Research Article

Coordination of progenitor specification and growth in mouse and chick spinal cord

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Science  26 Sep 2014:
Vol. 345, Issue 6204, 1254927
DOI: 10.1126/science.1254927

Structured Abstract

Introduction

The hallmarks of development are tissue growth and the generation of cell diversity, resulting in reproducibly patterned animals. Yet, how growth and cell fate specification are coordinated to determine the variety of cell types and the proportions of their populations is not well understood. The specification of cell types can be controlled by long-range signals, called morphogens. In some tissues, the shape of morphogen gradients is controlled to match the rate at which the tissue grows, which may keep the pattern proportional to the overall tissue size. To understand whether a similar strategy applies to the patterning of the spinal cord, we measured growth and cell fate specification in chick and mouse embryos of normal size, as well as mutant mice of smaller size.

Graphic

Growth and patterning of the spinal cord. Progenitors are organized in a striped pattern, revealed by their gene expression. In animals of different size, the pattern changes in the same way as the spinal cord grows. This is controlled sequentially, first by progenitor specification by opposing morphogen gradients (bottom left), then by cell-type–specific differentiation resulting in differently shaped clones (green, bottom right).

Rationale

Morphogen gradients emanating from the dorsal and ventral sides of the spinal cord establish a striped pattern of gene expression in neural progenitors along the dorsoventral axis. Ventrally, Sonic Hedgehog (Shh) is the key morphogen. As the tissue grows in size, the levels of Shh activity in progenitors decrease and are not constant at progenitor domain boundaries. This prompted us to examine whether growth contributed to pattern formation. To this end, we measured the four parameters that control the number of progenitors in a domain: (i) cell proliferation, (ii) cell death, (iii) terminal differentiation of progenitors into postmitotic neurons, and (iv) switches in cell identity—morphogen-driven changes in gene expression respecifying one progenitor type into another.

Results

Unlike systems in which pattern is proportional to size, we found that the relative dorsoventral sizes of neural progenitor domains change continuously during development . These changes in proportions are conserved between mouse, chick, and smaller mouse mutants. Because the proliferation rate of progenitors was spatially uniform and cell death was negligible, neither of these processes could account for the dynamics of pattern formation. Instead, the data revealed two distinct phases of spinal cord development. Initially, the influence of the morphogens dominates, and switches in cell identity establish pattern. During the second phase, domain-specific differentiation rates emerge, causing changes in the relative proportions of progenitor cell populations. Clonal analysis indicated that this effect is anisotropic: Differentiation affects dorsoventral and apicobasal, but not anterioposterior, domain growth. The outcome is that different domains grow in register along the anterioposterior axis. Consistent with the two-phase model, the switches in cell fate and the sensitivity to changes in morphogen signaling decrease as development proceeds. Conversely, experimentally flattening the difference in differentiation rate between domains during the second phase alters pattern.

Conclusion

The data reveal two phases of neural tube development and show that sequential control of progenitor cell specification and differentiation elaborates pattern without requiring signaling gradients to expand as tissues grow. Control of the differentiation rate is likely to contribute to pattern formation in other tissues. Furthermore, the domain-specific regulation of the differentiation rates could suggest a means to achieve reproducible development despite differences in individual size.

Differentiation rates regulate pool sizes

Even though a basketball player is bigger than a gymnast, their neural tubes are organized in the same way. Studying chick and mouse embryos, Kicheva et al. show that rates of cell differentiation are key (see the Perspective by Pourquie). In a two-phase process, signaling sweeps through the neural tube early on to establish some aspects of cell fate, but later, pools of progenitor cells take on their own regulation. A progenitor that differentiates is no longer a progenitor, and thus the rate of differentiation determines the size of the progenitor pool. The relative sizes of progenitor pools shift as development progresses, to build the spinal cord so that everyone, large or small, has the right proportion of each component.

Science, this issue p. 10.1126/science.1254927; see also p. 1565

Abstract

Development requires tissue growth as well as cell diversification. To address how these processes are coordinated, we analyzed the development of molecularly distinct domains of neural progenitors in the mouse and chick neural tube. We show that during development, these domains undergo changes in size that do not scale with changes in overall tissue size. Our data show that domain proportions are first established by opposing morphogen gradients and subsequently controlled by domain-specific regulation of differentiation rate but not differences in proliferation rate. Regulation of differentiation rate is key to maintaining domain proportions while accommodating both intra- and interspecies variations in size. Thus, the sequential control of progenitor specification and differentiation elaborates pattern without requiring that signaling gradients grow as tissues expand.

In most developing tissues, the spatiotemporal pattern of gene expression is generated by gene regulatory networks controlled by morphogens (13). This happens at the same time as the tissue grows. Understanding how growth and cell fate specification are coordinated within a tissue to determine the relative proportions of different cell types is of central importance. In some tissues, such as the Drosophila wing disc (4), early embryo (5, 6), and Xenopus gastrula (7, 8) the scaling of the morphogen gradient with tissue size determines the underlying pattern. Whether similar strategies apply to all tissues is unclear.

In the vertebrate neural tube, the dorsoventral pattern of neural progenitors is specified by 13 spatially distinct transcriptional states (9). These are encoded by the combinatorial expression of transcription factors in response to opposing morphogen gradients—ventrally secreted sonic hedgehog (Shh) and dorsally secreted bone morphogenetic protein (BMP) and Wnt (Fig. 1A). In mouse, the graded activation of Gli effectors downstream of Shh undergoes temporal adaptation after reaching a peak at embryonic day 9 (E9) (10, 11); hence, it does not correlate with tissue size. Moreover, Gli activity levels are not constant at the boundaries of the target genes Nkx2.2 and Olig2 over time (11). Although the transcriptional network is at least in part responsible for this lack of correspondence between Shh signaling and target gene boundary positions (11), anisotropic tissue growth might also affect progenitor domain sizes.

Fig. 1 Quantification of neural tube pattern and size over time.

(A) Markers used to partition the neural tube: floorplate FP (Arx+), motor neuron progenitors pMN (Olig2+), ventral interneuron progenitors p3 (marked by the absence of Olig2 and Arx), intermediate interneuron progenitors pI (absence of Olig2 and Pax3), and dorsal interneuron progenitors pD (Pax3+). (B) E10.5 transverse section and markers used for measuring the number of progenitors. Domains are outlined in white. Sox2 was used to determine the basal extent. Scale bars, 50 μm. (C) Schematic of neuroepithelium organization illustrating different apicobasal lengths of the progenitor nuclei (gray) layer. (D) Dorsoventral positions of indicated boundaries relative to the ventral midline. Time (hph) corresponds to twice the number of somites. Upper x axis, embryonic day (table S1). (E) The dorsoventral boundary positions relative to total dorsoventral length change over time. (F) Mean apicobasal length of the Sox2+ progenitor layer. (G) Mean number of Sox2+ nuclei per hemi-section in each domain based on the markers in (B), representing dorsoventral domain size in units of cells. (H) Number of progenitors in G relative to the total. Error bars, mean ± SEM. For sample sizes, see table S2.

During development, neural progenitors proliferate, and this is counterbalanced by their terminal differentiation into neurons, which migrate out of the epithelial progenitor layer (12) (Fig. 1, A to C). As a result, the neural tube grows anterioposteriorly, dorsoventrally, and apicobasally, but it is not known how much growth occurs in each dimension. Here, we assess the contribution of morphogen signaling and anisotropic growth to pattern formation and define how pattern adapts to size variability between individuals by measuring the growth characteristics of mouse and chick embryos.

Pattern does not scale with tissue size

To characterize how pattern is specified relative to neural tube growth and Shh signaling, we focused on five progenitor domains that partition the dorsoventral axis (Fig. 1, A and B). We collected transverse sections from the forelimb level of mouse embryos adjacent to somites 7 to 10 between E8 [~10 hours post headfold stage (hph)] and E11.5 [~90 hph, the onset of gliogenesis (13)].

During this period, the dorsoventral length of the neural tube increases by a factor of ~4, and the domain boundary positions shift with respect to the ventral midline (Fig. 1D). Before E9, these shifts result, at least in part, from the progressive induction of progenitor domains (11, 14). Moreover, the relative positions of boundaries (as a fraction of the total length) are not constant but also change (Fig. 1E). This could result from changes in cell shape, size, or number. Indeed, the apicobasal thickness of the single-cell layer of Sox2-positive (Sox2+) progenitors changes over time in a domain-specific manner (Fig. 1F), suggesting regulated changes in cell shape. Nevertheless, all progenitors attach to the apical surface; hence, the number of Sox2+ nuclei per section provides a measure of dorsoventral size in units of cells, independent of cell shape (Fig. 1, C and G, and fig. S1). The relative sizes of progenitor domains measured in this way change during development (Fig. 1H), showing that dorsoventral pattern does not change linearly with the overall neural tube size.

In systems where pattern scales with growing tissue size, domain proportions are also preserved between individuals of varying size (48). To study how neural tube pattern accommodates variations in size between individuals, we used a mouse Minute strain that is heterozygous for a deletion in Rpl24 (15), a large ribosomal subunit component. These smaller Minute mice have no apparent locomotion defects, yet they have 19 ± 10% fewer progenitors than wild-type littermates at E11.5 (Fig. 2, A, B, and D), and they produce 60 ± 7% fewer postmitotic neurons (Student’s t test, P < 0.05) (Fig. 2E). Although the neural tube size of Rpl24(Bst)/+ embryos is noticeably smaller than controls after 30 hph, the progenitor domain proportions follow a similar pattern of development [Fig. 2F, 95% confidence intervals (CIs)], and at 90 hph the mice end up with a similarly patterned, albeit smaller, neural tube.

Fig. 2 Comparison of wild-type, Rpl24(Bst)/+ mouse and chick embryos.

(A to C′′′) Transverse sections immunostained for Pax3, Olig2, Nkx2.2, and Arx. Identical magnification; scale bars, 50 μm. (D) Progenitors per hemisection in wild-type (circles, light shades) versus Rpl24(Bst)/+ (diamonds, dark shades) mouse embryos. The larger, more dorsal domains are plotted on the left panel; the smaller, more ventral domains are on the right. (E) Postmitotic neurons in Rpl24(Bst)/+ versus wild-type embryos [legend as in (D)]. (F) The progenitors per hemisection in each domain relative to the total number change in a similar way between Rpl24(Bst)/+ and control. (G) Wild-type mouse (circles, light shades) versus chick (diamonds, dark shades) comparison as in (F). The chick data set was registered to mouse, so the somite next to which the measurements were made was generated at equivalent corresponding time (table S1). [(D) to (G)] Error bars, mean ± SEM. Shaded areas, 95% CIs. For sample sizes, see table S2.

Furthermore, by comparing pattern at equivalent stages and anterioposterior positions, we found that the dynamics of progenitor domain proportions are also conserved between the mouse and chick neural tube (Fig. 2, C and G). Together, this indicates that the dorsoventral domain proportions change during development via a conserved sequence, which is independent of the size of the animal.

Proliferation is uniform but differentiation is cell-type specific

How is the temporal sequence of progenitor domain proportions controlled? Four factors control the number of progenitors in a domain: (i) cell proliferation, (ii) apoptosis, (iii) terminal differentiation leading to cell cycle exit and delamination, and (iv) switches in cell identity—i.e., changes in gene expression that respecify one progenitor type into another. It is possible that spatially nonuniform growth, driven by nonuniform differentiation, proliferation, or apoptosis, together with a memory of the transcriptional state (11), could account for the change in proportions independent of signaling. Alternatively, switches in gene expression could increase the size of one progenitor pool at the expense of another. To distinguish between these possibilities, we measured the growth parameters of the mouse spinal cord.

We measured the proliferation rate using sequential pulse labeling with two thymidine analogs, iododeoxyuridine (IdU) and bromodeoxyuridine (BrdU) (16, 17). The fraction of Sox2+ progenitors labeled only with IdU during the 1.5-hour pulse (IduLI) is directly related to the proliferation rate λ (fig. S2, A and B) (see materials and methods). We also measured the mitotic index (MI), the fraction of phospho-histone H3–labeled Sox2+ progenitors, in combination with progenitor domain markers (Fig. 3A and fig. S2C). The MI/IduLI ratio allows us to determine the duration of mitosis, 27.7 ± 11.3 min, and the domain-specific λ from the MI (see materials and methods). Both approaches indicate that the proliferation rate is uniform in all domains except the Shh-producing floorplate [analysis of variance (ANOVA), P > 0.05 for all stages, excluding floorplate].

Fig. 3 Mouse growth parameters.

(A) The proliferation rate determined from MI in sections is similar (ANOVA, P > 0.05) for all domains except FP. (B) Fraction of Caspase3+ Sox2+ progenitors. (C) Differentiation rate determined from transverse sections. (D and E) G1 length relative to the total cell cycle length (D) estimated from the fraction of S/G2/M-Fucci negative progenitors (E). Asterisks, one-way ANOVA across domains; P < 0.05. (F) Neural tube geometry and flat-mount preparation. Colors as in Fig. 1A; labeled cells, black. (G) Maximum projection though a flat mount, imaged between somites 6 to 13. Dorsal up, anterior left. Clones marked by EYFP expression. (H) Coordinates of the EYFP+ cells in (G). Clonal groups are color-coded. (I) Example clone. Cell coordinates (dots) and typical cell diameter (circles). First and second eigenvectors of the second moment matrix are shown by red and blue lines, respectively. Clone orientation angle relative to the anterioposterior axis, θ. Anterioposterior and dorsoventral clone spread, dashed lines. (J) The density distribution of pD, pI, and p3 clone orientation angles is non uniform (χ2 test, P < 0.05). (K to M) Mean dorsoventral (K), anterioposterior (L) clone spread and ratio of the mean anterioposterior/dorsoventral spread (M). Asterisks, Student’s t test; P < 0.05. (N) Progenitors in a hemisection with anterioposterior length = 1 cell at t = 10 hours and increasing in three dimensions as calculated from the clonal and section data (see the supplementary materials). [(A) to (N)] Error bars, mean ± SEM. For sample sizes, see table S2.

The proliferation rate is approximately constant before 40 hph (~0.08 hour−1, equivalent to a cell cycle length of ~9 hours) and decreases at later times (Fig. 3A). In parallel, the duration of the G1 phase of the cell cycle increases relative to the cell cycle length (Fig. 3, D and E, and fig. S3, A and B), but this increase is not spatially uniform. Thus, while the overall cell cycle length is similar between the motor neuron progenitor (pMN) and dorsal progenitor (pD) domains at 60 hph, their cell cycle phase distribution is different. This raises the possibility that a homeostatic control mechanism could coordinate G1/S and G2/M progression to maintain uniform proliferation (18).

Because the proliferation rate is spatially uniform, it cannot cause the observed changes in domain proportions. Furthermore, the fraction of apoptotic progenitors is less than 0.5% (Fig. 3B), and cleaved Caspase 3, used to detect apoptosis, can persist for more than 2 hours in neural tissues (19). Thus, the rate of progenitor apoptosis (<0.0025 hour−1) is negligible compared with the proliferation rate and does not significantly affect the domain growth rates.

To measure the differentiation rate, we quantified the number of Sox2-negative (Sox2) postmitotic neurons generated from each progenitor domain before E11 in transverse sections (Fig. 2E). We defined the differentiation rate as the number of neurons produced per unit time relative to the size of the progenitor domain, which reflects the probability of progenitors to exit the cell cycle. The differentiation rate was not constant over time. For MNs, a maximum rate was reached at 60 hph (Fig. 3C). For the intermediate and dorsal interneurons, peak differentiation occurred at ~100 hph (fig. S1, G and H). The differentiation rate differed between domains: Before 90 hph, pMNs differentiated at a higher rate (reaching 0.15 hour−1) than the ventral interneuron progenitors (p3) and more dorsal regions (<0.03 hour−1). The increase in differentiation rate of the pMN domain happens at the same time (40 hph) as the size of the domain starts decreasing (Fig. 1G). Thus, differential net growth rates resulting from cell-type–specific differences in the differentiation rate could be the main factor influencing domain size proportions.

Progenitor domain growth is anisotropic

The measurements of the proliferation and differentiation rates can be used to test whether these are sufficient to account for the temporal changes in domain sizes. If this is the case, cell identity does not switch (i.e., the respecification rate is zero) and the change in number of progenitors is given by:Embedded Image (1)where P is the number of progenitors, Embedded Image is the temporal change in progenitor number, λ is the proliferation rate, and γ is the differentiation rate; all of these change over time. If growth explains the dynamics of patterning, the measured net growth rate Embedded Image should be equal to the relative increase in progenitor number, Embedded Image.

To measure Embedded Image, in addition to the dorsoventral and apicobasal sizes, it is necessary to measure the change in progenitor number along the anterioposterior axis (Fig. 3F). To do this, we used a tamoxifen-inducible system, whereby CreERT2 knocked into the Sox1 locus (fig. S4A) excises a loxP-flanked transcription stop sequence resulting in the expression of enhanced yellow fluorescent protein (EYFP). With low tamoxifen doses, EYFP expression was activated in individual progenitors at E9.5 (Fig. 3, F and G). Forty-eight hours later, the sizes of the resulting clones were consistent with the measured proliferation and differentiation rate (fig. S4B). The shape of the clones relates the anterioposterior growth rate to the dorsoventral growth rate calculated from Fig. 1G (see the supplementary materials). This provides a measurement of the growth of a defined volume of the brachial neural tube (Fig. 3N).

Most labeled cells formed coherent groups, suggesting that cell rearrangements after E9.5 are limited (Fig. 3G) (20, 21). The clones often had irregular shape; to quantify these, we used the second moment matrix of cell coordinates (Fig. 3, G to I, and fig. S4). For all but the pMN domain, clones were elongated along the dorsoventral axis, and their orientation was dorsoventrally biased (Fig. 3, J to M, and fig. S4E). By contrast, pMN clones were on average isotropic. Furthermore, although the dorsoventral spread of clones differed between domains, they had a similar anterioposterior spread (Fig. 3, K and L). This implies that mechanical or molecular constraints ensure equivalent anterioposterior growth across the tissue, whereas the dorsoventral growth rates are position and cell-type dependent.

Using these data, we calculated the relative increase in progenitor number in three dimensions Embedded Image (see the supplementary materials) and directly compared it to the net growth rate (Eq. 1). To validate the measurements, Embedded Image was compared to Embedded Image of the whole tissue, because respecification is irrelevant for the total number of progenitors and Eq. 1 must hold true. This is indeed the case (Fig. 4A), except at 20 hph, which corresponds to the time neural crest delaminates from the neural tube (22). Thus Embedded Image decreases over time, indicating that the number of progenitors comprising the brachial spinal cord increases at a decelerating rate, by ~0.08 hour−1 at 10 hph and by ~0.02 hour−1 at later stages.

Fig. 4 Growth accounts for changes in pattern at later times.

(A to F) Relative temporal increase in progenitor number in all dimensions (Embedded Image, solid lines) compared to the net growth rate [Embedded Image, dashed lines] for each domain. (G) Two-phase model of neural tube development. (H and I) Comparison of mouse (circles) to chick (diamonds) mean proliferation rate (H) and differentiation rate (I). (J to L) Comparison of the mean proliferation rate (J), differentiation rate (K), and fraction of Caspase3+ progenitors (L) between wild-type mouse (solid lines) and Rpl24Bst/+ embryos (dashed lines). [(A) to (L)] Shaded areas, 95% CIs. Error bars, mean ± SEM. For sample sizes, see table S2.

A two-phase model for neural tube pattern formation

We analyzed individual progenitor domains (Fig. 4, B to F). Before ~40 hph there were discrepancies between Embedded Image and Embedded Image: The pD and pI domains expanded less than predicted by their growth rate (Fig. 4, B and C), whereas the ventral domains, which are progressively induced in progenitors that initially had pI identity, expanded more (Fig. 4, D to F) (23). By contrast, after ~40 hph, there was a good correspondence between the relative increase in progenitor number of each domain and the net growth rate. Thus after ~40 hph, the changes in domain size can be accounted for by proliferation and differentiation, suggesting that the net respecification rate is negligible. Consistent with this, 92.1% of the clones in our data set consisted of a single progenitor type (fig. S4C), indicating that cell identity changes within a lineage are infrequent after E9.5. Because proliferation is spatially uniform (Fig. 3A), the differences in Embedded Image between domains, and hence the changes in proportions, must be accounted for by cell-type–specific differences in the differentiation rates (Fig. 3C).

Together, these observations indicate that neural tube patterning can be viewed as a two-phase process: an early phase (before ~40 hph), where there is no differentiation and progenitor identity is actively specified, and a late phase, where progenitor identity does not change significantly and the relative domain sizes are controlled by cell-type–specific differentiation rates (Figs. 3C and 4G).

How are reproducible domain proportions between individuals of different sizes and species achieved during the second phase? In the absence of switches in cell identity and given a spatially uniform proliferation rate, the number of progenitors in any two domains (e.g., the dorsal half Pd, and the ventral half Pv) would each change in accordance to Eq. 1. Hence, the ratio of progenitors in the two domains would change asEmbedded Image (2)where Embedded Image and Embedded Image are the time-dependent differentiation rates in the two domains. Therefore, as long as two individuals have the same differences between the differentiation rates of domains over time, regardless of the absolute tissue size, their progenitor domain proportions would change in the same way. Thus, reproducible pattern proportions are achieved if four criteria are satisfied: (i) absence of net cell identity changes, (ii) conserved cell-type–specific differences in the differentiation rate, (iii) conserved temporal dynamics of the differentiation rate in different individuals, and (iv) reproducible initial proportions established during the early phase.

Because the chick neural tube shows similar changes in proportions as mouse, we hypothesized that the two-phase model also applies to this species and the differentiation rate dynamics are preserved. To test this hypothesis, we determined the change in progenitor number in chick. Photoconverting photoswitchable cyan fluorescent protein (PS-CFP) in a stripe of cells in the neural tube of transfected embryos indicated a homogenous anterioposterior growth rate across domains (fig. S5). The proliferation rate, measured from the mitotic index (Fig. 4H, fig. S2, F and G, and fig. S6) and IdU/BrdU incorporation (fig. S2, D and E), was spatially uniform, except in the floorplate (fig. S2G), and consistent with previous studies (24, 25). At later stages, the proliferation rate in chick was lower than in mouse (Fig. 4H), in agreement with the smaller size of the chick neural tube (fig. S1, D to F). The differentiation rate was cell-type–dependent, highest in the pMN domain, and undergoing similar temporal changes to mouse (Fig. 4I). Finally, comparing Embedded Image to Embedded Image (fig. S7) supported the idea that pattern formation in the chick neural tube proceeds in a similar biphasic way as mouse. The similarity in the differentiation dynamics in chick and mouse explains the overall similarity in pattern proportions.

The two-phase model was also consistent with the proportion dynamics observed in Minute mouse embryos. In these embryos, the proliferation rate was unaffected (Fig. 4J) (26), whereas the fraction of apoptotic cells was higher, particularly at later stages, explaining the smaller progenitor number compared with controls (Fig. 4L). The pMN differentiation rate in Rpl24(Bst)/+ embryos was consistent with the observed changes in proportions (Fig. 4K). Together, these data indicate that pattern formation in the Rpl24(Bst)/+ embryos is consistent with the two-phase model and that the preserved differentiation rate dynamics can account for the reproducible pattern of these mice relative to control.

Experimental validation of the two-phase model

The two-phase model for neural tube patterning makes several predictions. First, the rate of respecification of progenitor identity should decrease significantly at late developmental stages. To test this prediction, we measured the rate of Olig2 identity switching at different stages using a tamoxifen-inducible Olig2KICreER line (27) (Fig. 5, A to C). As predicted, the rate of Olig2 identity change decreases from 0.034 per hour−1 to 0.004 hour−1 the later the Cre activity was induced (Fig. 5C) (ANOVA, P < 0.05). Although this decrease occurs in parallel with the increase of G1 phase length (Fig. 3D), analysis of the cell cycle phase distribution in cells undergoing a Olig2-Nkx2.2 switch, marked by the coexpression of both genes, suggests that respecification can occur at any time of the cell cycle (Fig. 5D and fig. S3C).

Fig. 5 Validation of the two-phase model.

(A and B) Olig2KICreER-induced EGFP expression (green) from the indicated times. Olig2 immunostaining, red. (C) Quantification of rate of loss of Olig2 identity. Period of Olig2KICreER activity, horizontal gray bars. (D) Distribution of cell cycle phases (based on S/G2/M-Fucci expression) in progenitors expressing Olig2, Nkx2.2, or both (Fig. 3E). (E to J) Mouse embryo culture at the indicated stages without [(E) to (G)] or with [(H) to (J)] 5 μM cyclopamine. Sections in (H) and (I) are from the same embryos as (E) and (F), respectively. (K) Quantification of the experimental conditions in (E) to (J). The difference in mean boundary position between control and cyclopamine treatment was significant (Student’s t test, P < 0.05) for all boundaries at E8.5 and 3/6 at E9.5-brachial. The different boundaries were measured in independent experiments. Cyclopamine concentration for Nkx6.1 boundary in E8.5 is 3 μM. (L and M) pSmad and GBS-GFP mean fluorescence intensity versus relative distance from the ventral midline at different stages. (N) Profiles in (L) and (M) were normalized to the maximum intensity in each time series and summed to give combined pSmad and GBS-GFP activity. Error bars, mean ± SEM. For sample sizes, see table S2.

The decrease in Olig2 respecification rate, despite the continuing changes in Gli activity, raises the possibility that progenitors become less sensitive to Shh signaling. To investigate this, we reduced Shh signaling using moderate concentrations of the inhibitor cyclopamine at different stages of development in cultured mouse embryos (Fig. 5, E to K). The domain boundary positions had little sensitivity to 5 μM of cyclopamine at E9.5 of development, but shifted significantly at earlier stages (Fig. 5K). Moreover, the time at which gene expression becomes robust to experimental inhibition of Shh signaling coincided with the time at which Olig2 identity changes decreased (Fig. 5C) and the transition between the two phases of development (Fig. 4G).

Examination of the dynamics of Gli activity indicated that the transition between the two phases of pattern formation occurred when Gli activity levels were close to maximal (Fig. 5L and fig. S8) (11). The BMP signaling levels measured by immunostaining for phosphorylated Smad1/5/8 showed similar temporal dynamics (Fig. 5M and fig. S8). These measurements revealed that the maximum ranges and greatest overlap between the two gradients were before 30 hph (Fig. 5N). Thus, progenitors are exposed to the highest levels of BMP and Shh signaling before 30 hph. This suggests that the subsequent decrease in BMP and Shh activity permits the stabilization of lineages, in part through the action of the transcriptional network in progenitors (11), and allows for growth-dependent, rather than morphogen-dependent, regulation of progenitor domain proportions.

To investigate direcly whether the differentiation rate affects domain proportions, we reasoned that if the spatial differences in the differentiation rate were removed, the pMN domain, which normally differentiates at a higher rate than other domains, would increase in relative size. We imposed approximately uniform differentiation rates in chick using in ovo electroporation in two ways: (i) increasing differentiation in all domains by overexpressing Ngn2 or p21 (Fig. 6, A and B, and fig. S9, A and B) (28, 29); and (ii) inhibiting differentiation in all domains by overexpressing YAP (Yes-associated protein), an effector of Hippo signaling (Fig. 6, C and D), or the Notch intracellular domain (fig. S9, C and D) (30, 31). These perturbations have an established effect on neuronal differentiation (2831) and caused a decrease in progenitor number in the first case and an increase in the second, without a significant change in the mitotic index (Fig. 6, A and C, and fig. S9E). In the case of Ngn2 overexpression, the differentiation rate of nonelectroporated cells (fig. S9, F and G) was also affected and became spatially uniform, suggesting that nonautonomous mechanisms—e.g., feedback from postmitotic cells—are involved in differentiation control (32). Importantly, in all conditions the relative size of the pMN domain became larger on the electroporated compared to the contralateral side (Fig. 6, B and D) and was similar to the larger pMN relative size at the onset of the experiment (~30 hours) (Fig. 2G). Because these perturbations cause opposite effects on the overall tissue size, this result cannot be explained by changes in the relative range of the signaling gradients and respecification.

Fig. 6 Perturbing differentiation changes the relative pMN size.

(A) Chick electroporation at HH14 of Ngn2+GFP assessed after 48 hours. (B) Number of Sox2+ progenitors per hemisection on the control versus Ngn2 electroporated side for 13 sections (five embryos) as described in (A). (C) Electroporation of constitutive YAP+GFP, as in (A). Progenitors expand both dorsoventrally and apicobasally on the electroporated side. (D) Quantification of (C) for 12 sections (six embryos). Error bars, mean ± SEM.

Discussion

Here, we show that progenitor domain proportions in the neural tube continuously change through a conserved sequence that is independent of animal size. Pattern is first established by morphogen-driven cell fate specification and then elaborated by cell-type–specific regulation of differentiation rates.

How the spatiotemporal changes in the differentiation rate are regulated is a key question. The length of G1, Notch signaling, and proneural genes (e.g., Ascl1 and Ngn1/2), which are activated downstream of domain identity regulators such as Olig2, could play a role (28, 3338). The comparison of mouse to chick and Minute embryos suggests that the temporal changes in the differentiation rate are conserved and independent of embryo size, thus ensuring that domain proportions are comparable between individuals. This constrains the possible molecular mechanisms controlling the differentiation rate and implies that feedback regulation might ensure its robustness (32). The nonautonomous effect after Ngn2 electroporation suggests a possible role for postmitotic neurons in regulating the differentiation rate of progenitors, although other mechanisms cannot be excluded.

The transition from specification to differentiation phase correlates with the dynamics of Shh and BMP signaling. These dynamics depend on transduction cascades but are also likely to be constrained by the effective ligand diffusion, degradation, and the size of the morphogen source (39). Despite the decrease in Shh and BMP signaling, progenitor pattern is maintained during the differentiation phase. This could be explained by bistability produced by the transcriptional network (11). In the floorplate, a transcriptional network downstream of Fgf signaling contributes to these cells becoming refractory to Shh and BMP before E9.5 (40, 41). Our data suggests that neural progenitors in the other domains tolerate a decrease in Gli and pSmad activity, although some level of Shh signaling is clearly required during the differentiation phase (23, 42).

During the specification phase, chick, mouse, and Minute embryos are of similar initial size. This might result from the early period of regulative growth apparent from surgically manipulated embryos (43, 44). Thus, the timing of the transition from specification to differentiation could be connected to an optimal tissue size for the formation and activity of morphogen gradients. Further quantitative analysis will be needed to understand both morphogen-dependent and -independent scaling mechanisms in other tissues and species.

Materials and methods

Mouse strains

To generate Sox1CreER, the Sox1 reading frame was replaced with CreERT2 (fig. S4A). The following strains were previously described: Tg(GBS-GFP) (Gli binding sites–green fluorescent protein) (11), Olig2KICreER (27), CAG-CAT-EGFP (45), Fucci-S/G2/M #504 (46), and Rpl24(Bst) (15, 47). Strains were maintained on a Parkes background to maximize litter size.

Embryo staging

Embryos were staged according to the number of somites, where one somite is generated every 2 hours in mouse and 1.5 hours in chick (48). Hamburger and Hamilton staging criteria were used for late stages of chick development (49). The chick data set was registered to mouse, so that the brachial-level somite at which the measurements were made was generated at equivalent corresponding time (table S1).

For GBS-GFP and pSmad measurements, embryos were initially staged by somite number. The dorsoventral lengths of the neural tubes were fitted to Embedded Image, where a and b are fit parameters, t is time (fig. S8F), and then restaged based on the fit.

Immunohistochemistry and imaging

Transverse sections were processed as described (11). Idu/BrdU antigens were exposed by 40-min deoxyribonuclease I treatment at 37°C, except mouse E8.5, where 2N HCl was used.

Flat-mount preparation: the neural tube was cut at the roofplate and then fixed in 4% paraformaldehyde and subsequently methanol. Antibody incubations and washes were 24 hours each. The left/right neural-tube halves were split, then mounted with grease spacers between slide and coverslip.

Sections were imaged with 40x/1.25NAOil objective, flat mounts with 20x/0.7NADry on a Leica TCS-SP5-MP. Single optical sections were taken, except for GBS-GFP and pSmad analysis, where a maximum projection of 3 z slices 1 μm apart were used. For flat mounts, the entire apicobasal depth of the progenitor layer was imaged with z slices 1.5 μm apart.

Antibodies used were goat anti-Sox2 (R&D systems, 1:100), rat anti-pH3 (Novus Biologicals, 1:2000), rabbit anti-Olig2 (Millipore, 1:1000), rabbit anti-Arx (50) (from J. Chelly, 1:1000), mouse anti-Pax3(c) (Developmental Studies Hybridoma Bank, 1:100), rabbit anti-Islet1 (51) (from T. Jessell, 1:3000), sheep anti-GFP (Biogenesis, 1:1000), mouse anti-Nkx2.2 (DSHB, 1:25), rabbit anti-mAzami Green (MBL, 1:100), rabbit anti-cleaved Caspase3 (Cell Signaling, 1:500); rabbit anti-pSmad1/5/8 (from E. Laufer), mouse anti-BrdU/IdU (1:80, BD clone B44), rat anti-BrdU (1:80, Abcam, clone BU1/75).

Chick electroporation

Chick electroporation was performed in ovo at HH14 and analyzed 48 hours later. Plasmids used: pMIW-YAP (from Xinwei Cao), pCAGGS-NICD (from Olivier Pourquie), pCAGGS-p21 (from Cheryll Tickle), pCAGGS-Ngn2-IRES-GFP (from Francois Guillemot), pPS-CFP2-N (Evrogen), and pCI-H2B-EGFP (from Tatjana Sauka-Spengler). The first three were coelectroporated with pCAGGS-NLS-GFP to mark transfected cells. Final concentrations were 0.5 μg/μl for pMIW-YAP and pPS-CFP2-N, and 1 μg/μl for all other plasmids.

Mouse embryo culture

Mouse embryo culture was performed as previously described (11).

IdU/BrdU incorporation

Chick: 0.5 mg/ml IdU or 3.3 mg/ml BrdU (Sigma) in PB, 10% sucrose, 0.5% Fast Green, were injected into the neural tube, and 50 μl was added on top of the embryo. Embryos were treated with IdU for 1.5 hours, then BrdU for 50 min.

Mouse: Pregnant mice were intraperitoneally injected with 0.6 mg IdU and after 1.5 hours with 1 mg BrdU. Embryos were harvested after 30 min.

Chick live imaging

Membrane-anchored GFP transgenic chicken eggs were obtained from the Roslin Institute, Edinburgh. Embryos were electroporated with pCI-H2B-EGFP 8-15h before imaging.

For live imaging, we established a sagittal slice culture protocol, based on a “clot” method (52, 53). The brachial and anterior thoracic region was dissected in L15 medium, then transferred to a glass-bottom dish (MatTek) in a small drop of culture medium [DMEM-F12 1:1, supplemented with N2, B27 (Life Technologies)] containing 10 mg/ml fibrinogen (Calbiochem). Thrombin (0.5U/μl, Amersham) was added, and a fibrin gel was allowed to form for a few minutes. The slice was covered with ~0.5 ml culture medium, and the dish was humidified. Z stacks were collected for 3 hours on an inverted Leica-SP5 confocal at 37°C.

Photoconversion in chick embryos

Stage HH16 chick embryos electroporated with pPS-CFP2-N were cultured using the EC (early chick) culture method (54), dorsal side up, and immediately photoconverted along the entire dorsoventral length using Leica MP-SP5 microscope, 10X/0.7NADry lens, 30% laser (405 nm) power, ~25 s scan time. Either 15 hours or 0 hours after photoconversion, the neural tube was flat-mounted in phosphate-buffered saline and immediately imaged.

DV boundary positions and pSmad and Gli activity profiles

Image analysis was performed in Fiji (http://fiji.sc/Fiji) and data analysis in MATLAB (Mathworks, MA, USA).

The mean fluorescence intensity in immunostained sections was quantified across a 10-μm region adjacent to the apical lumen. The data was background-subtracted and smoothed with a 5-μm moving average. Boundaries were defined as the positions where the intensity increased above 10% of maximum.

pSmad and GBS-GFP intensity profiles were normalized to the mean profile for each time point, similarly to a described procedure (55), by normalized intensity = a × (raw intensity), where a is a fit parameter. Profiles that correlated poorly with the mean (R2 < 0.5) were discarded. These were usually sections damaged during dissection and represented <5% of the data.

Seven independent time courses of pSmad and GBS-GFP were collected. Sections in each time course were stained and imaged together to minimize technical variability. The seven data sets were pooled by normalizing to the median value of Φ for each data set, where Φ is the 90th percentile of the fluorescence intensity of each profile.

Progenitor and neuron numbers and differentiation rate

The number of progenitors per section was inferred from the Sox2+ domain area (Fig. 1B) and the average density of Sox2+ nuclei for each stage (fig. S1, A and B) determined from a subset of sections. The number of neurons was determined by counting Dapi+,Sox2 nuclei. Islet1+ and interspersed Islet1 nuclei [which are HB9/MNR2+ (not shown)] in the ventral horn were considered MNs. The Pax3 boundary was used to separate ventral interneurons V2-V0 and dorsal interneurons.

Neurons (N) are produced from progenitors (P) with a rate of differentiation γ, i.e.,Embedded Image. We obtained an estimate of γ using Embedded Image, where Embedded Image was the time interval between two time points, Embedded Image was the difference in neuron number between the end and the beginning of the time interval, and Embedded Image was the progenitor number in the middle of the interval. The error of γ was calculated by propagation of the standard deviations of all participating variables, assuming that the errors are independent and uncorrelated. The 95% CIs, calculated from the mean, SD, sample size, and Student’s t value, were linearly interpolated between time points.

Proliferation rate by IdU/BrdU incorporation

Three cell populations were distinguished by anti-IdU/BrdU, anti-BrdU, and anti-Sox2 immunostaining: (i) Sox2+, IdU+, and BrdU (denoted IduL) are progenitors labeled by IdU during the 1.5-hour pulse, which have exited S phase before BrdU addition; (ii) Sox2+, IdU+, and BrdU+; (iii) Sox2+, Idu, and BrdU.

The IdU labeling index IduLI is defined as the ratio of IduL over the total number of Sox2+ progenitors. It is related to the pulse duration Embedded Image hours and the total cell cycle length Embedded Imageas:Embedded Image(3)In turn, the proliferation rate λ is related to Embedded Imageand IduLI as:Embedded Image(4)Two assumptions are made: (i) cells divide asynchronously and (ii) the length of the pulse is shorter than the G2 phase. This is supported by the random appearance of mitotic figures in flat mounts and by the observation that no IduL cells were found in telophase, indicating that they are not completing mitosis within the experiment.

Mitotic index

The relationship between the duration of mitosis, the total cell cycle length, and the fraction of cells in mitosis depends on the exact growth characteristics of the tissue (56). The MI for an exponentially growing tissue is defined asEmbedded Image(5)where Embedded Image is the duration of the pH3-positive phase of mitosis and Embedded Image is the cell cycle length. The proliferation rate λ is related to Embedded Image and MI by:

Embedded Image(6)

Thus, to calculate λ, it is enough to know MI and the duration of mitosis. MI was directly measured from sections. To determine the duration of mitosis, we used the fact that λ is related to both MI (Eq. 6) and IduLI (Eq. 4). Hence,

Embedded Image(7)

The average values of MI and IduLI from all stages that were identical between the two types of experiments were used for calculating Embedded Image. The resulting mitosis duration is 24.6 ± 7.0 min for chick and 27.7 ± 11.3 min for mouse. These are similar to published values (24, 25).

MI in flat mounts (fig. S2, C and F) was estimated from the number of pH3+ cells per apical area, normalized to the average apicobasal length for the respective stage and domain measured in sections (Fig. 1F and fig. S1C).

Cell cycle phase distribution

Mitotic cells were identified using DapiS+G2 cells using the Fucci-S/G2/M-Green fluorescence intensity. The fluorescence intensities of Olig2, Nkx2.2, and Fucci-S/G2/M-Green were measured in individual nuclei. The Olig2 and Nkx2.2 levels were background-subtracted and normalized to the average intensity in the respective domain. Cells with Olig2/Nkx2.2 ratio between 0.1 and 10 were defined as coexpressing.

Coexpressing cells are assumed to undergo a transition from an Olig2 to an Nkx2.2 stable state or, with a smaller probability, vice versa (11). If the transition occurs preferentially in G1 or S+G2 phase, the cell cycle phase distribution in cells that are at the onset of the transition could appear different than in noncoexpressing populations. However, the distribution of both G1 and S+G2 phases across the Olig2-Nkx2.2 level difference was normal (fig. S3C), suggesting that the transition may occur at any time of the cell cycle.

Olig2 lineage tracing

Olig2KICreER mice (27) were crossed to CAG-CAT-EGFP (45). Cre expression was induced in Olig2+ progenitors by injecting 3 mg of tamoxifen. As a result of the recombination, EGFP was induced with a delay of 12 hours (fig. S10), allowing the tracking of cells after they lose Olig2 expression. Embryos were harvested 48 hours after injection; hence, the effective time interval of EGFP labeling was ~36 hours.

The change in the number of labeled progenitors P, regardless of their type, during the time course of the experiment Embedded Image(t1, time at the beginning; t2, end time) isEmbedded Image(8)Here, Embedded Image are all labeled progenitors at t2 and ΔN are all labeled neurons. Δt = 36 hours, and the proliferation rate, λ, are known (the values in Fig. 3A were used); hence, the only unknown is Embedded Image. Activation at t1 occurs only in Olig2+ cells; therefore, Embedded Image. Hence, the change in the Olig2+ progenitors alone isEmbedded Image(9)where Embedded Image are the labeled Olig2 progenitors at t2, ΔMN the number of labeled motor neurons, and ψ, which remains the only unknown, is the rate of loss of Olig2 identity at the expense of other progenitor types. Because Δt is large, the reported values of ψ (Fig. 5C) are approximate.

Clonal analysis

Sox1CreER/+ mice were crossed to Gt(Rosa)26-FloxSTOP-Flox-EYFP homozygotes. Pregnant mice were intraperitoneally injected with 0.3 mg tamoxifen at E9.5 and sacrificed 48 hours later. The labeled cells formed clusters that were usually >10 cell diameters away from each other, whereas within a cluster, cells were rarely separated by more than 3 unlabeled cells. Therefore, labeled cells were grouped into clones by scanning a 29-μm radius (≈6 cell diameters) around each cell. For most images, changing the radius by ±5 μm preserved clone grouping. Occasional too densely labeled images were discarded.

Clone shape descriptors (table S2) were derived from the second moment matrix of the cell coordinates of each clone, in which the unit eigenvectors represent two orthogonal axes, and the eigenvalues the variance along these axes. The first eigenvector represents the orientation of the clone with respect to the anterioposterior axis. The anterioposterior and dorsoventral spread of a clone were defined as the distance within ±2 SD from its center of mass.

The distribution of clone orientation angles was determined using a kernel density estimation method and was different in the pMN domain compared with pD, pI, and p3 (two-sample Kolmogorov-Smirnov test, P < 0.05).

The density of clonal nuclei (estimated by fitting an ellipse around large clones) corresponded to 19 ± 14 μm2 per cell. The density of nonclonal nuclei, determined in the Pax3 domain in small volumes (~120 cells) was 2.7 ± 0.1 μm2 per cell, suggesting that clonal nuclei are ~7 times more dispersed than nonclonal nuclei.

Supplementary Materials

www.sciencemag.org/content/345/6204/1254927/suppl/DC1

Supplementary Text

Figs. S1 to S10

Tables S1 to S3

Reference (57)

References and Notes

  1. Acknowledgments: We thank B. Simons, C. Tabin, A. Ugur, M. González-Gaitán, N. Bushati, and M. Cohen for comments on the manuscript; B. Simons and G. Zhang for discussions and help with the clonal analysis; R. Pérez and S. Loubéry for discussions; S. Booth, C. Scott, C. Galichet, S. Malas, K. L. Lee, and A. Ekonomou for generating the Sox1CreER strain; X. Cao, T. Sauka-Spengler, E. Laufer, J. Chelly, T. Jessell, C. Tickle, O. Pourquie, and M. Götz for providing reagents; and N. Mousavy for technical assistance. This work was funded by the Medical Research Council (MRC) (U117560541) and the Wellcome Trust (WT098326MA). A.K. was supported by Federation of European Biochemical Societies, Marie-Curie, and MRC fellowships. The supplementary materials contain additional data. Author contributions: A.K. performed the experiments. A.K. and J.B. conceived the work, analyzed the data, and wrote the manuscript. T.B. analyzed the gradient dynamics and helped with the quantitative analysis. A.R. analyzed the patterning dynamics. H.P.V. participated in the photoactivation and live imaging. V.E. and R.L.-B. contributed the Sox1CreER mouse.
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