-{k}_{3}{N}_{n}$$
(5)
$$\frac{d{N}_{l}}{dt}={k}_{3}{N}_{n}-{k}_{4}{N}_{l}$$
(6)

where numbers of each recognisable cell stage are denoted the following way; N0, loricate D. grandis inoculated into the culture that have not yet gone through a cell division. Nm, mature, loricate D. grandis. Nd, parental lorica with two protoplasts inside. Nn, motile, non-loricate cell. Nl, cell being in the process of assembling a lorica. Each term in Eqs. 26 represent a transition between cell stages, represented by a solid arrow in Fig. 2. Each rate constant, k0, k1, k2, k3, and k4 correspond to the inverse value of the characteristic life time of the particular cell stage in the cell division cycle, τ0−1, τ1−1, τ2−1, τ3−1, and τ4−1 (Fig. 2), respectively. If bacterial concentrations, cb are well below EC50, the rate of daughter cell formation is assumed to follow Monod type kinetics3 and the rate constant, k1 must therefore be determined during the exponential growth phase.

Equations 26 can be modified to describe temporal changes in the concentration of D. grandis if cell numbers are divided by the culture volume. If the bacterial prey does not grow and growth of D. grandis is balanced, the bacterial concentration, cb will decrease at rates described by

$$\frac{d{c}_{b}}{dt}=\frac{1}{{Y}_{f/b}\cdot V}\cdot \frac{dN}{dt}={Y}_{f/b}^{-1}\cdot \frac{d{c}_{f}}{dt}$$
(7)

where Yf/b is the yield of flagellate cells (D. grandis) feasting on bacterial prey, V is culture volume, and cf is the concentration of flagellate cells (D. grandis). The ingestion rate, I can be estimated as

$$I={Y}_{f/b}^{-1}\cdot \mu $$
(8)

Linking single cell growth kinetics to population growth

Concentrations of D. grandis and Pantoea sp. in 50 mL batch cultures were simulated by the growth model, Eqs. 27 while the rate constants were obtained from examination of single cells in 200 μL cultures. The individual equations in the model were solved numerically using Euler’s solution at time intervals, Δt = 0.2 h, starting at t = 24–36 h (corresponding to the length of lag phases), as shown in Supplementary Information, Eqs S4S9.

Results

Growth of Diaphanoeca grandis in batch culture

Diaphanoeca grandis from Mariager Fjord was recognized from the size and shape of the lorica (Figs 1 and 2). SEM images furthermore disclosed the presence of the apical membranous veil (Fig. 1B), and the silica transporter gene (Genbank ID MN369736) showed 98% sequence identity to GenBank ID HE981738.1, Diaphanoeca grandis. The isolate was grown in batch culture using Pantoea sp. (the 16 S rDNA sequence, Genbank ID MN250297 showed 99.7% sequence identity to GenBank ID KX891536.1, Pantoea eucalypti) as the sole prey. All attempts to grow D. grandis in stirred suspension cultures were unsuccessful. D. grandis was therefore grown in non-stirred batch cultures on initial Pantoea sp. concentrations of 4,000–26,000 μL−1. D. grandis, counted by flow cytometry after resuspension of the cells, grew to maximal concentrations of approximately 200 μL−1. Growth was always accompanied by a decrease in the concentration of bacteria (Fig. 3A and Supplementary Information, Fig. S2). During the exponential growth phase, the average yield of D. grandis per bacterium, Yf/b = 0.014 ± 0.001 (n = 27), meaning the production of one D. grandis occurred at the expense of Yf/b−1 = 74 ± 7 Pantoea sp. (Fig. 3B). Addition of sodium metasilicate to the seawater did not affect final concentrations of D. grandis. Length, diameter and volume of the protoplasts were 4.9 ± 0.7 μm, 3.9 ± 0.7 μm, and 60 ± 28 μm3, n = 259, respectively. There were considerable variability between individuals and the average protoplast volume decreased from an initial average of 95 μm3 to 44 μm3 as batch cultures progressed (Supplementary Information, Fig. S3).

Figure 3
figure3

Diaphanoeca grandis. Two replicate batch cultures grown on Pantoea sp. (A). Concentrations of D. grandis, cf (, ■) and bacterial prey Pantoea sp., cb (, □). (B). Increase in concentration of D. grandis vs. decrease in concentration of Pantoea sp. Slopes of regression lines correspond to the yield of choanoflagellates (D. grandis) per bacterium, Yf/b. (C). ln(cD. grandis) vs. time, exponential growth phase indicated by solid symbols, slope of regression line equals specific growth rates. (D). Specific growth rates, µ () of 34 D. grandis cultures grown on initial Pantoea sp. concentrations of 4,000–26,000 μL−1. Solid line shows best fit of Eq. 1, μmax = 0.9 day−1, Kb = 2,400 μL−1, EC50 = 19,000 μL−1, H = 0.46. Dotted line shows the Monod model (Supplementary Information, Eq. S1), μmax = 0.9 day−1, Kb = 2,400 μL−1. Dashed line shows fit of a dose-response curve (Supplementary Information, Eq. S2), μmax = 0.9 day−1, EC50 = 19,000 μL−1, H = 0.46. Reciprocal yields, Yf/b1, corresponding to the number of Pantoea sp. consumed per D. grandis produced during exponential growth phase ().

Specific growth rates were determined taking into account the initial lag phase of D. grandis (Fig. 3C). Figure 3D shows specific growth rates measured in 30 D. grandis cultures grown on Pantoea sp. The maximal specific growth rate estimated according to the Monod model (Supplementary Information, Eq. S1), μmax = 0.72 ± 0.10 day−1 (n = 24) was observed in cultures with initial Pantoea sp. concentrations of 4,000–15,000 μL−1. At higher initial Pantoea sp. concentrations, specific growth rate decreased. Best fit of a dose-response curve (Supplementary Information, Eq. S2) to the measured specific growth rates indicated that EC50 ≈ 19,000 bacterial cells per μL. The initial bacterial concentrations, cb,0 were used as rough estimates of the actual bacterial concentrations in the cultures, cb. Figure 3D also shows the best fit of Eq. 1 to the measured specific growth rates, using Kb = 2,400 bacteria per μL3. During exponential growth phases, the average ingestion rate was 53 Pantoea sp. day−1 (Eq. 8).

Qualitative observations on individual Diaphanoeca grandis

When Diaphanoeca grandis was grown in 96-well plates, individuals were continuously observed in the oCelloScope for periods of up to 6 days. D. grandis settled on the bottom of the wells within 2–3 h. Loricate cells, resting on the bottom, were immobile. All D. grandis present in the filmed area on Day 0 could therefore be followed until the experiment was terminated on Day 6 (Supplementary Information, Figs. S4-S5). Protoplast and lorica were visible in all individuals. In a few individuals, also the beating flagellum could be seen. The elongated cytoplasmic strand used to move daughter cells out of the parental lorica14 was occasionally visible during the cell separation phase (Supplementary Information, Figs. S8 and S11 and Supplementary Video S1). Most D. grandis settled with their longitudinal axis in parallel to the bottom substratum (Supplementary Information, Fig. S6A). Daughter cells were motile until they began to assemble their lorica. They did not swim but glided along the bottom of the well (Supplementary Information, Figs. S6B and S13) with maximal velocities of 60–70 μm min−1 (Supplementary Information, Fig. S9). Daughter cells therefore remained within the optical focus range of the oCelloScope. Some daughter cells did, however, move out of the filmed area before they settled, while others came into and settled within the filmed area. The elongated cytoplasmic strand did not always break and the daughter cell then settled in close proximity of its parental lorica (Supplementary Information, Fig. S9 and Supplementary Video S1). We also observed that D. grandis occasionally abandoned their lorica without going through a cell division (Supplementary Information, Fig. S11 and Supplementary Video S2). Protoplasts then became temporarily motile until they again settled and formed new lorica and resumed daughter cell formation. The resolution of the oCelloScope was insufficient to quantify the bacterial cells in the wells, and it was not clear to which extent also bacteria settled on the bottom of the wells.

Single cell growth kinetics

Three Diaphanoeca grandis cultures were followed in the oCelloScope for a period of 6 days (Fig. 4), generating 1.9 Terabytes of image-data. Between 129 and 157 individual D. grandis settled on the bottom of the wells within the filmed area. After 16–20 h, the number of D. grandis started to increase in the cultures grown on initial Pantoea sp. concentrations of 3,000 and 6,000 μL−1. In the third culture where the initial Pantoea sp. concentration was 12,000 μL−1, the lag phase lasted approximately 92 h. The number of D. grandis increased 3.6–9.6 times, corresponding to 1.8–3.3 cell divisions (Supplementary Information, Table S1). Specific growth rates during exponential growth phases reached values of 0.49–0.66 day−1.

Figure 4
figure4

Diaphanoeca grandis. Number of individuals in filmed area in oCelloScope, grown on 3,000 (), 6,000 () and 12,000 (□) Pantoea sp. μL−1. Inset. ln(D. grandis numbers) vs. time, exponential growth phase indicated by solid symbols, slope of regression line equals specific growth rates, µ (Supplementary Information, Table S1).

Figure 5 shows a number of observations made on cohorts of 38–40 parental Diaphanoeca grandis inoculated into the 3 cultures shown in Fig. 4. These individuals represented 24–31% of the total number of D. grandis that originally had settled within the filmed area. All individuals in the 3 cohorts were followed for 6 days and all individual life history events shown in Fig. 2 were recorded. There was considerable variation within each culture with respect to the point in time when each parental D. grandis produced its first daughter cell. The lower the initial Pantoea sp. concentration was, the earlier did daughter cell formation begin (Fig. 5A,E,I). Between 1 and 5 parental D. grandis did not produce daughter cells within the 6 days of the experiment (Fig. 5B,F,J). Most of these individuals maintained the same physical appearance as the active ones. Only 2 individuals in the culture grown at the lowest of the Pantoea sp. concentrations (Fig. 5B) lost their normal appearance and presumably died.

Figure 5
figure5

Diaphanoeca grandis. Data on cohorts of individuals inoculated and filmed in the oCelloScope and grown on 3,000 (38 individuals, AD), 6,000 (40 individuals, EH) and 12,000 (40 individuals, IL) Pantoea sp. μL−1. A, E and I. Number of cell divisions within 12 h time intervals. Solid bars indicate first release of a daughter cell, open bars indicate release of subsequent daughter cells. B, F and J. Number of inoculated D. grandis that have not yet carried out a cell division. C, G and K. Time span between cell divisions, excluding the first cell division (), τ1 and time span between replacement of a lorica and the following cell division (). D, H and L. Number of protoplasts leaving and replacing their lorica within 12 h time intervals.

Most of the parental D. grandis in the cohorts produced several daughter cells (Fig. 5A,E,I), so each individual ended up producing 1–5 daughter cells in total (Supplementary Information, Fig. S10). On average, 2.1–2.7 daughter cells were produced by each of the parental D. grandis. The cultures inoculated into 3,000 and 6,000 Pantoea sp. μL−1 grew beyond the exponential growth phase (Fig. 4). In these 2 cultures, the rate of daughter cell formation reached a maximum of 15–18 daughter cells every 12 h for periods of time lasting 0.5 and 2 days, respectively. The time span between individual cell divisions, τ1 showed considerable variation (16–69 h) while the average value remained at the same level (26 ± 8 h) until the end of the experiment (Fig. 5C,G,K, and Table 1). In the cultures inoculated into 3,000 or 6,000 Pantoea sp. μL−1, it was therefore a decrease in the fraction of actively dividing individuals that resulted in the apparent decrease of specific growth rate after 80–90 h, rather than a decrease in the activity of all individuals in the cultures.

Table 1 Diaphanoeca grandis. Characteristic life times (average values ± standard deviation) of individual cell stages from 3 cultures grown in the oCelloScope on Pantoea sp. (Figs 5 and 6). Time span between cell divisions, τ1. Life time of stage with two cells (mother and daughter) inside the parental lorica, τ2. Life time of motile, non-loricate cell stage, τ3. Time expenditure for assembly of new lorica, τ4. Time span since last cell division when a protoplast abandons its lorica, τ5. Number of events, n.

We also observed parental protoplasts abandoning their lorica (Fig. 5D,H,L and Supplementary Information, Fig. S11). These events began earlier in the culture inoculated into 3,000 Pantoea sp. μL−1 than in the culture inoculate into 6,000 Pantoea sp. μL−1 while none of the protoplasts abandoned their lorica in the culture inoculated into 12,000 Pantoea sp. μL−1. Before a protoplast abandoned its lorica, it had not produced a daughter cell for a period, τ5 of 59 ± 19 h (Table 1). After they had constructed a new lorica, daughter cell formation resumed after 21 ± 5 h, n = 12, a period of time quit similar to the characteristic time span between cell divisions, τ1 (Fig. 5C,G). When a protoplast abandoned its lorica, the formation of daughter cells was thereby delayed by more than 2 days.

Figure 6 shows characteristic life times of the 3 distinguishable cell stages that follow a cell division in D. grandis (Fig. 2). The stage where two protoplasts (mother and daughter) reside inside the lorica after a cell division, τ2, lasted 0.29 ± 0.10 h (Table 1). The motile, non-loricate cell stage, τ3, lasted 0.64 ± 0.32 h, and finally the daughter cells used 0.29 ± 0.09 h to assemble their new lorica, τ4. All in all, daughter cells spend about 1.2 h to transform into mature, loricate choanoflagellates. The characteristic life times, τ2, and τ4, showed only little variation. Only on a few occasions did a daughter cell stay inside the parental lorica either considerably longer or shorter than the average value. Larger variations were observed in the lifetime of the motile, non-loricate daughter cells, τ3, and there may have been a weak tendency for motile, non-loricate daughter cells to exist for shorter periods of time during the late phases of the cultures.

Figure 6
figure6

Diaphanoeca grandis. Data on cohorts of individual D. grandis inoculated and filmed in the oCelloScope and grown on 3,000 (38 individuals, AC), 6,000 (40 individuals, DF) and 12,000 (40 individuals, GI) Pantoea sp. μL−1. A, D and G. Life time of stage with two cells (mother and daughter) inside the parental lorica, τ2. B, E and H. Life time of motile, non-loricate cell stage, τ3. C, F and I. Time expenditure for assembly of new lorica, τ4. Open symbols indicate events following cell divisions. Closed symbols indicate events that occurred after a protoplast had abandoned its lorica.

Linking growth kinetics at the culture and at the single cell level

In order to test if the observations made on individual D. grandis observed in the oCelloScope would be able to explain the progression of cultures grown at larger scale, we carried out a series of 50 mL batch cultures where D. grandis was grown on 8 different initial Pantoea sp. concentrations between 4,500 and 12,000 μL−1. At each Pantoea sp. concentration, 3 replicate cultures were carried out. The Pantoea sp. concentrations were selected within the range where the specific growth rate was maximal (Fig. 3D). Concentrations of D. grandis and Pantoea sp. were quantified daily and compared to concentrations predicted by Eqs. 27 (cell numbers were divided by culture volume to predict cell concentrations), while the rate constants, k0 - k4 were based upon single cell kinetics (Table 1). In all cultures, the predicted concentrations of D. grandis as well as Pantoea sp. were well in line with experimentally determined cell concentrations (Fig. 7). Predicted concentrations of the individual cell stages can be seen in Supplementary Information, Fig. S1. The mature, loricate cell stage was always dominating because the other cell stages were comparatively short lived (Table 1).

Figure 7
figure7

Diaphanoeca grandis. Batch cultures grown on Pantoea sp. at initial concentrations of 4,500 (A), 5,000 (B), 5,500 (C), 7,000 (D), 9,000 (E), 9,500 (F), 12,000 (G) and 13,000 (H) Pantoea sp. μL-1. Concentrations of D. grandis, cf () and bacterial prey Pantoea sp., cb (). All data points are average measurements from 3 replicate cultures ± standard error. Curves show the concentrations of D. grandis and bacteria modelled by Eqs. 27, using the characteristic life time of the different cell stages listed in Table 1.

Discussion

Diaphanoeca grandis grew in batch cultures on Pantoea sp. as its sole prey. The immobility of loricate D. grandis and the close association to the bottom substratum of all cell stages made D. grandis an ideal candidate to be examined in the oCelloScope. Growth kinetics observed in 200 μL cultures analysed at the individual cell level in the oCelloScope (Figs 46) was in agreement with kinetics observed in 50 mL cultures analysed at the culture level by flow cytometry (Fig. 7), indicating that D. grandis behaved similarly in both culture types. These analyses provided novel insights into the life history of D. grandis with relevance to our understanding of the role of D. grandis in the environment. The analyses also demonstrated an unforeseen high degree of heterogeneity within the cultures.

D. grandis is a common member of marine planktonic communities1,2,4. Loricate D. grandis have been described as slow swimmers3 but can also be found attached to detritus31. The isolate used in this study was isolated from the water column, albeit sampled at shallow waters at a coastal location. All observations in the laboratory seemed, however, to contradict that D. grandis should have a planktonic life style. All attempts to grow D. grandis in stirred suspension cultures failed, irrespectively of stirring method and long term observations on individual cells showed that loricate D. grandis are immobile and reside on the bottom substratum. Individuals remained at the same position for the experimental period of 6 days, except when protoplasts abandoned their lorica and temporarily became motile. Cells were, in most cases, motile for less than one hour (Fig. 6B,E,H). Since the elongated cytoplasmic strand, used to push out daughter cells from the parental lorica14, did not always break and daughter cells then settled in proximity of their parental lorica (Supplementary Information, Fig. S9), individual D. grandis did not distribute themselves homogeneously at the bottom surface of the 96-well plates, in where they were grown. Some tended to form smaller groups of up to 10–20 individuals (Supplementary Information, Figs S4-S5). Also when the elongated cytoplasmic strand did break, and the daughter cell became fully motile, they did not swim but glided on the bottom substratum. Sediments and other surfaces such as e.g. marine snow may therefore be important and somewhat overlooked habitats for D. grandis.

D. grandis was not attached to the bottom substratum and its lorica is also without a stalk, which secures other Diaphanoeca species a fixed orientation perpendicularly to the substratum22. Occasionally we observed that motile, non-loricate daughter cells collided with mature lorica, which were then either pushed or rolled slightly out of the way (Supplementary Information, Fig. S13). It may therefore be that D. grandis is easily brought temporarily into suspension in turbulent waters where it can then be found in the water column, often near the coast1,2,4. Several fluid flow models have been used to predict magnitude and direction of fluid flows generated by D. grandis and other choanoflagellates that are either freely suspended in the water column13,32 or anteriorly attached to a solid substratum with their longitudinal axis oriented perpendicularly to the surface32,33. Most D. grandis settled with their longitudinal axis in parallel to the bottom substratum (Supplementary Information, Fig. S6), and therefore in a different orientation than normally expected for a choanoflagellate.

We were able to grow D. grandis successfully only in non-stirred cultures, mixed only before samples were collected once or twice per day. In between, D. grandis concentrated on the bottom of the culture flasks. Inhomogeneous distribution of cells may therefore have influenced kinetic and stoichiometric characteristics. Ingestion rate (53 Pantoea sp. day−1) and specific growth rate (0.72 day−1) were low compared to the maximal rates (40 Pseudomonas h−1 and 0.12 h−1 (2.88 day−1), respectively, observed before in D. grandis3. In Stephanoeca diplocostata, a second loricate choanoflagellate, the maximal specific growth rate was 1.9 day−1, but at bacterial concentrations of 100,000 per μL15, which is 5 times higher than the bacterial concentrations tolerated by D. grandis without negative effects on growth (Fig. 3D). The cell cycle also proceeds at a slightly faster rate in S. diplocostata, in which species the total time from a protoplast visibly starts to divide until the daughter cell is released has been measured to 12 min (Leadbeater 1976) as compared to 0,29 h (17 min) in D. grandis (Table 1). The average protoplast volume of 60 ± 28 μm3 was, however, close to earlier estimates in D. grandis (70–83 μm3)3,13 but covered at wide span from 15–160 μm3 (Supplementary Information Fig. S3). The average protoplast size of D. grandis decreased considerably during batch cultivation. D. grandis may therefore need more than 74 Pantoea sp. to produce one daughter cell (Fig. 3B) during steady state situations where the cell size is preserved.

Analyses on individual cells furthermore revealed that balanced growth in batch cultures of D. grandis was not necessarily obtained although specific growth rates and growth yields measured at the culture level reached constant values. Balanced growth is, however, a common presumption in models used for determination of specific rates of e.g. growth and food uptake in growing microbial cultures25,34. D. grandis could be grown only at a narrow range of bacterial prey concentrations that either did not limit or inhibit growth (Fig. 3D). Cultures inoculated at 2–10 D. grandis μL−1 and 5,000–12,000 Pantoea sp. μL−1 completed 3–6 generations. Cell counts indicated that growth was exponential (Fig. 3B), and yields became constant after a lag phase (Fig. 3C). Still, analyses of individual cells displayed substantial heterogeneity. Figure 4 indicates that D. grandis cultures grown at initial Pantoea sp. concentrations of 3,000 or 6,000 μL−1 entered the exponential growth phase in less than 24 h. Some of the parental D. grandis did, however, not produce their first daughter cell until after 48–72 h (Fig. 5B,F). Also the time span between consecutive releases of daughter cells, τ1 was variable, ranging from 16–69 h (Fig. 5C,G,K). There were therefore parental D. grandis that produced 2 or 3 daughter cells, and there were daughter cells that matured and began to divide, before the last of the parental D. grandis produced their first daughter cell. This led to a large degree of heterogeneity also in the productivity among the parental D. grandis (Supplementary Information, Fig. S10).

Although the time span between releases of daughter cells showed considerable variability, τ1 seemed not to be a function of time within the 6 days the cultures were monitored (Fig. 5C,G,K). The decrease in the rate of daughter cell formation, which occurred after 60–84 h at 3,000 and 6,000 Pantoea sp. μL−1 (Fig. 5A,E), and the subsequent decrease in specific growth rate (Fig. 3, inset) was rather a consequence of protoplasts abandoning and replacing their lorica (Fig. 5D,H). Before protoplasts replaced their lorica, they experienced a more than 2-day break in the formation of new daughter cells. Protoplasts began to replace their lorica earlier when grown on 3,000 Pantoea sp. μL−1 than on 6,000 Pantoea sp. μL−1 and more than half of the D. grandis initially inoculated into the cultures ended up replacing their lorica in these two cultures. This behaviour was not observed in the culture grown on 12,000 Pantoea sp. μL−1, which did not grow beyond the exponential growth phase before it was terminated. Protoplasts did not differ in appearance or motion pattern (Supplementary Information, Figs. S11 and S12) from the motile, non-loricate daughter cells. It could be observed that they are carrying costal strips (Supplementary Information, Fig. S11) as also daughter cells do11,14. Naked Stephanoeca diplocostata, deprived of their lorica, is able to resynthesize a new lorica35 and this could potentially have been a possibility also in D. grandis. The abandoning protoplasts resembled the daughter cells also with respect to size, shape, and motion pattern (Supplementary Information, Figs. S7-S9 and S11-S12). Some protoplasts stayed active within the same lorica during the entire experimental period, showing that the lifetime of a functional lorica exceeds 6 days, although silica may continuously dissolve from the costal strips, limiting the lifetime of a lorica36.

Figure 5 shows that lorica replacements can be frequent events in D. grandis and may be associated to prey availability. Protoplasts did, however, most likely start to replace their lorica before Pantoea sp. was depleted from the cultures since they managed to resume daughter cell formation after they had reconstructed a new lorica (Fig. 5C,G). What actually triggered protoplasts to abandon and replace their lorica remain unresolved, why this phenomenon was not incorporated in the growth model (Eqs. 27). Monod kinetics (Supplementary Information, Eq. S1) describes the transient decrease in specific growth rate, which takes place when batch cultures progress from exponential to stationary phase due to food limitation and the time span between cell divisions is prolonged for all cells in a culture. In D. grandis cultures, this interpretation is too simplistic since the specific growth rate is also affected when protoplasts abandon and replace their lorica. It has, to our knowledge, not previously been described that D. grandis can replace its lorica but this may provide D. grandis an opportunity to temporarily regain motility and move to new and potentially better positions.

More than 115 species of loricate choanoflagellates have been identified based on morphology, and from more than 20 species are also sequence data available37. Growth, feeding, and life history have been described in only a few of these. In this study, we have linked single cell growth kinetics to growth kinetics at the culture level in D. grandis. The structured growth model (Eqs. 27) provides a more detailed and comprehensive interpretation of growth kinetics in D. grandis than the Monod model3. The characteristic time span between cell divisions, τ1 was much longer than the characteristic life times, τ2 - τ4 associated with the different daughter cell stages (Table 1), meaning that the maximum specific growth rate of D. grandis is mainly controlled by the frequency by which mature individuals form new daughter cells, k1. When protoplasts abandoned and replaced their lorica, daughter cell formation slowed down considerably, and the event represents a substantial investment in time, indicating that the ability to regain motility and obtain the opportunity to move to a new location is of importance to D. grandis. The combination of analyses at the culture level and at the individual cell level furthermore demonstrated an extensive degree of heterogeneity in D. grandis cultures, even during exponential growth phases. Individual cell performances may therefore not necessarily be well represented by kinetic data representing the average performances of all cells in cultures of D. grandis and possibly also other microorganisms.

Data Availability

The datasets generated during and/or analysed during the current study are available from the corresponding author on reasonable request.

References

  1. 1.

    Nitsche, F. & Arndt, H. Comparison of similar arctic and Antarctic morphotypes of heterotrophic protists regarding their genotypes and ecotypes. Protist 166, 42–57 (2015).

    Article  Google Scholar 

  2. 2.

    Andersen, P. & Sørensen, H. M. Population dynamics and trophic coupling in pelagic microorganism in eutrophic coastal waters. Mar. Ecol. Prog. Ser. 33, 99–109 (1986).

    ADS  Article  Google Scholar 

  3. 3.

    Andersen, P. Functional biology of the choanoflagellate Diaphanoeca grandis Ellis. Mar. Microb. Food Webs 3, 35–50 (1988/1989).

  4. 4.

    Thomsen, H. A., Nitsche, F. & Richter, D. J. Seasonal occurrence of loricate choanoflagellates in Danish inner waters. Protist 167, 622–638 (2016).

    Article  Google Scholar 

  5. 5.

    Gonzalez, J. M., Sherr, E. B. & Sherr, B. G. Size-selective grazing on bacteria by natural assemblages of estuarine flagellates and ciliates. Appl. Environ. Microbiol. 56, 583–589 (1990).

    CAS  PubMed  PubMed Central  Google Scholar 

  6. 6.

    González, J. M. Efficient size-selective bacterivory by phagotrophic nanoflagellates in aquatic ecosystems. Mar. Biol. 126, 785–789 (1996).

    Article  Google Scholar 

  7. 7.

    Boenigk, J. & Arndt, H. Comparative studies on the feeding behavior of two heterotrophic nanoflagellates: the filterfeeding choanoflagellate Monosiga ovata and the raptorial-feeding kinetoplastid Rhynchomonas nasuta. Mar. Ecol. Prog. Ser. 22, 243–249 (2000).

    Google Scholar 

  8. 8.

    Fenchel, T. Ecology of heterotrophic microflagellates. IV. Quantitative occurrence and importance as bacterial consumers. Mar. Ecol. Prog. Ser. 9, 35–42 (1982).

    ADS  Article  Google Scholar 

  9. 9.

    Massana, R. & Jürgens, K. Composition and population dynamics of planktonic bacteria and bacterivorous flagellates in seawater chemostat cultures. Aquat. Microb. Ecol. 32, 11–22 (2003).

    Article  Google Scholar 

  10. 10.

    Azam, F. et al. The ecological role of water-column microbes in the sea. Mar. Ecol. Prog. Ser. 10, 257–263 (1983).

    ADS  Article  Google Scholar 

  11. 11.

    Leadbeater, B. S. C. & Cheng, R. Costal strip production and lorica assembly in the large tectiform choanoflagellate Diaphanoeca grandis Ellis. Eur. J. Protist. 46, 96–110 (2010).

    Article  Google Scholar 

  12. 12.

    Leadbeater B. S. C. The choanoflagellates. Evolution, biology and ecology (Cambridge University Press, 2015).

  13. 13.

    Nielsen, L. T. et al. Hydrodynamics of microbial filter feeding. Proc. Natl. Acad. Sci. 114, 9373–9378 (2017).

    ADS  CAS  Article  Google Scholar 

  14. 14.

    Leadbeater, B. S. C. Developmental studies on the loricate choanoflagellate Stephanoeca dipIocostata Ellis. II. Cell division and lorica assembly. Protoplasma 98, 311–328 (1979).

    Article  Google Scholar 

  15. 15.

    Geider, R. J. & Leadbeater, B. S. C. Kinetics and energetics of growth of the marine choanoflagellate Stephanoeca diplocostata. Mar. Ecol. Prog. Ser. 47, 169–177 (1988).

    ADS  Article  Google Scholar 

  16. 16.

    Marchant, H. J. & Scott, F. J. Uptake of sub-micrometre particles and dissolved organic material by Antarctic choanoflagellates. Mar. Ecol. Prog. Ser. 92, 59–64 (1993).

    ADS  Article  Google Scholar 

  17. 17.

    Carr, M., Leadbeater, B. S. C., Hassan, R., Nelson, M. & Baldauf, S. L. Molecular phylogeny of choanoflagellates, the sister group to Metazoa. Proc. Natl. Acad. Sci. 105, 16641–16646 (2008).

    ADS  CAS  Article  Google Scholar 

  18. 18.

    Hoffmeyer, T. T. & Burkhardt, P. Choanoflagellate models - Monosiga brevicollis and Salpingoeca rosetta. Curr. Opin. Gen. Develop. 39, 42–47 (2016).

    CAS  Article  Google Scholar 

  19. 19.

    Sebé-Pedrós, A., Degnan, B. M. & Ruiz-Trillo, I. The origin of Metazoa: a unicellular perspective. Nature Rev. Gen. 18, 498–512 (2017).

    Article  Google Scholar 

  20. 20.

    King, N. et al. The genome of the choanoflagellate Monosiga brevicollis and the origin of metazoans. Nature 451, 783–788 (2008).

    ADS  CAS  Article  Google Scholar 

  21. 21.

    Dayel, M. A. et al. Cell differentiation and morphogenesis in the colony-forming choanoflagellate Salpingoeca rosetta. Dev. Biol. 357, 73–82 (2011).

    CAS  PubMed  PubMed Central  Google Scholar 

  22. 22.

    Nitsche, F., Carr, M., Arndt, H. & Leadbeater, B. S. C. Higher level taxonomy and molecular phylogenetics of the Choanoflagellatea. J. Eukaryot. Microbiol. 58, 452–462 (2011).

    Article  Google Scholar 

  23. 23.

    Marchant, H. J. Grazing rate and particle size selection by the choanoflagellate Diaphanoeca grandis from the sea-ice of Lagoon Saroma Ko, Hokkaido. Proc. NIPR Symp. Polar Biol. 3, 1–7 (1990).

    Google Scholar 

  24. 24.

    Ellis, W. N. Recent researches on the Choanoflagellata (Craspedomonadines) (freshwater and marine) with description of new genera and species. Ann. Soc. R. Zoo. Belgium 60, 49–88 (1930).

    Google Scholar 

  25. 25.

    Tophøj, J., Wollenberg, R. D., Sondergaard, T. E. & Eriksen, N. T. Feeding and growth of the marine heterotrophic nanoflagellates, Procryptobia sorokini and Paraphysomonas imperforata on a bacterium, Pseudoalteromonas sp. with an inducible defence against grazing. PLoS ONE 13, e0195935 (2018).

    Article  Google Scholar 

  26. 26.

    Altschul, S. F., Gish, W., Miller, W., Myers, E. W. & Lipman, D. J. Basic local alignment search tool. J. Mol. Biol. 215, 403–410 (1990).

    CAS  Article  Google Scholar 

  27. 27.

    Marron, A. O. et al. A family of diatom-like silicon transporters in the siliceous loricate choanoflagellates. Proc R Soc B 280, 20122543 (2013).

    Article  Google Scholar 

  28. 28.

    Frank, J. A. et al. Critical evaluation of two primers commonly used for amplification of bacterial 16S rRNA genes. Appl. Environ. Microbiol. 74, 2461–2470 (2008).

    CAS  Article  Google Scholar 

  29. 29.

    Fredborg, M. et al. Real-time optical antimicrobial susceptibility testing. J. Clin. Microbiol. 51, 2047–2053 (2013).

    CAS  Article  Google Scholar 

  30. 30.

    Wollenberg, R. D. et al. Real-time imaging of the growth-inhibitory effect of JS399-19 on Fusarium. Pest. Biochem. Physiol. 134, 24–30 (2016).

    CAS  Article  Google Scholar 

  31. 31.

    Patterson, D. I., Nygaard, K., Steinberg, G. & Turley, A. M. Heterotrophic flagellates and other protists associated with oceanic detritus throughout the water column in the mid North Atlantic. J. Mar. Biol. Ass. UK 73, 67–95 (1993).

    Article  Google Scholar 

  32. 32.

    Pettitt, M. E., Orme, B. A. A., Blake, J. R. & Leadbeater, B. S. C. The hydrodynamics of filter feeding in choanoflagellates. Europ. J. Protistol. 38, 313–332 (2002).

    Article  Google Scholar 

  33. 33.

    Orme, B. A. A., Blake, J. R. & Otto, S. R. Modelling the motion of particles around choanoflagellates. J. Fluid Mech. 475, 333–355 (2003).

    ADS  Article  Google Scholar 

  34. 34.

    Heinbokel, J. F. Studies on the functional role of tintinnids in the Southern California Bight. I. Grazing and growth rates in laboratory cultures. Mar Biol 47, 177–189 (1978).

    Article  Google Scholar 

  35. 35.

    Leadbeater, B. S. C. Developmental studies on the loricate choanoflagellate Stephanoeca diplocostata Ellis. VI. Effects of silica replenishment on silica impoverished cells. Protoplasma 153, 71–84 (1989).

    Article  Google Scholar 

  36. 36.

    Leadbeater, B. S. C. & Davies, M. E. Developmental studies on the loricate choanoflagellate Stephanoeca diplocostata Ellis. III. Growth and turnover of silica, preliminary observations. Exp. Mar. Biol. Ecol. 81, 251–268 (1984).

    CAS  Article  Google Scholar 

  37. 37.

    Nitsche, F., Thomsen, H. A. & Richter, D. J. Bridging the gap between morphological species and molecular barcodes – Exemplified by loricate choanoflagellates. Europ. J. Protistol. 57, 26–37 (2017).

    Article  Google Scholar 

Download references

Acknowledgements

We thank Professor Tom Fenchel for constructive criticism of the manuscript and laboratory assistant Annemarie Højmark for assistance in the laboratory. This work was supported by a research grant (9278) from VILLUM FONDEN.

Author information

Affiliations

Authors

Contributions

N.T.E. wrote the first draft, J.T. carried out growth experiments, R.D.W. and T.E.S. carried out genetic analysis and took part in the growth experiments, P.F. and P.A. isolated Diaphanoeca grandis and carried out electron microscopy. All authors contributed to the data analysis and the editing of the manuscript.

Corresponding author

Correspondence to Niels Thomas Eriksen.

Ethics declarations

Competing Interests

The authors declare no competing interests.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license 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 license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Eriksen, N.T., Tophøj, J., Wollenberg, R.D. et al. Growth and single cell kinetics of the loricate choanoflagellate Diaphanoeca grandis. Sci Rep 9, 14543 (2019). https://doi.org/10.1038/s41598-019-50998-0

Download citation

Further reading

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.

Search

Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing