Article | Open | Published:

Cdh2 coordinates Myosin-II dependent internalisation of the zebrafish neural plate

Scientific Reportsvolume 9, Article number: 1835 (2019) | Download Citation

Abstract

Tissue internalisation is a key morphogenetic mechanism by which embryonic tissues generate complex internal organs and a number of studies of epithelia have outlined a general view of tissue internalisation. Here we have used quantitative live imaging and mutant analysis to determine whether similar mechanisms are responsible for internalisation in a tissue that apparently does not have a typical epithelial organisation – the zebrafish neural plate. We found that although zebrafish embryos begin neurulation without a conventional epithelium, medially located neural plate cells adopt strategies typical of epithelia in order to constrict their dorsal surface membrane during cell internalisation. Furthermore, we show that Myosin-II activity is a significant driver of this transient cell remodeling which also depends on Cdh2 (N-cadherin). Abrogation of Cdh2 results in defective Myosin-II distribution, mislocalised internalisation events and defective neural plate morphogenesis. Our work suggests Cdh2 coordinates Myosin-II dependent internalisation of the zebrafish neural plate.

Introduction

The internalisation of superficial sheets of cells is a widely used developmental strategy to generate complex three-dimensional structures with well-defined shape and size. Through this mechanism, animal tissues form a number of internal organs including the vertebrate central nervous system1,2. In recent years, live imaging studies and mutant analysis has begun to define the cellular, molecular, and biomechanical mechanisms responsible for tissue internalisation in a growing number of tractable model systems3,4. Collectively, these studies have identified that tissue internalisation is thought to occur by an interplay of cell shape changes, cell adhesion remodelling and subcellular cytoskeletal protein dynamics, including the cortical Actomyosin motor complex2,4. In recent years, Drosophila ventral midline furrow formation during gastrulation has been an instrumental model system to dissect the cellular and molecular mechanisms underlying in vivo tissue internalisation5,6,7. Live imaging analysis in gastrulating flies have indicated that tissue internalisation is achieved by a coordinated activity of medial cells which show progressive and irreversible cell surface constriction while keeping a more or less constant cell volume6,8. Furthermore, recent studies have demonstrated that this cell behaviour is powered by cortical Myosin-II network7, and that the cell-cell adhesion molecules including E-Cadherin are critical to efficiently transmit and coordinate tension across the internalising tissue9. Thus apical constriction has been identified as a dominant and instrumental cell behaviour for surface tissue internalisation in epithelia.

Neurulation in zebrafish is a complex morphogenetic event that first transforms the neural plate into a neural keel and then a neural rod before lumen formation generates the neural tube structure. The details of this process are incompletely understood but initially involve two components, one is convergence of neural plate cells towards the midline and the second is an internalisation of cells at or close to the midline10,11. The efficiency of convergence depends on Planar Cell Polarity signaling12,13,14 and requires extracellular matrix and adjacent mesoderm for coordination15,16. Internalisation is less well understood but is a key step that deepens the most medial zone of the neural plate to generate the solid neural keel. While the most medial cells of the plate are internalising the more lateral cells are still converging to the midline to take the place of the internalised cells. In this respect the tissue movement appears somewhat like a conveyor belt, narrowing the neural plate as it deepens medially. The cell behaviours that underlie this tissue movement are not fully understood, however they are not simple and likely involve cell shape changes, cell orientation changes and cell intercalations. During this period of internalisation the cells of the neural plate and keel are not organised as a columnar neuroepithelium as found in other vertebrates. The pseudostratified epithelial organisation does not arise in teleosts until late neural rod stage, coincident with lumen formation12,13,14,15,16,17,18,19. This is in contrast to amniote and amphibian neural plates that have a clear epithelial organisation and use apical constriction to fold the epithelium and internalise the neuroectoderm during neurulation20,21. This poses the question of what cell behaviours drive internalisation in the fish neural plate. So far the best clue to this is the dependence of this process on the cell adhesion protein Cdh2 (previously called N-cadherin). Embryos mutant for Cdh2 fail to complete convergence and internalisation of the neural plate, with the phenotype particularly strong in the hindbrain region19,22. A reduction in protrusive behavior of neural plate cells has been suggested to contribute to this phenotype19 but Cdh2-dependent convergence and internalisation remains incompletely understood.

Here we have applied quantitative live imaging and genetic analysis to understand tissue internalisation in the hindbrain region of the zebrafish neural plate. We show that while the organisation and movements of the teleost neural plate are distinct from neural plate in other vertebrates, cell internalisation at the dorsal midline is achieved by adopting similar cellular strategies. This includes deployment of Cdh2 and Myosin-II to effect constriction of the dorsal cell surfaces to generate inward traction. Furthermore, we show this medial neural plate behaviour depends on Cdh2 function and superficial non-muscle Myosin-II activity at the internalisation zone. While Myosin-II inhibition blocks cell surface constriction and cell internalisation, depletion of Cdh2 leads to mislocalised Myosin-II distribution and random cell internalisation events along the dorsal surface. Together, these results suggest the zebrafish neural plate deploys strategies of cell surface constriction similar to conventional epithelia to effect internalisation. Overall, our observations suggest Cdh2 coordinates Myosin-II dependent internalisation of the zebrafish neural plate.

Results

Neural plate internalisation occurs through reorientation and elongation of neural plate cells

In the prospective hindbrain region, the zebrafish neural plate is a multi-layered tissue of 3–6 cell deep at 10 hours post fertilisation (hpf)12,15 (Fig. 1a timepoint 0 min). To study changes in cell morphology we first labelled cells with the plasma membrane constructs CAAX-GFP and made confocal time-lapse movies in the transverse plane. At the 10 hpf stage, most cells are largely round-shape in transverse section and progressively elongate in the transverse plane as they converge to the midline and internalise to form the neural keel (Fig. 1a–c and Movie 1). To quantify these cell shape changes we assigned cells to lateral zones (between 20–60 µm from the midline) and medial zones (within 20 µm of the midline) of the neural plate, and then measured the long axis of cells and the angle they subtend to the parasagittal plane of the embryo (Fig. 1c,d). Up to 11 hpf mean cell length increases at the same rate in both lateral and medial zones, after 11 hpf cells in the medial zone continue to elongate while the mean length of more lateral cells is more stable (Fig. 1d). The orientation of the long axis of both medial and lateral cells leans in towards the midline at an angle of approximately 50° up to 11 hpf, after that time medial cells reduce this angle to approximately 30° while lateral cells increase their angle to approximately 80°. Between 11 and 13 hpf the depth of the neural plate increases in the medial zone by approximately 300% (from 42 µm to 138 µm on average, Fig. 1a,b, and Movie 1, nembryos = 4) as medial cells internalise and the plate begins to transform into the neural keel. To analyse the overall coordination of hindbrain neural plate cells during internalisation we made movies from 9–11 hpf of cells labelled with the nuclei marker H2B-GFP (Movie 2). We then tracked nuclei movements using 3D + time tracking analysis on the Bioemergence platform + Mov-IT pipeline23 (Fig. 1e–g, nembryos = 3). We first assessed and quantified nuclei movements from the dorsal view (Movie 2). Up to 11 hpf nuclei are seen to move both medially and anteriorly (Fig. 1e). From 11 hpf nuclei move more directly medially and the anterior component to their movement is largely lost (Fig. 1e’). We next tracked nuclei in the transverse plane and between 9 and 11 hpf most nuclei move medially with relatively straight trajectories towards the midline (Fig. 1f,g). Between 11 and 12 hpf nuclei close the midline change their direction and begin to move deeper into the embryo. Between 12 and 13 hpf most nuclei within 40 µm of the midline are directed down into the embryo. While medial nuclei move deep into the embryo, more lateral nuclei are still moving medially as they converge towards the midline. An analysis of speed shows lateral cells accelerate towards the midline between 10 and 11.5 hpf, while medial cells initially move quicker than lateral cells but after 11 hpf move more slowly (Fig. 1h) (nembryos = 3, naverage of medial cells analysed = 90, naverage of lateral cells analysed = 80 in each transverse view assay, P < 0.0001). In conclusion, convergence towards the midline is accompanied by an elongation and reorientation of cells, and internalisation involves a distinctive reorientation of nuclei movements in the medial zone of the neural plate.

Figure 1
Figure 1

Cell and tissue dynamics during zebrafish neural plate internalisation. (a) Four transverse view confocal images depicting the neural plate, keel, rod and tube stages of wild-type zebrafish neurulation at hindbrain levels. Cells membranes labelled with CAAX-GFP. Scale bar is 20 µm and OV indicates otic vesicle as hindbrain landmark. The medial zone (mz) and lateral zone (lz) of the neural plate are indicated in (a) and each is 20 µm wide. (b) Time course showing depth of the neural anlage at the midline. Internalisation deepens the neural anlage by approximately 300% in the plate to keel transition (initial thickness ~42 µm on average vs final thickness ~138 µm on average, nembryos = 4). np, neural plate; nk, neural keel; nr, neural rod; and nt, neural tube. (c) Frames from transverse view time-lapse to illustrate cell profile changes during plate to keel transition. Double headed arrows illustrate examples of measurements of the long axis of cells used to quantify cell elongation. EVL (enveloping cell layer) is highlighted in pale blue. (d) Quantification of cell elongation and cell angle in medial and lateral zones during plate to keel transition. (e and e’) Projected views from dorsal surface of nuclei tracks at 11 hpf and 12 hpf. Nuclei tracked from movies of cells labelled with H2B-GFP. (f) Transverse view image of nuclei tracked during convergence to midline (10.5 hpf). Scale bar, 20 µm. (g) Transverse views of nuclei tracks of neural plate dynamics during convergence and internalisation (9–13 hpf, for simplicity only half of the neural plate is illustrated). Red arrows indicate tissue movement, and arrowhead indicates midline position. D, indicates dorsal, while v, indicates ventral. (h) Quantification of nuclei speeds for medial and lateral cells during convergence and internalisation (nembryos = 3, naverage of medial cells analysed = 90, naverage of lateral cells analysed = 80, 5 z-slice analysed in each embryo).

Internalisation of neural plate cells is achieved by progressive cell surface reduction

To better understand neural plate cell internalisation, we imaged membrane labelled cells from dorsal to obtain an en face surface view of hindbrain neural plate (Fig. 2a). Using z-stacks with 0.25 µm z-intervals, we could eliminate dorsal enveloping layer cells (EVL) from above the neural cells to reveal the cell dynamics at the dorsal surface of neural plate. At 11–12 hpf, following individual medial cells showed that these cells undergo progressive dorsal surface reduction and internalisation and eventually become lost from the imaging plane (Fig. 2b). Most individual lateral cells largely do not reduce their dorsal profile over this time (Fig. 2b). This was confirmed by quantifying the dorsal cell profiles within a medial and a lateral region of interest over a 60 minute time period (Fig. 2c, Movies 3,4). In general the dorsal profiles in the medial zone are smaller than the profiles in the lateral zone, but there is some heterogeneity in both (small profiles are darker grey than the larger profiles in Fig. 2c). Over this time period the mean dorsal surface profile of medial cells decreases by approximately 50%, while the mean of cells in the lateral zone remains constant (Fig. 2d). Contraction of the superficial dorsal surface of cells thus occurs largely in the medial zone of the neural plate and largely occurs on a cell by cell basis as we find small profiles surrounded by large profiles in this zone. To quantify cell surface constriction we measured both cell aspect ratio (independent of cell orientation), and cell surface alignment relative to the embryo axis (Fig. 2e,f, nembryos = 4, 75 medial and 70 lateral cells in each assay). These data show the dorsal surface of cells tends to constrict anisotropically (more in the mediolateral dimension than their anteroposterior dimension) and the long axis of this surface of the cells is weakly aligned to the anteroposterior axis of the embryo. Taken together, these analyses demonstrate that neural plate internalisation is preceded by progressive anisotropic reduction of the dorsal surface of cells in the medial zone.

Figure 2
Figure 2

Dorsal cell surface dynamics during internalisation. (a) Schematic of the imaging approach to visualise dorsal cell surface profile during convergence and internalisation. Inverted LUT image depicts cell membrane outlines. D is dorsal, v is ventral, and n is notochord. Scale bar is 20 µm. (b) Tangential z-slices 5–7 µm below EVL were selected for automated segmentation of dorsal surface of superficial neural plate cells. Top panels: image of dorsal surface of medial cell over time (pseudocoloured in cyan). Bottom panels: images of dorsal surface of lateral cell over time (pseudocoloured in yellow). Scale bar, 5 µm and time is in minutes. (c) Dorsal surface profiles of medial and lateral populations of cells one hour apart. For simplicity only half of the neural plate is shown. Colour code indicates relative dorsal surface profile area in µm2, darker greys are smaller than lighter greys. Black arrowhead indicates midline position. Scale bar, 10 µm. (d) Mean dorsal surface area of medial (red) and lateral (blue) cells over time (nembryos = 4 wt analysed, P < 0.0001). (e) Schematic representation of a cell’s dorsal surface area to illustrate cell aspect ratio and alignment of this surface area to the anteroposterior axis of the embryo. (f) Quantification of surface aspect ratio and alignment to embryonic axis. In all graphs error bars indicate SEM.

Myosin-II is required for zebrafish neural plate internalisation

In other systems, apical surface constriction leading to internalisation is thought to be powered by apical actomyosin networks3,4,7 To assess whether myosin activity is likely to drive contraction of the dorsal surface of medial neural plate cells we first used immunohistochemistry to analyse the localisation of phospho-Myosin light chain. Consistent with a role for myosin in surface constriction we detected high levels of phosho-Myosin along the dorsal surface of superficial neural plate cells immediately underneath the large non-neural EVL cells (Fig. 3a–d). Distinctive phospho-Myosin puncta could also be seen deeper in the neural plate scattered along the Phalloidin stained cell cortices (Fig. 3e–g”). We next checked whether we could monitor actomyosin localisation in the neural plate in living embryos to determine its dynamic distribution during neural plate morphogenesis. The transgenic embryos (Tg(actb1:myl12.1-GFP), hereafter called Myosin-II:GFP) and (Tg(actb1:GFP-utrCH), hereafter called Actin:GFP)24,25 faithfully recapitulated the distribution of phospho-Myosin and F-actin in neural plate cells revealed by antibody and Phalloidin staining respectively (Fig. 3h–j”).

Figure 3
Figure 3

Myosin and actin in the neural plate. (a–d) Transverse confocal section of neural plate stained for phosho-myosin and F-actin. (e,e”) Horizontal confocal section through EVL stained for phospho-myosin and F-actin. (f,f”) Horizontal confocal section at level of dorsal surface of neural plate cells stained for phospho-myosin and F-actin. (g,g”) Horizontal confocal section 3 µm below level of dorsal surface of neural plate cells stained for phospho-myosin and F-actin. (h–j”) Myosin and actin revealed in living neural plate by Tg(actb1:myl12.1-GFP) and Tg(actb1:GFP-utrCH) transgenic embryos. Sections equivalent to panels (e–g”). Scale bars are 5 µm.

Tranverse plane confocal movies of the Myosin-GFP and Actin-GFP embryos from 11 hpf to 14 hpf revealed their distribution during neural plate to neural keel morphogenesis. During internalisation at 11–13 hpf, non-muscle Myosin-II:GFP is strongly enriched at the dorsal surface of medial regions of neural plate (white arrows in Fig. 4a, nembryos = 3, and Movie 5), and some focal accumulation can be also found at the ventral surface of the plate (cyan arrow in Fig. 4a) and scattered through the depth of the plate. As neurulation reaches the end of keel formation at 14 hpf, Myosin-II:GFP enrichment is lost from the dorsal midline position (Fig. 4a), suggesting that its activity is temporally and spatially correlated with tissue internalisation. Analysis of confocal z-stacks collected from a dorsal view confirms high levels of Myosin-II:GFP are largely restricted to dorsal surface of the neural plate cells (Fig. 4b, nembryos = 3) with a marked distribution close to the superficial plasma membrane (Fig. 4b z-levels 7.5–10 µm, Fig. 4c). In contrast to Myosin-II:GFP localisation however, the distribution of Actin:GFP is somewhat more uniform across both the dorsoventral axis and mediolateral axis of the neural plate (Fig. 4e). There is a slight bias of Actin:GFP to the dorsal side of the neural plate but, in contrast to Myosin-II:GFP, the Actin:GFP gradient is much shallower within the first 40 µm from the dorsal surface (Fig. 4e). To investigate Myosin-II function during internalisation we made use of the specific Myosin-II inhibitor Blebbistatin26. The movements of convergence of the neural plate and neural keel formation were inhibited by 50 µM Blebbistatin (Fig. 4f,g). Moreover, we found that abrogating Myosin-II activity during this developmental time, leads to a complete block of dorsal cell surface constriction that usually characterises medial neural plate cells (Fig. 4h,i, nembryos = 3, nmedial cells = 35, nlateral cells = 40). Thus Myosin-II is a significant driver of superficial cell constriction and the movements of convergence and keel formation.

Figure 4
Figure 4

Myosin distribution and function during convergence and internalisation. (a)Transverse confocal images depicting the distribution of the Myosin-II:GFP fusion protein using Tg(actb1:myl12.1-GFP)24 transgenic line during zebrafish neural plate internalisation. White arrows in (a) indicate medial accumulation of Myosin-II:GFP, while cyan arrow shows basal accumulation. Insets show dorsal medial zone at higher magnification. Yellow arrowheads indicate midline position. Scale bar is 20 µm. (b) Dorsal view confocal images of Myosin-II:GFP expression at different depths. Top image is in EVL (the superficial non-neural epithelium), then successive depths through the neural plate. Each image is a maximum intensity projection of 5 confocal slices. Scale bar, 10 µm. (c) Representative transverse view confocal images showing actin expression by using zebrafish Tg(actb1:GFP-utrCH)25 reporter line during early internalisation. Arrowhead shows midline and brackets indicate superficial-deep axis for quantification in (e, bottom graph). Scale bar, 30 µm and arrowhead indicates midline. (d) Dorsal view confocal images of Actin:GFP distribution at dorsal surface of neural plate and 10 µm deeper. Scale bar is 20 µm. (e) Top graph: quantification of medio-lateral surface distribution of Myosin-II:GFP (red) versus Actin:GFP (black) throughout internalisation. Bottom graph: quantification of Myosin-II:GFP (red) and Actin:GFP (black) pixel intensity distribution along the superficial (EVL first 5 µm) to deeper (ventral) axis of the neural plate (see methods for quantification procedure). A.U, indicates arbitrary units. (f) Transverse views of neural morphogenesis in control and Blebbistatin treated embryos. Scale bar is 20 µm. (g) Quantification of neural plate to keel transition in control and Blebbistatin treated embryos. (h) Dorsal cell surface profiles in medial and lateral zones of neural plate in control and Blebbistatin treated embryos. Scale bar, 10 µm and time is in minutes. Arrowheads indicate position of the tissue midline. (i) Quantification of dorsal cell surface profiles and alignment of dorsal surface areas to embryonic axis in control and Blebbistatin treated embryos (nembryos = 3, nmedial cells = 35, nlateral cells = 40). In all graphs, bars indicate SEM.

Loss of cdh2 leads to aberrant cell and tissue dynamics during internalisation

The generation of traction through Myosin-II dependent contractility during epithelial morphogenesis is thought to depend partially on cell-cell adhesion molecules like Cadherins9,27 and through adaptor proteins including α-Catenin28,29. Since Myosin-II drives dorsal cell constriction during neural plate internalisation and previous work shows a requirement for Cdh2 in the early stages of zebrafish neural tube morphogenesis, it is likely that the tissue and cell behaviours of internalisation should be defective in the previously identified cdh2 mutant parachute (pac)19,22. Quantification of cell and tissue behaviours from transverse view imaging at prospective hindbrain levels shows that at 10–11 hpf, cdh2/pac mutant embryos start neurulation with a fairly normal neural plate morphology similar to wild-type animals (Fig. 5a,a’). However, by neural keel stages (12–13 hpf), cdh2/pac mutants display abnormal neural plate internalisation leading to a consistent and highly-reproducible aberrant T-shape or “parachute” morphology19,22, leading to aberrant neural tube organisation (Fig. 5a,a’, nembryos = 5, Fig. S1, and Movie 6). Quantification confirms cdh2 is required to complete internalisation as pac mutants deepen only 62% of the neural tissue as compare to wild-type (wt 138 µm vs cdh2/pac 85 µm, nembryos = 4 wt, 4 cdh2/pac, P < 0.0001, Fig. 5b). To better define Cdh2 dependent cell behaviours we reconstructed nuclei tracks in wt and pac mutants. Abnormal cell behaviours were evident in pac neural plates from 9 hpf through to 12 hpf (Fig. 5c,d). The most prominent defects were seen at 11 and 12 hpf when convergence of lateral cells towards the midline (Fig. 5e) and the inward trajectory of medial cells (Fig. 5f) are severely compromised. In contrast to wt nuclei that show clear differences in behaviour at lateral and medial locations, the tracks of nuclei of pac cells appear very similar at both lateral and medial locations (Fig. 5e,f), thus the distinctive behaviours of cells at the midline is lost. The speed of movement of medial pac nuclei is slower than wt nuclei, and lateral pac cells are initially slightly faster than wt cells but by 12 hpf are significantly slower than lateral wt cells (Fig. 5g). Although loss of a cell adhesion protein might be expected to alter tissue compaction, the distance between neighbouring nuclei is not significantly different between wt and pac cells, showing the density of cells is unchanged (Fig. 5h).

Figure 5
Figure 5

Defective cell and tissue internalisation in cdh2/pac mutants. (a-a’) Transverse confocal time-lapse images of tissue internalisation between wild-type (a) and cdh2/pac mutant (a’) embryos at hindbrain level. Cell membranes labelled with CAAX-GFP. ov, otic vesicle. Yellow dots outline neural tissue. (b) Comparative internalisation dynamics between wild-type (red) and cdh2/pac (blue) embryos as measured by depth of the neural primordium at its midline (cyan bar in a,a’). While in wild-type embryos, internalisation is responsible to deepens up to 70% of the neural primordium (~42 µm/~138 µm on average), cdh2/pac mutants average only 62% to wt values (~44 µm/~85 µm, nembryos = 4 cdh2/pac. Average depth; 85 µm cdh2/pac vs 138 µm wt). (c and d) Representative transverse images of nuclei tracks in wild-type (c) and cdh2/pac (d) neural plate cells during convergence and internalisation stages. Cdh2/pac nuclei show defective convergence and internalisation. (e) Higher magnification of lateral nuclei tracks taken from red boxes in (c,d). (f) Higher magnification of medial nuclei tracks taken from yellow boxes in (c,d). (g,h) Quantification of nuclei speeds and density between wild-type and cdh2/pac (nembryos = 3, naverage of medial cells analysed = 90, naverage of lateral cells analysed = 80, 5 z-slices analysed in each embryo). Scale bar in (a-f), 20 µm. Bars indicate SEM.

Cdh2 is enriched at superficial surface during internalisation

We next asked whether Cdh2 protein localisation was consistent with a role in mediating Myosin-II dependent constriction of dorsal cell surfaces. We studied Cdh2 localisation using the BAC-reporter TgBAC(cdh2:cdh2-tFT), which faithfully recapitulates zebrafish Cdh2 expression30. The tandem fluorescent timer (tFT) technology coupled in TgBAC(cdh2:cdh2-tFT) comprising a rapidly maturing superfolded GFP and a slower maturing red fluorescent counterpart (tagRFP) has been used to assess protein life-time turnover, including Cdh2 maturation30,31. We were only able to detect robust expression of the more stable Cdh2-RFP in cell-cell junctions after internalisation at rod stages of development (14–15 hpf, Fig. S2), however Cdh2-GFP expression is readily detected from neural plate stages. Although Cdh2-GFP is present at low levels throughout the neural cell membranes, there is markedly higher expression at the dorsal surface of the neural plate (Fig. 6a,b, nembryos = 4). In addition, by imaging from the dorsal surface we found Cdh2-GFP is particularly enriched at cell-cell and multi-cellular interfaces during dorsal surface constriction events close to the neural plate midline (arrowheads in Fig. 6c,c’).

Figure 6
Figure 6

Cdh2 distribution during neural plate internalisation. (a,a’) Confocal transverse plane views of Cdh2-GFP at the dorsal surface of the neural plate. Cdh2-GFP is expressed throughout the cell membranes but is enriched at the dorsal surface (arrowheads). d, indicates dorsal surface. (b) Diagram indicating location of transverse views shown in (a,a’). (c,c’) Time-lapse frames of confocal images in dorsal view of the dorsal surface of the neural plate show that Cdh2-GFP is enriched at superficial surface in neural plate cells and at multi-cell interfaces. Fire lookup table indicating intensity values (0–255) in (c’). (d) Quantification of Cdh2-GFP intensity at different depths of the neural plate (nembryos = 4). Scale bars, 10 µm.

Depletion of Cdh2 reduces dorsal contraction of medial neural plate cells

The orientation of tissue contractility and force transmission depends on the integrity of intercellular adhesion molecules to mechanically couple cells within a giving tissue9,32. While this phenomenon has been described in folding insect epithelia9, it is not entirely clear to what extent this is conserved in vertebrate neural tube morphogenesis. To explore the interrelationship of Cdh2 and Myosin-II contractility during neural plate internalisation, we studied Myosin-II:GFP dynamics in cdh2 deficient embryos. Reduction of Cdh2 was achieved by using a previously characterised antisense morpholino (MO), which faithfully phenocopy the cdh2 mutant pac22. We found that although Myosin-II:GFP is still enriched at the dorsal surface of the cdh2 MO neural plate (arrows in Fig. 7a,a’, and Movie 7) its distribution is different to wild-type embryos. Elevated Myosin-II:GFP expression is found in the medial region of the wild-type neural plate (Fig. 4a), but this preferential medial distribution is absent from pac embryos (Fig. 7a,b). This abnormal Myosin-II:GFP localisation is maintained into later stages of neural plate morphogenesis (Fig. 7a,b,d). To test whether reduced Cdh2 function and an abnormal Myosin-II:GFP distribution impacts the dorsal cell surface contraction events of normal internalisation we monitored dorsal cell surface profiles in Cdh2 deficient neural plates (Fig. 7e–g). In contrast to wild-type animals where internalisation is largely restricted to cells close to the midline, reduction of Cdh2 results in random cell internalisation events across the entire width of the dorsal surface of the neural plate (Fig. 7h, nembryos = 5 cdh2/pac, ncells = 120 per assay, and Movie 8). Individual internalisation events were confirmed by transverse view imaging (Fig. 7c). Furthermore the dorsal surface constriction of medial neural plate cells is reduced in Cdh2 depleted embryos, while constriction of lateral cells is increased (Fig. 7i,j). The orientation of the cells’ dorsal surface profile relative to the embryo’s axis is also slightly altered from wild-type (Fig. 7i,j).

Figure 7
Figure 7

Cdh2 is required to organise midline Myosin-II during internalisation. (a) Frames from a transverse confocal time-lapse showing surface distribution of Myosin-II:GFP during cdh2 MO deficient neural plate internalisation (left panel). White arrows show surface Myosin-II:GFP distribution, while cyan arrows indicate basal Myosin-II:GFP accumulation. (a’) Fire lookup table indicating intensity values (0–255). (b) Comparative quantification of medio-lateral surface Myosin-II:GFP distribution between wild-type (red) and cdh2 MO (blue) during internalisation (nembryos = 5 wt, 4 cdh2 MO, P < 0.0001). (c) Representative example of ectopic cell internalisation in cdh2 MO (nembryos = 3, nectopic cells internalisation = 28). (d) Left panels: single dorsal confocal frames showing abnormal midline Myosin-II:GFP distribution in cdh2 MO embryos (arrowheads). Right panels: fire lookup table, showing intensity profile. Dashed line represent midline. (eg) Dorsal picture of cdh2 MO neural plate. (e) Bright field dorsal view images in cdh2/pac tissue by 12 hpf. Scale bar is 20 µm. (f) Single dorsal confocal slice depicting cells’ dorsal area profiles in cdh2/pac neural plate labelled with membrane-GFP (gray). (g) Automated cell area profile reconstruction from (f). a = anterior, p = posterior. Arrowhead and dashed lines in (eg) represent tissue midline. (h) Cdh2/pac mutant dorsal cell surface profiles during defective internalisation. Arrowheads indicate cell constriction events and dashed line represent tissue midline (ml). Scale bar, 10 µm and time is in hpf. (ij) Quantification of dorsal cell area profiles during cdh2/pac mutant internalisation. (i) Mean cell surface area between medial (wt red, cdh2/pac green left, P = 0.0121), and lateral cells (wt blue, cdh2/pac orange, P < 0.0001). (j) Comparative cell aligment along the anterior-posterior embryo’s axis between medial (wt red, cdh2/pac green left, P = 0.023), and lateral cells (wt blue, cdh2/pac orange, P = 0.078).

Discussion

Zebrafish embryos generate a neural tube by a complex array of cell behaviors10,11,12,15. Initially this involves the movement of a large body of cells towards the dorsal midline14,15,16. Then tissue internalisation at the midline transforms the neural plate into a neural keel and then solid cylindrical neural rod structure. These highly organised collective movements of dorsal midline cells are dependent on extrinsic cues from mesoderm and extracellular matrix15,16,17, as well as cell-cell interactions between the neural cells themselves13,14,17,19,22. While tissue internalisation is a fundamental step in this morphogenetic process, its cellular and molecular nature has remained rather elusive. In this work we have shed light on some of the cellular events of neural plate cell internalisation in the zebrafish. This step is driven by previously uncharacterised cell surface constriction events in the medial zone of the neural plate. We show these superficial constriction events are dependent on Cdh2 and Myosin-II.

Unlike other vertebrates the teleost neural plate is not a columnar epithelium and does not transform into a neural tube by the conventional primary neurulation mechanism of epithelial folding. Additionally the distribution of polarity proteins within the teleost neural plate18 and its unusual cell behaviours have led to the view that it is not an obviously epithelialised tissue. Despite this, our study suggests internalising zebrafish neural plate cells deploy a similar strategy and molecular machinery to that widely used in epithelial tissue infolding events. Central to this in other systems is the presence of a contractile activity of non-muscle Myosin-II and cell-cell adhesion machinery of Cadherins at cell and tissue surfaces4,7,9,20,21. During epithelial morphogenesis in flies, cortical Myosin-II has been shown to exhibit a distinctive pulsatile behaviour in internalising cells while assuming a more interconnected network at tissue level7,9. Our live imaging analyses reveal that during zebrafish neural plate internalisation, Myosin-II shows a transient enrichment at the superficial surface of medial neural plate cells. While at the moment we do not know the higher resolution organisation and dynamics of Myosin-II activity in individual cells of the fish neural plate, we hypothesise that Myosin-II activity exerts a mechanical tension across the dorsal surface of medial neural plate cells to progressively constrict their superficial surface and mediate cell internalisation. We find cell internalisation appears to occur on a cell by cell basis rather than a coordinated internalisation of neighbouring cells.

Myosin-II dependent forces at the cell cortex are thought to be organised and transmitted through the tissue by cell-cell surface molecules including Cadherin family9,27,29. During Drosophila mesoderm invagination, precise accumulation of Myosin-II at the ventral midline surface greatly depends on adherens junctions33. Disruption of these cell-cell adhesion molecules during insect gastrulation, result in broader Myosin-II expression at the midline surface and impaired tissue invagination33, which is reminiscent to our observation of Myosin-II distribution in neural plate depleted of Cdh2. Similar to E-cadherin function9, lack of N-cadherin during insect epithelial morphogenesis result in abnormal tissue remodeling, impaired Myosin-II organisation and defective cell anisotropy34. During neurulation in mice and frogs, the depletion of Cdh2 results in defective Myosin-II expression and aberrant neural tube development35,36,37. Although the teleost neural plate is structurally different to other vertebrates the impaired convergence and internalisation of neural cells in the zebrafish cdh2/pac mutant has some similarities to an open neural tube phenotype. Here we show Myosin II contractility is a significant driver of cell surface constriction at the dorsal surface of neural plate and cell surface constriction is defective in Cdh2 mutants. Thus Cdh2 is required to mediate the dorsal cell surface remodeling required in the medial zone of the neural plate to effect cell internalisation.

It is interesting to note that although the mechanisms used to transform neural plate into a neural tube are quite different in teleosts compared to other vertebrates, the deployment of actomyosin-based contractility to the superficial surface of the neural plate is conserved. In most vertebrates this drives apical constriction to effect bending of the neural plate epithelium and elevation of the neural folds38,39,40,41, whereas in the teleost it is necessary for cells to internalise from the superficial surface of the neural plate midline to generate the solid neural keel and rod.

Our current work has focused on the cell constriction behaviours at the dorsal surface of the zebrafish neural plate and the contribution of deeper cell behaviours to neural plate morphogenesis remain unknown. In other systems apical constriction is often accompanied by expansion of basal cell surface resulting in wedge-shaped cell morphologies and this is thought to be a paradigm for tissue folding in a wide range of developmental contexts3,4,6, including vertebrate neural tube formation4,20,21. Our preliminary analysis of cell morphologies from ubiquitously labelled cells (Fig. 1) suggests zebrafish cells acquire spindle shaped morphologies during internalisation rather than wedge-shaped morphologies, and suggest most cells do not stretch from the dorsal surface to the ventral surface of the plate during this behavior. It seems likely that cell elongation in the medial zone of the neural plate contributes to deepening of the tissue as it transforms into the neural keel, but an accurate description of individual cell morphologies and behaviours awaits more comprehensive analysis of mosaically labelled tissues. It will also be important to understand the nature of the junctions between cells at the dorsal surface of the plate and this will probably require a 3D-EM characterisation42.

In conclusion, although its organisation and cell behaviours10,11,12,14,15,16,17,18,19 mean the epithelial nature of the teleost neural plate remains somewhat enigmatic, our results suggest it none the less employs cell surface constriction strategies, based on Cadherin adhesions and Myosin II contractility, typically used by epithelia for internalisation events. Moreover, we hypothesise that this epithelia-like remodeling has to be transient in the fish neural plate in order to allow the subsequent repertoire of cell interdigitation and mirror-symmetric divisions that occur across the neural midline during keel and rod stages12,13,17,19.

Methods

Ethics statement

All experimental procedures involving animals were approved by the College Research Ethics Committee at King’s College London (London, UK) and covered by the Home Office Animals (Scientific Procedures) Act 1986 (ASPA) project licence, and by the Comité de Etica y Bioética DID-UACh (Bioética en uso de Animales en la Investigación, DID-UACh). All methods were performed in accordance with the relevant guidelines and regulations.

Zebrafish husbandry and strains

Wild-type, transgenic and mutant adult zebrafish were maintained under standard conditionsm43 on a 14-hour photoperiod at the KCL, and UACh Fish Facilities, respectively. Embryos were collected from timed matings and raised at 28.5 °C in fish water or E3 embryo medium43. Animals were staged according to published morphological criteria44 and stages are given in terms of hours post fertilisation (hpf). The following strains were used in this study: wild-type (wt) TL and AB, cdh2fr722, Tg(actb1:myl12.1-GFP)24, Tg(actb1:GFP-utrCH)25, and TgBAC(cdh2:cdh2-tFT)30.

mRNA synthesis and microinjections

PCS2+ expression vectors carrying membrane-localised fluorescent proteins CAAX-GFP or CAAX-mRFP, nuclear localized proteins H2B-GFP or H2B-RFP were linearised using restriction enzymes for 3 hours at 37 °C and precipitated at −20 °C in 70% ethanol. DNA was then washed and resuspended in RNAase free water. Sense capped mRNA was transcribed using the mMESSAGE SP6/T7/T3 Kit (Ambion) and purified later using columns (Roche). Finally, mRNA concentration was measured in nanodrop (Thermoscientific). All microinjections were performed in a dissecting microscope using a glass slide and petri dish. Injections were made at one-cell stage embryo and mRNA constructs (150 pg per embryo) were delivered using a glass micropipette with filament (Harvard Apparatus) mounted on a micromanipulator and attached to a Picospritzer® (General Valve Corporation).

Plasmid DNAs were obtained from competent bacteria and linearised by enzymatic reaction using specific restriction enzymes for 2–3 hours at 37 °C in sterile 1.5 ml tubes (normally in 20 µl reaction). The linearised DNA was re-suspended in 100 µl of RNAase free water and extracted using 2 volumes of Phenol-Chloroform-Isoamyl alcohol mixture (25:24:1, Sigma). After vortexing for at least 3 minutes, the supernatant (normally 100 µl) was taken into a sterile 1.5 ml and precipitated overnight at −20 °C adding 2–3 volume of ethanol at 100% and 1/10 volume of Sodium acetate 0.05 M. Next day, the DNA was washed in 70% ethanol during 15 minutes by cold centrifugation (14.000 rpm). After removing of the supernatant, the linearised DNA was re-suspended in RNAase free water (normally 6 µl) ready for RNA transcription. Capped RNAs were transcribed using SP6 and T7 RNA polymerase using the mMessage mMachine kit (Ambion). Transcription reactions were carried out at 37 °C for 2–3 hours. mRNA was purified on columns (Mini Quick Spin RNA columns, Roche) and the final concentrations were calculated using a Nanodrop 3300 spectrometer (Thermo Scientific).

Antisense morpholino oligonucleotide injections

To inhibit Cdh2 function we used a previously characterised cdh2 morpholino (MO) oligonucleotide (cdh2 MO)22 against (5-TCTGTATAAAGAAACCGATAGAGTT-′3), corresponding to −40 to −16 of cdh2 cDNA22. cdh2 MO was purchased from Gene Tools (Philomath, OR), dissolved in water to a stock solution of 1 mM, and injected at 1-cell stage embryo at a final concentration of 50 µM.

Antibody staining

Whole-mount and tissue section immunohistochemistry was performed as previously described12,16. In this study we used mouse anti-ZO-1 (339111; Zymed) at 1:300, anti-rabbit Phospho-Myosin Light Chain 2 (Ser19) (3671; Cell Signaling) at 1:20 in 2.5% normal goat serum (Sigma). For secondary antibodies we used anti-mouse Alexa 488 and 633 (Molecular Probes) at 1:1,000 in 2.5% normal goat serum. For F-actin labelling we used Phalloidin (A12379; Invitrogen) at 1:1,000 in 2.5% normal goat serum. For analysis of neural tube organsition tissue sections were made every 14 mm on a HM 560 MV Micron microtome.

Blebbistatin treatment

To block Myosin-II activity, wild-type or Tg(actb1:myl12.1-GFP) embryos at 10 hpf were put in a small dish containing either 50 µM or 100 µM of Blebbistatin dissolved in E3 medium and raised at 28.5 °C. Transient Blebbistatin treatments were kept until 12 hpf while embryos were imaged by confocal microscopy. After pharmacological treatments embryos were washout from Blebbistatin and their morphology was assessed by 24 hpf.

Time-lapse imaging

For Supplementary Movie 2 and data Fig. 4, we used Bioemergence/Mov-IT workflow analysis23. Dechorionated wild-type and cdh2/pac embryos were transferred to 0.5% low melting point agarose (Sigma) and mounted dorsally at level of hindbrain in a 3 cm petri dish with glass containing a 0.5 × 0.78 mm2 hole at the centre and surrounded by teflon mold. Image acquisition was performed at 28.5 °C on an upright Leica SP5 confocal microscope using an Olympus objective 20X/0.95 NA water dipping lens. For imaging field size, we recorded at 351 × 351 µm for XY and 171 µm of Z depth, with 0.69 × 0.69 × 1.05 µm3 voxel size and time step of 2.5 m. After imaging recording, embryos were assessed for general morphology and potential neural tube defects. For all other movies, dechorioanted embryos were mounted in 0.8% low melting point agarose (Sigma) in embryo medium (E3). Transgenic animals and embryos expressing RFP/GFP-tagged membrane or nuclei constructs were imaged in either transverse or dorsal view at the level of the prospective hindbrain using the otic ear as anatomical landmark at 18 hpf. For transverse view registration images were taken 3–5 µm apart while for dorsal recording confocal images were taken 0.25 µm apart. In both cases, time-lapses were acquired on an upright Leica TCS SP5 LSM using a Leica 25 × 0.95 NA water dipping lens and a temperature chamber at 28.5 °C. Z-stacks were collected at 2–4-minute intervals, starting at 10 hpf and continuing in some cases up to 20 hpf.

Imaging processing

Center detection and automatic tracking at Bioemergence

Collections of.vtk files were uploaded to Bioemergences workflow23. Nucleus centre detection and cell tracking was performed using Mov-IT23. Automated 4D tracking of approximately 3500 cells within a 351 × 351 µm volume was performed16. For reconstruction of transverse movies, groups of ~100 neural plate cells were manually selected in standardised ROI in the developing hindbrain near the otic vesicle. Automated nuclei tracking was manually validated.

Cell dynamics

To quantify cell shape changes during internalisation, we used FIJI imaging software45 and customised Matlab code. Briefly, segmented cells were automatically obtained with FIJI by using the “trainable weka segmentation”46 plugin. Segmented binary images were then used in our customised Matlab code (MathWorks, Cambridge, UK) to extract cell parameters using major/minor axis on each cell computed using second order image moments (regionprops function in Matlab). A gray scale was used to quantify cell area (black = minimum cell area, white = maximum cell area, for each movie). To quantify cell aspect ratio independently of area, we divided the major axis by the minor axis to build an eccentricity index. For cell anisotropy measurements, we computed the absolute value of the relative angle of the major cell axis with respect to the anterior-posterior embryo axis, where the later was obtained manually from bright-field images.

Pixel intensity analysis

To quantify pixel intensity for Figs 4 and 6, the following approach was used: i) a consistent imaging set up was kept in all experimental conditions (stage of development, day of embryo imaging, construct concentration, confocal settings, laser power, offset, pinhole and averaging), ii) a histogram of all pixel intensities (256 gray levels) was calculated using three small region of interest (ROI, 3 µm × 3 µm) in 20 cells at each individual z-level. For dorsal surface measurements, we calculated “true signal” by averaging the intensity from maximum intensity projections of 3–4 representative z-slices, including EVL signals when necessary (i.e. Myosin-II:GFP). Background pixel intensity (avoiding membrane signal) was subtracted from the average values. Images were analysed using FIJI software41 and presenting intensity in Fire LUT colour code when necessary (values, 0–255).

Statistics

To test for significance between mean values, student’s t-test p values were calculated using non-parametric Mann-Whitney post-test (Matlab, Cambridge, UK statistic toolbox and Graph Pad, La Jolla, CA, USA). We used a probability of 0.05 for significance. All the error bars shown in figures are SEM (standard error of the mean). For each experiment, we normally used 3–6 embryos. Graphical representations were performed using GraphPad Prism programme.

Additional information

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

Change history

  • 17 May 2019

    A correction to this article has been published and is linked from the HTML and PDF versions of this paper. The error has been fixed in the paper.

References

  1. 1.

    Keller, R. & Shook, D. The bending of cell sheets-from folding to rolling. Bmc Biol. 9, 90 (2011).

  2. 2.

    Nikolopoulou, E., Galea, G. L., Rolo, A., Greene, N. D. & Copp, A. J. Neural tube closure: cellular, molecular and biomechanical mechanisms. Development 144, 552–566 (2017).

  3. 3.

    Heer, N. C. & Martin, A. C. Tension, contraction and tissue morphogenesis. Development 144, 4249–4260 (2017).

  4. 4.

    Martin, A. C. & Goldstein, B. Apical constriction: themes and variations on a cellular mechanism driving morphogenesis. Development 141, 1987–1998 (2014).

  5. 5.

    Sweeton, D., Parks, S., Costa, M. & Wieschaus, E. Gastrulation in Drosophila: the formation of the ventral furrow and posterior midgut invaginations. Development 112, 775–89 (1991).

  6. 6.

    Leptin, M. Drosophila gastrulation: from pattern formation to morphogenesis. Annu. Rev. Cell Dev. Biol. 11, 189–212 (1995).

  7. 7.

    Martin, A. C., Kaschube, M. & Wieschaus, E. F. Pulsed contractions of an actin-myosin network drive apical constriction. Nature 457, 495–4999 (2009).

  8. 8.

    Gelbart, M. A. et al. Volume conservation principle involved in cell lengthening and nucleus movement during tissue morphogenesis. Proc. Natl. Acad. Sci. USA 109, 19298–19303 (2012).

  9. 9.

    Martin, A. C., Gelbart, M., Fernandez-Gonzalez, R., Kaschube, M. & Wieschaus, E. F. Integration of contractile forces during tissue invagination. J. Cell Biol. 188, 735–749 (2010).

  10. 10.

    Araya, C., Ward, L. C., Girdler, G. C. & Miranda, M. Coordinating cell and tissue behavior during zebrafish neural tube morphogenesis. Dev. Dyn. 245, 197–208 (2016).

  11. 11.

    Clarke, J. Role of polarized cell divisions in zebrafish neural tube formation. Curr. Opin. Neurobiol. 2, 134–138 (2009).

  12. 12.

    Tawk, M. et al. A mirror-symmetric cell division that orchestrates neuroepithelial morphogenesis. Nature 446, 797–800 (2007).

  13. 13.

    Quesada-Hernández, E. et al. Stereotypical cell division orientation controls neural rod midline formation in zebrafish. Curr. Biol. 20, 1966–1972 (2010).

  14. 14.

    Ciruna, B., Jenny, A., Lee, D., Mlodzik, M. & Schier, A. F. Planar cell polarity signalling couples cell division and morphogenesis during neurulation. Nature 439, 220–224 (2006).

  15. 15.

    Araya, C. et al. Mesoderm is required for coordinated cell movements within zebrafish neural plate in vivo. Neur. Dev. 9, 9 (2014).

  16. 16.

    Araya, C., Carmona-Fontaine, C. & Clarke, J. D. Extracellular matrix couples the convergence movements of mesoderm and neural plate during the early stages of neurulation. Dev. Dyn. 245, 580–589 (2016).

  17. 17.

    Buckley, C. E. et al. Mirror-symmetric microtubule assembly and cell interactions drive lumen formation in the zebrafish neural rod. EMBO Journal 32, 30–44 (2013).

  18. 18.

    Yang, X., Zou, J., Hyde, D. R., Davidson, L. A. & Wei, X. Stepwise maturation of apicobasal polarity of the neuroepithelium is essential for vertebrate neurulation. J. Neurosc. 29, 11426–11440 (2009).

  19. 19.

    Hong, E. & Brewster, R. N-cadherin is required for the polarized cell behaviors that drive neurulation in the zebrafish. Development 133, 3895–3905 (2006).

  20. 20.

    Haigo, S. L., Hildebrand, J. D., Harland, R. M. & Wallingford, J. B. Shroom induces apical constriction and is required for hingepoint formation during neural tube closure. Curr. Biol. 13, 2125–2137 (2003).

  21. 21.

    Hildebrand, J. D. Shroom regulates epithelial cell shape via the apical positioning of an actomyosin network. J. Cell Sci. 118, 5191–51203 (2015).

  22. 22.

    Lele, Z. et al. parachute/n-cadherin is required for morphogenesis and maintained integrity of the zebrafish neural tube. Development 129, 3281–3294 (2002).

  23. 23.

    Faure, E. et al. A workflow to process 3D+ time microscopy images of developing organisms and reconstruct their cell lineage. Nat. Commun. 7, 8674 (2016).

  24. 24.

    Maître, J. L. et al. Adhesion functions in cell sorting by mechanically coupling the cortices of adhering cells. Science 338, 253–256 (2012).

  25. 25.

    Behrndt, M. et al. Forces driving epithelial spreading in zebrafish gastrulation. Science 338, 257–260 (2012).

  26. 26.

    Limouze, J., Straight, A. F., Mitchison, T. & Sellers, J. R. Specificity of blebbistatin, an inhibitor of myosin II. Musc. Res. Cell Mot. 25, 337–241 (2004).

  27. 27.

    Borghi, N. et al. E-cadherin is under constitutive actomyosin-generated tension that is increased at cell-cell contacts upon externally applied stretch. Proc. Natl. Acad. Sci. USA 109, 12568–12573 (2012).

  28. 28.

    Dickinson, D. J., Robinson, D. N., Nelson, W. J. & Weis, W. I. α-catenin and IQGAP regulate myosin localisation to control epithelial tube morphogenesis in Dictyostelium. Dev. Cell 23, 533–546 (2016).

  29. 29.

    Yonemura, S., Wada, Y., Watanabe, T., Nagafuchi, A. & Shibata, M. alpha-Catenin as a tension transducer that induces adherens junction development. Nat. Cell Biol. 12, 533–542 (2010).

  30. 30.

    Revenu, C. et al. Quantitative cell polarity imaging defines leader-to-follower transitions during collective migration and the key role of microtubule-dependent adherens junction formation. Development 141, 1282–1291 (2014).

  31. 31.

    Khmelinskii, A. Tandem fluorescent protein timers for in vivo analysis of protein dynamics. Nat. Biotech. 30, 708–714 (2012).

  32. 32.

    Pouille, P. A., Ahmadi, P., Brunet, A. C. & Farge, E. Mechanical signals trigger Myosin II redistribution and mesoderm invagination in Drosophila embryos. Sci. Sig. 2, 66 (2009).

  33. 33.

    Dawes-Hoang, R. E. et al. Folded gastrulation, cell shape change and the control of myosin localization. Development 132, 4165–4178 (2005).

  34. 34.

    Chan, E. H., Chavadimane Shivakumar, P., Clément, R., Laugier, E. & Lenne, P. F. Patterned cortical tension mediated by N-cadherin controls cell geometric order in the Drosophila eye. Elife 6, e22796 (2017).

  35. 35.

    Nandadasa, S., Tao, Q., Menon, N. R. & Heasman, J. & Wylie, C. N- and E-cadherins in Xenopus are specifically required in the neural and non-neural ectoderm, respectively, for F-actin assembly and morphogenetic movements. Development 136, 1327–138 (2009).

  36. 36.

    Radice, G. L. Developmental defects in mouse embryos lacking N-cadherin. Dev. Biol. 181, 64–78 (1997).

  37. 37.

    Morita, H. et al. Nectin-2 and N-cadherin interact through extracellular domains and induce apical accumulation of F-actin in apical constriction of Xenopus neural tube morphogenesis. Development 137, 1315–1325 (2010).

  38. 38.

    Lee, H. Y. & Nagele, R. G. Studies on the mechanisms of neurulation in the chick: interrelationship of contractile proteins, microfilaments, and the shape of neuroepithelial cells. J. Exp. Zool. 235, 205–215 (1985).

  39. 39.

    Rolo, A., Skoglund, P. & Keller, R. Morphogenetic movements driving neural tube closure in Xenopus require myosin IIB. Dev. Biol. 327, 327–338 (2009).

  40. 40.

    Ossipova, O. et al. Role of Rab11 in planar cell polarity and apical constriction during vertebrate neural tube closure. Nat. Commun. 5, 3734 (2014).

  41. 41.

    Escuin, S. et al. Rho-kinase-dependent actin turnover and actomyosin disassembly are necessary for mouse spinal neural tube closure. J. Cell. Sci. 128, 2468–2481 (2015).

  42. 42.

    Kasthuri, N. et al. Saturated reconstruction of a volume of neocortex. Cell 162, 648–661 (2015).

  43. 43.

    Westerfield, M. The Zebrafish Book. A guide for the laboratory use of Zebrafish (Danio rerio). (University of Oregon Press, 2000).

  44. 44.

    Kimmel, C. B., Ballard, W. W., Kimmel, S. R., Ullmann, B. & Schilling, T. F. Stages of embryonic development of the zebrafish. Dev. Dyn. 203, 253–310 (1995).

  45. 45.

    Schindelin, J. et al. Fiji: an open-source platform for biological-image analysis. Nat. Methods 9, 676–682 (2012).

  46. 46.

    Arganda-Carreras, I. et al. Trainable Weka Segmentation: a machine learning tool for microscopy pixel classification, Bioinformatics (Oxford Univ Press, 2017).

Download references

Acknowledgements

We thank members of Araya’s lab for helpful discussion and comments on the manuscript. This work was supported by grants from Dirección de Investigación y Desarrollo UACh S-201613 to CA and LC, FONDECYT 11161033; FONDEQUIP EQM140119; ACT1402; P09–015-F; CORFO (16CTTS-66390); DAAD (57220037, 57168868) to MC, CONICYT/ECOS-SUD C13B03 to CA, TS and NP, and Wellcome Trust to JC.

Author information

Affiliations

  1. Laboratory of Developmental Biology, Instituto de Ciencias Marinas y Limnológicas, Facultad de Ciencias, Universidad Austral de Chile, Campus Isla Teja, 5090000, Valdivia, Chile

    • Claudio Araya
    • , Hanna-Maria Häkkinen
    •  & Luis Carcamo
  2. Centro Interdisciplinario de Estudios del Sistema Nervioso (CISNe), UACh, Valdivia, Chile

    • Claudio Araya
  3. Anatomy and Developmental Biology Program, Institute of Biomedical Sciences, Faculty of Medicine, Universidad de Chile, PO Box 70031, Santiago, Chile

    • Mauricio Cerda
  4. Biomedical Neuroscience Institute, Independencia, 1027, Santiago, Chile

    • Mauricio Cerda
  5. UPS3611 Complex Systems Institute Paris Ile-de-France (ISC-PIF), CNRS, Paris, France

    • Thierry Savy
    •  & Nadine Peyriéras
  6. USR3695 BioEmergences, CNRS, Paris-Saclay University, Gif-sur- Yvette, France

    • Thierry Savy
    •  & Nadine Peyriéras
  7. Centre for Developmental Neurobiology, Institute of Psychiatry Psychology and Neuroscience, King’s College London, New Hunt’s House, Guy’s Campus, London, SE1 1UL, United Kingdom

    • Christopher Rookyard
    •  & Jonathan D. W. Clarke

Authors

  1. Search for Claudio Araya in:

  2. Search for Hanna-Maria Häkkinen in:

  3. Search for Luis Carcamo in:

  4. Search for Mauricio Cerda in:

  5. Search for Thierry Savy in:

  6. Search for Christopher Rookyard in:

  7. Search for Nadine Peyriéras in:

  8. Search for Jonathan D. W. Clarke in:

Contributions

C.A. conceived and designed the study. C.A. and J.C. analysed all experimental results. H.H. helped to analyse data from Figs 1 and 5 and generated time-lapses in Figs 3 and 5. M.C. implemented algorithm to analyse Figs 2, 3 and 7. L.C. helped to analyse Figs 1, 2 and 7. T.S. generated Bioemergence and MOVIT platforms and helped to analyse data from Fig. 1. C.R. helped to generate data for Fig. 3 and analyse data for Fig. 3. N.P. helped to generate time-lapse data from Figs 1 and 5 and supervised Bioemergence/MOVIT analysis. C.A., and H.H. carried out the experiments. C.A. and J.C. wrote and revised the manuscript. All authors reviewed the manuscript.

Competing Interests

The authors declare no competing interests.

Corresponding author

Correspondence to Claudio Araya.

Supplementary information

About this article

Publication history

Received

Accepted

Published

DOI

https://doi.org/10.1038/s41598-018-38455-w

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.