# Fgf8 dynamics and critical slowing down may account for the temperature independence of somitogenesis

Weiting Zhang, Pierluigi Scerbo, Marine Delagrange, Virginie Candat, Vanessa Mayr, Sophie Vriz, Martin Distel, Bertrand Ducos, David Bensimon

► To cite this version:

Weiting Zhang, Pierluigi Scerbo, Marine Delagrange, Virginie Candat, Vanessa Mayr, et al. Fgf8 dynamics and critical slowing down may account for the temperature independence of somitogenesis. Communications Biology, 2022, 5 (1), pp.113. 10.1038/s42003-022-03053-0. hal-03727212

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# Fgf8 dynamics and critical slowing down may account for the temperature independence of somitogenesis

Weiting Zhang<sup>1,2,7</sup>, Pierluigi Scerbo<sup>1,2,7</sup>, Marine Delagrange<sup>1,2,3</sup>, Virginie Candat<sup>1,2</sup>, Vanessa Mayr<sup>4</sup>, Sophie Vriz<sup>5</sup>, Martin Distel<sup>1,4</sup>, Bertrand Ducos<sup>1,2,3✉</sup> & David Bensimon<sup>1,2,6✉</sup>

Somitogenesis, the segmentation of the antero-posterior axis in vertebrates, is thought to result from the interactions between a genetic oscillator and a posterior-moving determination wavefront. The segment (somite) size is set by the product of the oscillator period and the velocity of the determination wavefront. Surprisingly, while the segmentation period can vary by a factor three between 20 °C and 32 °C, the somite size is constant. How this temperature independence is achieved is a mystery that we address in this study. Using RT-qPCR we show that the endogenous *fgf8* mRNA concentration decreases during somitogenesis and correlates with the exponent of the shrinking pre-somitic mesoderm (PSM) size. As the temperature decreases, the dynamics of *fgf8* and many other gene transcripts, as well as the segmentation frequency and the PSM shortening and tail growth rates slows down as T-T~c~ (with T~c~ = 14.4 °C). This behavior characteristic of a system near a critical point may account for the temperature independence of somitogenesis in zebrafish.

<footnote n="1">¹LPENS, PSL, CNRS, 24 rue Lhomond, 75005 Paris, France. ²IBENS, PSL, CNRS, 46 rue d'Ulm, 75005 Paris, France. ³High Throughput qPCR Core Facility, ENS, PSL, 46 rue d'Ulm, 75005 Paris, France. ⁴St Anna Children's Cancer Research Institute, Zimmermannplatz 10, 1090 Vienna, Austria. ⁵CIRB, Collège de France, 75005 Paris, France. ⁶Department of Chemistry and Biochemistry, UCLA, Los Angeles 90094, USA. ⁷These authors contributed equally: Weiting Zhang, Pierluigi Scerbo. ✉email: bertrand.ducos@phys.ens.fr; david@phys.ens.fr</footnote>
Somitogenesis is the process of segmentation of the antero-posterior axis in vertebrates. In zebrafish this process starts at about 10 hpf and ends at 24 hpf¹. During that developmental interval, as the embryo elongates, pairs of somites synchronously and periodically pinch off from the anterior part of the PSM in an anterior to posterior series until 31 pairs of somites are formed. The period between somites, but surprisingly not their size, is strongly temperature dependent².

The formation of somites in zebrafish is preceded by the establishment of a segmental pre-pattern in the anterior PSM accomplished by a stripe of gene expression that is thought to result from the interactions between a genetic oscillator and a posterior-moving determination wavefront. This pre-pattern determines the position of the next somite. The Clock and Wavefront framework first proposed by Cooke and Zeeman³ in 1976, is currently used to describe the output of the complex genetic network underlying the formation of this pre-pattern. In this framework, periodic oscillations (the segmentation clock) that move anteriorly (in the PSM reference frame⁴), pass through a determination wavefront moving posteriorly (in both the lab and the PSM reference frames) and stop oscillating. As a result, a stripe of genes such as *mesp2* are activated to establish the future boundary of the following somite¹. In this model, the size of a somite is determined by the distance traveled by the determination wavefront during one cycle of the segmentation clock⁴,⁵ (see Fig. 1).

The segmentation clock driving the differentiation of the PSM into somites at the determination wavefront, has been amply studied and described⁴,⁶ and is not the subject of this work. Rather we here focus on the determination wavefront. In contrast to the segmentation clock whose details are species dependent, the main putative actors of the wavefront (e.g., fibroblast growth factors (Fgf), retinoic acid (RA)) are conserved in vertebrates (from fish to mammals, including snakes and amphibians⁷). Previous studies have shown that as cells exit from the progenitor domain at the posterior end of the PSM, they stop transcribing *Fgf* genes⁸⁻¹¹. Thus, *fgf* mRNA progressively decays as cells move towards the anterior of the PSM and an *fgf* gradient is formed¹². This mRNA gradient is translated into a protein gradient and into a MAPK activity gradient along the PSM (as Erk, a MAPK protein is activated downstream off the FGF receptor)⁹,¹⁰.

Spurred by these experiments we have decided to investigate the dynamics of the PSM in fish embryos subjected to various perturbations of the putative actors of the wavefront (Fgf, RA, Erk, etc.). For these investigations we used time-lapse and fluorescent microscopy on live wild-type or transgenic embryos

expressing either a fluorescent reporter of Erk activity or an exogenous source of Fgf8. In agreement with experiments on tail explants¹³, our results imply that somite formation results from a coupling between the somitogenetic clock and the local spatial (but not temporal) gradient of Fgf8 (or Erk activity). Expanding on these previous investigations, we observe that the PSM size vary as the logarithm of the *fgf8* mRNA concentration, a result that has a simple explanation if the *fgf8* mRNA concentration decays exponentially in both space and time.

In addition, we took advantage of the external development of zebrafish embryos to manipulate the temperature of development. As the temperature T is lowered we find that the dynamics of *fgf8* and many other genes implicated in somitogenesis and cellular differentiation slow down by the same factor, namely as (*T*−*T*<sub>c</sub>) (with *T*<sub>c</sub> = 14.4 °C). Slowing down by this factor is also observed² for the segmentation frequency *f*<sub>s</sub>, the spatio-temporal dynamics of Erk and the PSM shrinkage and tail growth rates. These observations suggest that the temperature invariance of the developmental program during somitogenesis could be a simple reflection of the critical slowing down of some cellular metabolic networks near a critical temperature *T*<sub>c</sub>.

## Results

**Kinetics of somitogenesis impairment by Fgf-pathway inhibition.** We monitored the dynamics of Erk during somitogenesis in transgenic zebrafish (DREKA) embryos expressing a fluorescent reporter which cytoplasmic localization increases upon increasing Erk phosphorylation<sup>14,15</sup>. Changes in Erk activity (i.e., phosphorylation) are thus well reflected and reported by changes in the ratio between cytoplasmic and nuclear fluorescence (Fig. 2a–c). As previously reported<sup>16–18</sup> we observed that the domain of Erk activity shrank over time (Fig. S1a, b), with transitions at the segmentation clock period from a high activity to a low activity domain at a distance of about 3–4 somites down from the last somite, i.e., 3–4 segmentation periods prior to the appearance of a new somite (Fig. S1c). This transition in Erk phosphorylation is the earliest indication of commitment to differentiation into somites<sup>16</sup>.

Having confirmed the role of Erk as an early somitic marker, we then studied the response of an embryo to perturbations of the Fgf pathway (of which Erk is a downstream effector) by pharmacological inhibition of the pathway with SU5402. Embryos exposed to a low concentration of SU5402 (50 µM), display an increase in the next jump of the Erk domain of activity (i.e., a larger somite three periods later) (Fig. 2a), followed by

<figure><img src="image_3.png" /><figcaption>**Fig. 1 Schematics of somitogenesis.** a The Clock and Wavefront model: antagonistic gradient of Fgf8 (originating from the posterior PSM, green) and RA (originating from the somites, violet) define a wavefront which interacts with a particular phase of the segmentation clock (in the PSM, red) to generate somites at periodic times and positions. b Kymograph of somitogenesis from 7 to 20 somites. The tail elongates at a constant rate $V_{\text{tail}}$ while the PSM shrinks at a roughly constant rate $V_{\text{PSM}}$ resulting in a somite wavefront propagating<sup>5</sup> (in the lab frame) at a rate $V_{\text{front}} = V_{\text{tail}} - V_{\text{PSM}}$.</figcaption></figure>
<figure><img src="image_4.png" /><figcaption>**Fig. 2 Somitogenesis at low Erk activity.** a Time lapse observations of the Erk activity domain in DREKA embryos following exposure to a low (50 µM) concentration of SU5402 (an inhibitor of the Fgf pathway). The time span between images is 4 min. (the period of the clock in this experiment is about 45 min.) The yellow lines point to the boundary of Erk activity which periodically jumps by about 50 µm except in the first period after administration of SU5402 where the jump is larger (labeled as SU). Scale bar: 50 µm. b–e Normal somitogenetic development in DREKA embryos (control). b Erk activity in DREKA embryos at 14 somite stage: dark nuclei point to high Erk activity. c The false color images represent the Erk activity averaged over a 30 µm perpendicular stack of images. Notice the low activity area in the pre-pattern region (shown by the bracket) at the anterior PSM. d In situ hybridization (ISH) against *xirp2a* (a marker of somite boundaries) in 30 hpf embryos. e Immuno-Histochemical (IHC) staining against Mesp2a, a determinant of the last somite boundary (arrow). f–i Somitogenetic development in DREKA embryos in presence of a high (200 µM) concentration of SU5402 from the 10 somite stage (arrow in (h)). Somitogenesis is impaired past 13 somite stage (indicated by a * in h) with unclear somite boundaries. f, g The Erk activity is repressed (low) throughout the PSM. h ISH against *xirp2a* in 30 hpf embryos. i The determinant of the last somite boundary (Mesp2a), shown by an arrow is absent past 13 somite stage in i but present in e. Scale bar: 50 µm.</figcaption></figure>

regular jumps (and somites) similar to WT embryos¹⁸. However, if the embryos are exposed (at the ten somites stage) to 200 µM of SU5402 the activity of Erk is completely repressed in all the PSM (compare Fig. 2f, g with the control shown in Fig. 2b, c). In such case, somite formation is impaired three segmentation periods later (i.e., from the 13 somites stage onward) (compare Fig. 2h, i with Fig. 2d, e); regular somites are not observed and expression of Mesp2a (a marker of the last somite¹) is absent.

**Uniform activation of the Fgf pathway impairs somitogenesis.**
Next, we examined the role of RA in somitogenesis. Embryos were incubated from one cell stage in 10 µM DEAB (an inhibitor of RA synthesis) and exposed or not at 70% epiboly to 10 nM transRA (a physiological level which has been shown to rescue rhombomere formation following DEAB treatment¹⁹). These perturbations had minimal effects on the domain of activity of Erk (Fig. S2a) and on the dynamics of the somitogenetic wavefront (Fig. S2b). On the other hand, embryos treated with DEAB from the one-cell stage and incubated in 1 µM transRA at the onset of somitogenesis display a strong uniform activation of Fgf8 in the PSM²⁰ (Fig. S3). Subjecting DREKA embryos to such a high RA concentration from the ten somite stage onward has dramatic effects: the Erk activity is uniformly enhanced throughout the PSM (Fig. 3e, f), and somitogenesis is impaired from 13 somites stage with unclear somite boundaries and no expression of Mesp2a¹ (Fig. 3g, h).

The data shown in Figs. 2 and 3 suggest that a spatial gradient of Erk activity (or Fgf8) is required for proper somite formation. To check whether a temporal variation of Erk activity could also alter somite formation, we next studied somitogenesis in presence

of an increasing uniform concentration of Fgf8 from an exogenous source.

**Uniform activation of an exogenous Fgf8 source does not affect somitogenesis.** Our data in agreement with previous results¹³ suggest that somitogenesis is sensitive to the gradient of Fgf8 (or Erk activity) but insensitive to physiological perturbations of the RA concentration. To investigate the role of the Fgf8 variation during somitogenesis, we used a transgenic embryo *Tg(uas;fgf8-T2A-cfp)* to superpose an increasing but uniform source of Fgf8 on the endogenous one. The exogenous *fgf8* gene is turned on (Fig. 4a) when a transcription factor Gal4-ERT is released from its cytoplasmic chaperone complex by binding of cyclofen²¹.

Embryos uniformly expressing this exogenous source of Fgf8 display two characteristic phenotypes at 24 hpf, Fig. 4b: a mild phenotype (phenotype 1) characterized by enlarged heart and yolk and abnormal development of the head, and a severe phenotype (phenotype 2) characterized by enlarged heart, abnormal development of the head (with often no eyes), lost yolk extension and disordered late somites (>20 s). In contrast with embryos where the transgene has not been activated (similar to WT), upon expression of this exogenous source of Fgf8, Erk activity is observed throughout the embryo while still stronger at the posterior PSM (Fig. 4c). The continuous expression of the exogenous *fgf8* results in a total concentration of transcripts increasing roughly linearly with time (Fig. 4d), with a doubling of the initial (endogenous) concentration after about 8 h (20 somite stage). In spite of the presence of this uniformly expressed and continuously increasing exogenous source of Fgf8 on top of the endogenous one, the somitogenetic wavefront is barely affected
<figure><img src="image_5.png" /><figcaption>**Fig. 3** Somitogenesis at high Erk activity. **a–d** Control: normal development. **a** Erk activity in DREKA embryos at 14 somite stage: dark nuclei point to high Erk activity. **b** The false color images represent the Erk activity averaged over a 30 µm perpendicular stack of images. **c** ISH against *xirp2a* (a marker of somite boundaries) in 30 hpf embryos. **d** IHC against Mesp2a, a marker of the last somite boundary at 14 somites (arrow). **e–h** Somitogenetic development in DREKA embryos incubated from one-cell stage in 10 µM DEAB in presence of 1 µM RA from the ten somite stage (arrow in **g**). **e, f** The Erk activity is high throughout the PSM. **g** ISH against *xirp2a* in 30hpf embryos. Somitogenesis is impaired past 13 somites (indicated by a *) with unclear somite boundaries. **h** IHC against Mesp2a show that it is not expressed past 13 somite stage (arrows in **d** and **h**). Scale bar: 50 µm.</figcaption></figure>

<figure><img src="image_6.png" /><figcaption>**Fig. 4** Somitogenesis upon induction of exogenous Fgf8. **a** The transgene *uas:fgf8-T2A-cfp* (under control of Gal4-ERT) and its marker Eos. **b** The two characteristic phenotypes observed at 24 hpf upon activation of the transgene. **c** Erk domain of activity visualized by IHC against phosphorylated Erk (pErk) at ten somites in non-activated embryos (left) or in embryos in which the transgene was activated from bud stage (right): the uniformly expressed exogenous Fgf8 enlarges the domain of activity of Erk to the whole embryo, but doesn't alter the Erk activity gradient, Fig. S4. **d** Time variation of total *fgf8* mRNA (RTqPCR data) in presence of an exogenous source of Fgf8. At time *t* = 0 (bud stage) the concentration of *fgf8* is contributed by the endogenous one (continuous line: best linear fit *y* = 0.11 *x* + 1 with *r*² = 0.98). From then on, the endogenous concentration decreases (see Fig. 5) while the exogenous concentration increases: it typically doubles the initial endogenous concentration in 9 h (about 20 somite stage). Inset: gel displaying the increase in exogenous *fgf8* mRNA at various times post activation versus a reference gene (*β-actin*). **e** Rates of PSM shrinkage (*V*<sub>PSM</sub>), tail growth (*V*<sub>tail</sub>), and wavefront velocity (*V*<sub>front</sub>) in embryos (*n* = 17) in which an exogenous source of Fgf8 was turned on. The various rates are only mildly affected by the increase in Fgf8 due to the exogenous source.</figcaption></figure>

and the PSM shrinks at the same rate as in WT embryos (Fig. 4e). In conjunction with the data shown in Figs. 2 and 3 this observation implies that the somitogenetic wavefront is sensitive to the spatial gradient of Fgf8, not its local concentration, a conclusion reached earlier in different studies¹³,¹⁸.

**The endogenous Fgf8 concentration decreases during somitogenesis.** If during somitogenesis the morphogen fields translate with the growing tail, namely if they are stationary in the tail

moving frame, then one expects the PSM size to remain constant. Since the PSM shrinks one is forced to conclude that the morphogen fields are not stationary in the tail moving frame during somitogenesis: their amplitude and/or their extant¹⁸ may vary.

To investigate that question we decided to monitor by RTqPCR the mean endogenous *fgf8* mRNA concentration (⟨|*fgf8m*|⟩) normalized by the mean concentration of *rpl13a*, a reference gene) during somitogenesis in the whole embryo and in the PSM. That concentration is related to the measured qPCR threshold
<figure><img src="image_7.png" /><figcaption>**Fig. 5** Variation of the fgf8 mRNA concentration with somite stage.</figcaption></figure>

Negative ln(<[fgf8m]>) (=ln(2) δCt values from the RTqPCR data) at different somitic stages (blue ○: whole embryo; red ◊: PSM only). Red line: linear best fit (y = ax + b) with a = 0.094 ± 0.013 (X² = 22; DF = 36), corresponding to an exponential decrease of <[fgf8m]> with a time constant τ = 1/a ≅ 11 somitic periods, Eq. (1). Green ◊: -ΔPSM/λ with λ = 260 µm and the PSM shrinkage, ΔPSM, taken from Fig. 4e. From the value of λ and τ we deduce a mean velocity: VPSM = λ/τ ≅ 24 µm/somite.

cycle difference (δCt) via:

$$ \delta Ct = \log_2 \left( \frac{\langle [rpl13] \rangle}{\langle [fgf8m] \rangle} \right) \sim - \frac{\ln(\langle \langle [fgf8m] \rangle \rangle)}{\ln 2} \quad (1) $$

In both whole embryo and PSM, we observed an overall linear increase in the δCt values between the 5 and 21 somite stages, see Fig. 5, corresponding to an exponential decrease in the mean fgf8 concentration $\langle [fgf8m] \rangle \sim \exp(-t/\tau)$ with a typical timescale: τ ~4.5 h or about 11 segmentation periods.

In that time interval the PSM shrinks at a constant rate⁵ (see Fig. 4e): ΔPSM = VPSM·t, with VPSM ~58 µm/h = 24 µm/somite at 27 °C. Therefore, one can also relate the decrease in $\langle [fgf8m] \rangle$ to the PSM shrinkage: $\langle [fgf8m] \rangle \sim \exp(-\frac{\Delta\text{PSM}}{\lambda})$, where: λ = τ VPSM ~ 260 µm is a characteristic length roughly equal to the extent of diffusion of the Fgf8 morphogen field²².

**The dynamics of fgf8 slows down with decreasing temperature by the same factor as the PSM shrinkage rate.** The data obtained previously at 27 °C suggest that the PSM shrinkage rate VPSM = λ/τ is inversely proportional to the characteristic decay time τ of the mean fgf8 mRNA concentration. Since VPSM varies significantly with the temperature² (see Fig. 6c), if that relation is not fortuitous it should hold at all temperatures, namely the variation of 1/τ with temperature should be the same as that of VPSM. To investigate that point we studied the time dependence of the mean fgf8 mRNA concentration at various temperatures.

At all temperatures we observed that the fgf8 δCt values (between 5 and 21 somites) increase linearly with time, i.e., $\langle [fgf8m] \rangle$ decays exponentially with time. The typical timescale τ of that exponential decay (i.e., the slope of δCt vs. time, see Eq.(1)) varies with temperature as: 1/τ ≅ 0.0152 (T - Tc) h⁻¹ with Tc = 14.4 °C (Fig. 6a, b), a behavior similar to the variation

with temperature of the growth rate and PSM shrinkage rate, see Fig. 6c. Therefore, the relation between the PSM shrinkage and the fgf8 decay rate holds at all temperatures and is not fortuitous. Notice also that the divergence of τ with temperature is similar to that of the segmentation period²²: τs ≅ 5.32/(T - Tc) hours (see inset in Fig. 6a).

These observations on the temperature independence of the average level of fgf8 mRNA at given stages of somitogenesis (Fig. 6b) are further supported by measurements of the spatial activity of Erk, a downstream effector of Fgf8. As shown in Figs. 7 and S5, the spatial distribution and intensity of pErk is temperature independent: it is the same at similar stages of somitogenesis but different temperatures (from 20 to 32 °C).

**The dynamics of many gene transcripts active during somitogenesis slow down with temperature as T - Tc.** The variation with temperature of the segmentation period, tail growth rate, PSM shrinkage rate and fgf8 decay rate are characteristic of the critical slowing down of a system near Tc. If somitogenesis is indeed a critical system, all time-varying gene transcripts should behave similarly, i.e., their characteristic time should scale as 1/(T - Tc) or stated differently their variation as a function of the somite stage, s = t/τs should be temperature independent. To address this question, we studied, using RTqPCR, the dynamics of the relative average concentration of many gene transcripts at different temperatures, see Table S1. If they scale with temperature in the same way as the segmentation clock period, the data for a given transcript taken at different temperatures should fall on the same curve.

This is the case for genes known to play a role during somitogenesis²³, see Fig. 8, such as the genes implicated in the segmentation clock²⁴ (her1, her7, and hes6) and its synchronization²⁵ (deltaC, deltaD, and notch1a), in segmental patterning (mespa and mespb) and myogenesis (myog) but also for genes involved more generally in cellular differentiation (vox, ventx, nanog, and oct4) (Fig. S6). For genes which δCt value vary linearly with time during somitogenesis we can compute the slope of the linear best fit at various temperatures (Figs. 6a and S7). This analysis confirms the critical slowing down of genes as the temperature is decreased. Notice however that not all genes vary during somitogenesis. For some of them (fgf4, igf2a, wnt3, and xpc), the relative mean concentration seems constant between 5 and 21 somite stage (Fig. S8).

## Discussion

In this work, we have studied some factors affecting the somitogenic wavefront velocity, in particular the PSM shortening rate. The observed impairment of somitogenesis in absence of an Erk activity gradient (with either uniformly high or low Erk phosphorylation) suggests, in agreement with recent reports¹³,¹⁸, that it is the spatial variation of Fgf8 (via its downstream effector, Erk) and not its local concentration which sets the position of the somitogenetic wavefront. This conclusion is further confirmed by the observed invariance of somitogenesis in presence of a uniformly increasing concentration of Fgf8. The observed periodic jumps in the anterior boundary of the Erk activity domain moreover imply that commitment to somite formation is triggered when the gradient of Fgf8 falls below a threshold at a certain phase of the segmentation clock.

The shortening of the PSM therefore implies that the Fgf8 gradient decays with time. To investigate that issue we have measured the mean fgf8 mRNA concentration during somitogenesis (in whole embryo and in the PSM). Our observations point to an exponential decrease of the mean fgf8 mRNA concentration with a typical time scale of τ ~11 somitogenetic
<figure><img src="image_8.png" /><figcaption>**Fig. 6** Variation with temperature of the dynamics of fgf8 mRNA, tail growth and PSM shrinkage. **a** Variation with temperature of the slope α of δCt(fgf8(t)) vs time (Fig. 5), which is linearly related to the exponential decay rate of <[fgf8m]>: 1/τ = ln(2) α. The red point at 27 °C is from PSM only data. The data can be fit (blue line) by α = a (T-Tc) with: a = 0.022 ± 0.0038; T_c = 14.4 °C (χ² = 6.57; DF = 6). Inset: variation of the clock frequency f_s = 1/τ_s vs temperature² (data from Schröter et al.²) which can be fit by f_s = a_s (T - T_c) with a_s = 0.188. **b** Another way to represent the data shown in **a**: since δCt(fgf8 (t)) varies with temperature in a similar way as the segmentation period, τ_s, the δCt(fgf8(t)) data taken at different temperatures collapse on the same curve as a function of somite stage: s = t/τ_s (=number of segmentation periods). The data at all temperatures can be fit (blue line) by δCt = a' s + b, with a' = 0.122 ± 0.0098 and b = 3.955 (χ² = 26.5; DF = 55). Notice that as expected: a = a'· a_s. **c** variation with temperature of the growth rate (blue points) and the PSM shrinkage rate (red points) and linear best fits (blue lines): y = β(T - T_c) with β = 4.79 ± 0.46 (χ² = 6.35; DF = 2; blue points) and β = -5.08 ± 0.20 (χ² = 0.51; DF = 2; red points).</figcaption></figure>

periods: <[fgf8m]> ~ exp(-t/τ). Since the PSM shrinks at a constant rate V<sub>PSM</sub> ~24 µm/somite: ΔPSM = V<sub>PSM</sub> t, the mean fgf8 mRNA decay can also be expressed as a function of the PSM size: <[fgf8m]> ~ exp(-ΔPSM/λ), with λ = τ V<sub>PSM</sub> ~ 260 µm.

These results are consistent with a source-sink mechanism for the Fgf8 gradient²², where the fgf8 mRNA is generated in the progenitor domain with a time decreasing concentration (see Supplementary Note 1) and is degraded on a typical length-scale λ towards the anterior part of the PSM: [fgf8m(x,t)] = F₀ exp(-x/λ - t/τ) ≡ u(x,t), where x is the distance to the tail end. Thus, the measured mean concentration <[fgf8m]> varies

exponentially with time, as indeed observed:

$$ \langle [fgf8m] \rangle = \int_{0}^{\infty} dx [fgf8m(x, t)] \sim \exp(-t/\tau) \quad (2) $$

Our results suggest that a new somite n is formed at distance x_n from the tail end when the gradient of Fgf8(x,t) falls below a certain threshold, η_t at a given phase of the somitogenesis clock: t = nτ_s.

$$ \eta_t = - \frac{d \text{Fgf8}}{dx} (x_n, n\tau_s) \quad (3) $$
<figure><img src="image_9.png" /><figcaption>**Fig. 7** Somitogenesis at different temperatures. Phosphorylated Erk (pErk) distribution in WT embryos grown at different temperatures (20, 24, 28, and 32 °C) at 4 different stages of somitogenesis (7, 11, 15, or 19 somites stages) visualized by fluorescence following Immunohistochemistry staining (IHC). Even though embryos at 20 °C grow about three time slower than embryos at 32 °C, at similar stages embryos grown at different temperatures are similar and display similar pErk domain.</figcaption></figure>

If the concentration of Fgf8 protein is a monotonous function of its mRNA: Fgf8(x,t) = G(fgf8m(x,t)), then:

$$ \eta_t = \frac{1}{\lambda} u_t G'_u(u_t) = \frac{F_0}{\lambda} \exp\left(-\frac{x_n}{\lambda} - \frac{n\tau_s}{\tau}\right) G'_u(u_t) \quad (4) $$

In other words: $x_n = x_0 - n\tau_s\lambda/\tau = x_0 - n\tau_s V_{PSM}$ with $x_0 = \lambda\ln(G'_u(u_t)F_0/\eta_t\lambda)$. Namely the PSM shrinks at a velocity entirely determined by the dynamics of Fgf8 (the ratio between its degradation length-scale $\lambda$ and its decay rate $\tau$) (Fig. S9 and Supplementary Note 1). Notice that if the threshold (i.e., $x_0$) is altered by a drug such as SU5402 from somite stage n onwards, only the size of the first somite after the perturbation $l_{n+1} = x_{n+1} - x_n$ will be altered (as $x_{n+1}$ and $x_n$ are associated to different thresholds (i.e., $x_0$)), while later somites will have a regular size (same threshold, i.e., $x_0$), as indeed observed¹⁸. It may be interesting to check in other model organisms if $\langle [fgf8m] \rangle$ decays exponentially with time and if differentiation into somite is set by its gradient. If so one expects the *fgf8* mRNA concentration to correlate with the PSM size as observed here, i.e., as $\exp(-\Delta\text{PSM}/\lambda)$.

Our results are also compatible with a recent report of a scaling relation between somite and PSM size in tail explants¹³, if the time dependence of the *fgf8* mRNA concentration in these tail explants does not decay exponentially (Fig. S9 and Supplementary Note 1).

We have further observed that the relation between the *fgf8* decay time, $\tau$, and the PSM shrinkage rate $V_{PSM}: V_{PSM} = \lambda/\tau$ was conserved over a temperature range, where $V_{PSM}$ varies by a factor two, implying that this relation established initially at 27 °C is not fortuitous. We observed that the *fgf8* decay rate, the spatio-temporal behavior of its downstream effector (pErk), the PSM shrinkage and tail growth rates and the clock frequency, all display the characteristic behavior of a system near its critical temperature at $T_c = 14.4$ °C: all rates slow down as $T - T_c$. We have generalized that observation to many time-varying genes implicated in somitogenesis and cellular differentiation. These results imply that somitogenesis shares the characteristic

dynamics of a system near criticality²⁶ (all times-scales increase as $1/(T - T_c)$, see Supplementary Note 1), even though the critical temperature is experimentally not achievable (embryos die below about 19 °C). Our observations may explain the invariance of the developmental process to temperature even if its characteristic times-scale changes by a factor 2–3. In other words, there is no need for a specific thermal compensation mechanism to keep all the relevant genes in synchrony, further highlighting the robustness of that system.

One may speculate about the biological significance of the critical temperature. Its value is close to the lowest recorded temperature of the natural environment of zebrafish²⁷. It is also close to the critical temperature below, which swimming is impaired²⁸ and lethality in adult fish increases²⁷. This suggests that zebrafish evolution has tuned some metabolic networks to stop functioning below Tc. In certain fish²⁹, a mechanism known as diapause, can be triggered at certain developmental stages (e.g., mid-somitogenesis) and under certain environmental conditions (such as too high or too low temperatures), which cause the developing animal to enter a state of dormancy. A diapause-like state has been reported in zebrafish, though induced by blockage of the vitamin D synthesis pathway, not by exposure to a low temperature²⁹. It is tempting to speculate that a critical mechanism that causes metabolic networks to stop working below a given temperature and is lethal in zebrafish could have been coopted in other species to shut down some networks and enter a dormancy state.

## Methods

**Fish lines and maintenance.** Zebrafish were raised and maintained on a 14–10 h light-dark diurnal cycle with standard culture methods³⁰. Embryos collected from natural crosses were staged according to Kimmel³¹. The *Tg(uas:fgf8-T2A-cfp;ubi:EOS)* was generated by injecting the plasmid *pt24-uas:fgf8-T2A-cfp;ubi:EOS* (a gift from M. Volovitch), which contains the homologous cDNA sequence of *fgf8* from Danio rerio, with *tol2* mRNA transposase. Founder transgenic fish were identified by global expression of *EOS*. The *Tg(ubi:gal4-ERT;cry:CFP)* was previously described³². The double transgenic line *Tg(ubi:gal4ERT;cry:CFP; uas:fgf8-T2A-cfp;ubi:EOS)* was created by crossing *Tg(uas:fgf8-T2A-cfp;ubi:EOS)* and *Tg(ubi:gal4-ERT;cry:CFP)*. Founder double transgenic fish were selected by global expression of *EOS* and expression of *CFP* in the developing eyes. The transgenic line *tg(ubi:ERK-KTR-Clover)*¹⁰⁰¹ (DREKA) allowing for real time monitoring of Erk activity in live embryos has been described elsewhere¹⁵. Embryos were imaged for phenotypic analysis at 24 hpf and then fixed with PAXgene Tissue Container Product (Qiagen) for RT-PCR.

**RT-PCR.** Extraction of total RNA was performed by using RNeasy Micro Kit (Qiagen), according to the manufacturer's instructions. cDNA synthesis was performed using sensiscript reverse transcriptase (Qiagen) with an anchored Oligo(dT) 23VN primer (NEB). PCR was performed using the Phusion High-Fidelity DNA Polymerase (NEB) with the following protocol: 98 °C for 30 s; then 30 cycles (98 °C for 10 s, 60 °C for 30 s, 72 °C for 30 s); 72 °C for 10 min. A pair of primers, P1 (5'-ACCATTCAGTCCCGCCTAA-3') and P3 (5'-GCCAATCAGTTTCCCCTCC-3'), which respectively match exon3 and exon4 of Fgf8, were used to detect the expression of the pre-mRNA of the endogenous Fgf8 resulting in a 1900 bp PCR product and the expression of the exogenous and correctly spliced Fgf8 resulting in a 283 bp PCR product. Another pair of primers, P3 (same as before) and P2 (5'-CCCCTCCGTTTGAACCGTAA-3') against intron3 of Fgf8, was used to analyze the expression of the pre-mRNA of the endogenous Fgf8 with a PCR product of 722 bp. This pair cannot amplify the exogenous and correctly spliced Fgf8. Actb2 was amplified as a reference gene with the following primers: 5'-TGTACCCTG GCATTGCTGAC-3' and 5'-CCATGCCAATGTTGTCGTTTG-3'.

**Reverse transcriptase quantitative PCR (RT-qPCR).** Wild type embryos (10–15 embryos in each group) grown in an incubator at a given temperature (23, 26, 27, 29, or 31 °C) were fixed (as mentioned above) at the somite stages mentioned in the text. In some experiments (24, 28, and 33 °C) embryos were fixed at intervals of 1 h after onset of somitogenesis, though this procedure resulted in less reproducible and consistent results, possibly due to differences in developmental stage between the embryos. For gene quantification on specific tissue, single PSM (15 in each group) were dissected from fixed WT embryos at the last somite boundary.

**RNA extraction.** Total RNAs were extracted using the RNeasy micro kit (Qiagen) according to the manufacturer's protocols. Contaminating genomic DNA was
<figure><img src="image_10.png" /><figcaption>**Fig. 8** Variation with temperature of various gene transcripts. The δCt of genes (*her1*, *her7*, *hes6*, *deltaC*, *deltaD*, *notch1a*, *myog*, *mespa*, and *mespb*) known to play a role in somitogenesis relative to reference genes (*rpl13a* or *β-actin*) are plotted as a function of somite stage. Notice that as a function of somite stage the data taken at different temperatures collapse on the same curve. For some genes for which δCt appears to vary linearly with somite stage (exponentially decreasing concentrations) we display the best fit. For others the continuous curve is just a guide to the eye. The increasing concentration of *myog* (decreasing δCt values) is consistent with its role as a differentiation factor during myogenesis which follows somite formation.</figcaption></figure>

degraded by treatment with DNaseI (Qiagen) for 20 min at room temperature. Total RNAs were eluted in 14 µL nuclease-free water (Qiagen). RNA concentration and purity were first assessed using NanoDrop (ThermoFisher). Sample quantity and purity were estimated by measuring the ratios of spectrophotometric absorbance 280/260 nm and 260/230 nm. RNA quality and integrity were further analyzed by capillary electrophoresis (Fragment Analyzer, Agilent Technologies) to determine the RNA quality number (RQN) for each sample. Defined on a scale ranging from 1 to 10, the mean RQN of the 194 samples was 9.9, indicating very good RNA quality. RNA were stored at -80 °C before reverse transcription.

*Reverse transcription.* RNA samples were diluted at 10 ng/µL by adding nuclease-free water. cDNA synthesis was performed using Reverse Transcription Master Mix from Fluidigm™ according to the manufacturer's protocol in a final volume of 5 µL containing 40 ng total RNA. Reverse transcription was performed using a Nexus Thermocycleur (Eppendorf®) following the temperature protocol: 5 min at 25 °C, 30 min at 42 °C followed by heat-inactivation of the reverse transcriptase for 5 min at 85 °C and immediately cooled to 4 °C. cDNA samples were diluted 5× by adding 20 µL of low TE buffer [10 mM Tris; 0.1 mM EDTA; pH = 8.0] (TEKNOVA®) and stored at -20 °C before specific target pre-amplification.

*Specific target pre-amplification.* Each diluted cDNA was used for multiplex pre-amplification in a total volume of 5 µL containing 1 µL of 5× Fluidigm® PreAmp Master Mix, 1.25 µL of cDNA, 1.25 µL of pooled TaqMan® Gene Expression assays (Life Technologies, ThermoFisher) with a final concentration of each assay of 180 nM (0.2×) and 1.5 µL of nuclease-free water. The cDNA samples were subjected to pre-amplification following the temperature protocol: 95 °C for 2 min, followed by 18 cycles at 95 °C for 15 s and 60 °C for 4 min. The pre-amplified cDNA was diluted 5× by adding 20 µL of low TE buffer and stored at -20 °C before qPCR.

*High throughput qPCR.* Quantitative PCR was performed using the high-throughput platform BioMark™ HD System and the 48.48 GE Dynamic Arrays (Fluidigm®). The expression of 48 target genes was quantified in 108 samples by quantitative PCR on five 48.48 microfluidic chips. Each of the five chips contained a non-template control (NTC), and a serial dilution of a cDNA sample has been used both as a standard curve to determine efficiencies and inter-chip calibrator. The Ct obtained from the standard curve and an internal control were identical among the five chips allowing inter-chip comparisons. Six microliter of Sample

Master Mix (SMM) consisted of 2.7 µL of 5× diluted pre-amplified cDNA, 0.3 µL of 20× GE Sample Loading Reagent (Fluidigm) and 3 µL of TaqMan® Gene Expression PCR Master Mix (Life Technologies, ThermoFisher). Each 6 µL Master Mix Assay (MMA) consisted of 3 µL of TaqMan® Gene Expression assay 20× (Life Technologies, ThermoFisher) and 3 µL of 2× Assay Loading Reagent (Fluidigm). Five microliter of each SMM and each MMA premixes were added to the dedicated wells. The samples and assays were mixed inside the chip using MX IFC controller (Fluidigm). The loaded Dynamic Array was transferred to the Biomark™ real-time PCR instrument and subjected to PCR experiment (25 °C for 30 min and 70 °C for 60 min for thermal mix; 50 °C for 2 min and 95 °C for 10 min for hot start; 40 cycles at 95 °C for 15 s and 60 °C for 1 min). The parameters of the thermocycler were set with ROX as passive reference and single probe FAM-MGB as fluorescent detector. To determine the threshold cycle Ct, data were processed by automatic threshold for each assay, with linear derivative baseline correction using BioMark Real-Time PCR Analysis Software 4.0.1 (Fluidigm). The quality threshold was set at the default setting of 0.65.

*Normalization and quantification.* The reference gene *rpl13a* (or *β-actin* when mentioned in the text) has been chosen after pair-wise correlation analysis using Bestkeeper algorithm³³. The difference in the number of quantification cycles between the genes of interest (GOI) (in various conditions) and a reference gene (GRF, i.e., *rpl13a* or *β-actin*) was δCt = Ct<sub>GOI</sub> - Ct<sub>GRF</sub>. The normalized transcripts abundance (averaged over three PCR replicates) was calculated as δCt = log₂(([rpl13a])/([goi])) ~ -ln([goi])/ln2. The list of genes studied is described in Table S1.

**IHC on zebrafish embryos.** The embryos obtained in the various conditions and the different stages mentioned in the text were fixed in 4% PFA overnight at 4 °C, followed by dehydration with 100% methanol at -20 °C for more than 1 day. After gradual rehydration of methanol and wash with PBS/Tween 0.1%, the embryos were incubated in a blocking solution: 1% Triton, 1% DMSO, 1% BSA and 10% sheep serum (Sigma) in PBS on a shaker for 1 h at room temperature, followed by incubation with 1:400 Phospho-ERK Monoclonal Antibody as the primary antibody (Thermo, MA5-15173) on a shaker overnight at 4 °C. After extensive washing with PBS/Tween and incubation in blocking solution, a second antibody (anti-Rabbit conjugated to Alexa Fluor 488, Invitrogen) diluted 700× was added overnight at 4 °C. After washing with PBS/Tween, images were taken on a Nikon Ti microscope equipped with a Hamamatsu Orca camera.
**Whole-mount in-situ hybridization (ISH).** Whole-mount in-situ hybridization with digoxigenin-labeled riboprobes was performed as described previously³⁴. The antisense riboprobes were synthesized from template plasmids (gift of P. Rosa, IBENS) containing fgf8 full length cDNA³⁵. The antisense riboprobes were synthesized from template plasmids containing fgf8 full length cDNA³⁴ or xirp2a³⁶.

**Drug treatments.** Wild type embryos were incubated in 10 µM DEAB (with or without addition at 70% epiboly of 10 nM all-trans RA). The double transgenic embryos *Tg(ubi:Gal4ERT;cry:CFP;uas:fgf8-T2A-cfp;ubi:Eos)* were incubated at 70% epiboly in 3 µM cyclofen²⁷ (gift of L. Jullien) diluted in EM. DREKA embryos were treated with 50 µM, 200 µM of SU5402 (Sigma-Aldrich) at 10 somite stage for 1 h and 10 nM and 1 µM of all-trans RA (Sigma-Aldrich) from ten somite stage until observation. As controls, siblings were kept in EM.

**Fluorescent microscopy.** DREKA embryos were imaged on a Leica sp5 confocal microscope with a 20× water objective in GFP channel. All other fluorescent images were taken on a Nikon Ti microscope equipped with a Hamamatsu ORCA V2+ camera and a 10× plan fluo objective. Filter setting of CFP: excitation at 438 ± 24 nm, emission at 483 ± 32 nm; mEosFP and Alexa 488: excitation at 497 ± 16 nm, emission at 535 ± 22 nm.

**Time lapse video.** All embryos were dechorinated before bud stage using acute tweezers. The embryos were mounted in an agarose mold and kept in a temperature incubator at 27 ± 0.3 °C during imaging, following published protocols³⁸. To prevent evaporation during recording caused by the difference in temperature between the microscope room and the incubator, mineral oil (Sigma) was added to cover the surface of the medium. Time-lapse video was performed on a Nikon Ti Microscope with a 10× plan fluo objective. Images were taken by an ORCA V2 + Camera (Hamamatsu). The entire microscope system including the filter rotor, the motorized stage and the camera was driven by Micro-Manager. Up to 20 embryos per experiment were scanned at an interval of ~5 min. For each embryo, a Z-stack with six planes at 25 µm intervals was recorded.

**Image analysis of time lapse video.** Time lapse images were analyzed by FIJI. The Gaussian-based stack focuser in FIJI Time Lapse plugin was used to choose and combine the focused areas from different Z-positions of one timepoint. The measurement of tail, PSM and somite length was done using the measurement function in FIJI. ERK activity of DREKA was quantified in FIJI by the ratio between the mean fluorescence of nucleus and a 2-pixel wide cytoplasm ring.

**Statistics and reproducibility.** To assess the reproducibility of our observations, we repeated them on many embryos. Thus, measurements of growth rates and PSM shrinkage rates in different conditions were obtained from experiments on typically *n* > 10 embryos (see captions to Fig. 4e and S2b). RTqPCR measurements were done in triplicate on pooled embryos and repeated in full embryos or in the PSM (at 27 °C). Similarly experiments on the domain of activity of Erk, were done over many (*n* > 16) embryos at 27 °C (Fig. S4) and over *n* = 3 embryos at different stages and temperatures (Fig. S5). Linear fits to the data were done with maximum likelihood estimates: the value of χ² and the number of degrees of freedom (df) are indicated next to each fit (Figs. 7, S6, and S7) or in the figure captions (Figs. 5 and 6).

**Reporting summary.** Further information on research design is available in the Nature Research Reporting Summary linked to this article.

**Data availability**

Raw data are provided in Supplementary Data 1 or are available upon request from the authors.

Received: 1 August 2020; Accepted: 29 December 2021;
Published online: 07 February 2022

**References**

1. Stickney, H. L., Barresi, M. J. F. & Devoto, S. H. Somite development in zebrafish. *Dev. Dyn.* **219**, 287–303 (2000).

2. Schröter, C. et al. Dynamics of zebrafish somitogenesis. *Dev. Dyn.* **237**, 545–553 (2008).

3. Cooke, J. & Zeeman, E. C. A clock and wavefront model for control of the number of repeated structures during animal morphogenesis. *J. Theor. Biol.* **58**, 455–476 (1976).

4. Dequéant, M.-L. & Pourquié, O. Segmental patterning of the vertebrate embryonic axis. *Nat. Rev. Genet.* **9**, 370–382 (2008).

5. Bajard, L. et al. Wnt-regulated dynamics of positional information in zebrafish somitogenesis. *Development* **141**, 1381–1391 (2014).

6. Soroldoni, D. et al. Genetic oscillations. A Doppler effect in embryonic pattern formation. *Science* **345**, 222–225 (2014).

7. Gomez, C. et al. Control of segment number in vertebrate embryos. *Nature* **454**, 335–339 (2008).

8. Dubrulle, J., McGrew, M. J. & Pourquié, O. FGF signaling controls somite boundary position and regulates segmentation clock control of spatiotemporal Hox gene activation. *Cell* **106**, 219–232 (2001).

9. Sawada, A. et al. Fgf/MAPK signalling is a crucial positional cue in somite boundary formation. *Development* **128**, 4873–4880 (2001).

10. Delfini, M.-C., Dubrulle, J., Malapert, P., Chal, J. & Pourquié, O. Control of the segmentation process by graded MAPK/ERK activation in the chick embryo. *Proc. Natl Acad. Sci. USA* **102**, 11343–11348 (2005).

11. Aulehla, A. & Pourquié, O. Signaling gradients during paraxial mesoderm development. *Cold Spring Harb. Perspect. Biol.* **2**, a000869 (2010).

12. Dubrulle, J. & Pourquié, O. Fgf8 mRNA decay establishes a gradient that couples axial elongation to patterning in the vertebrate embryo. *Nature* **427**, 419–422 (2004).

13. Simsek, F. M. & Özbudak, E. M. Spatial fold change of FGF signaling encodes positional information for segmental determination in zebrafish. *Cell Rep.* **24**, 66–78 (2018).

14. Regot, S., Hughey, J. J., Bajar, B. T., Carrasco, S. & Covert, M. W. High-sensitivity measurements of multiple kinase activities in live single cells. *Cell* **157**, 1724–1734 (2014).

15. Mayr, V., Sturtzel, C., Stadler, M., Grissenberger, S. & Distel, M. Fast dynamic in vivo monitoring of Erk activity at single cell resolution in DREKA zebrafish. *Front. Cell Dev. Biol.* **6**, 111 (2018).

16. Akiyama, R., Masuda, M., Tsuge, S., Bessho, Y. & Matsui, T. An anterior limit of FGF/Erk signal activity marks the earliest future somite boundary in zebrafish. *Development* **141**, 1104–1109 (2014).

17. Sari, D. W. K. et al. Time-lapse observation of stepwise regression of Erk activity in zebrafish presomitic mesoderm. *Sci. Rep.* **8**, 4335 (2018).

18. Ishimatsu, K. et al. Size-reduced embryos reveal a gradient scaling-based mechanism for zebrafish somite formation. *Development* **145**, dev161257 (2018).

19. Xu, L. et al. Spatio-temporal manipulation of retinoic acid activity in zebrafish hindbrain development via photo-isomerization. *Development* **139**, 3355–3362 (2012).

20. Hamade, A. et al. Retinoic acid activates myogenesis in vivo through Fgf8 signalling. *Dev. Biol.* **289**, 127–140 (2006).

21. Zhang, W. et al. Control of protein activity and gene expression by cyclofen- OH uncaging. *ChemBioChem* **19**, 1232–1238 (2018).

22. Yu, S. R. et al. Fgf8 morphogen gradient forms by a source-sink mechanism with freely diffusing molecules. *Nature* **461**, 533–537 (2009).

23. Holley, S. The genetics and embryology of zebrafish metamerism. *Dev. Dyn.* **236**, 1422–1449 (2007).

24. Schröter, C. et al. Topology and dynamics of the zebrafish segmentation clock core circuit. *PLoS Biol.* **10**, e1001364 (2012).

25. Riedel-Kruse, I. H., Müller, C. & Oates, A. C. Synchrony dynamics during initiation, failure and rescue of the segmentation clock. *Science* **317**, 1911–1915 (2007).

26. Byrd, T. A. et al. Critical slowing down in biochemical networks with feedback. *Phys. Rev. E* **100**, 022415 (2019).

27. Lopez-Olmeda, J. F. & Sanchez-Vazquez, F. J. Thermal biology of zebrafish (Danio rerio). *J. Therm. Biol.* **36**, 91–104 (2011).

28. Wakamatsu, Y., Ogino, K. & Hirata, H. Swimming capability of zebrafish is governed by water temperature, caudal fin length and genetic background. *Sci. Rep.* **9**, 16307 (2019).

29. Romney, A. L. T., Davis, E. M., Corona, M. M., Wagner, J. T. & Podrabsky, J. E. Temperature-dependent vitamin D signaling regulates developmental trajectory associated with diapause in an annual killifish. *Proc. Natl Acad. Sci. USA* **115**, 12763–12768 (2018).

30. Westerfield, M. *The Zebrafish Book. A Guide for The Laboratory Use of Zebrafish* (Danio rerio) (The University of Oregon Press, 2000).

31. 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).

32. Feng, Z. et al. Optical control of tumor induction in the zebrafish. *Sci. Rep.* **7**, 9195 (2017).

33. Pfaffl, M. W., Tichopad, A., Prgomet, C. & Neuvians, T. P. Determination of stable housekeeping genes, differentially regulated target genes and sample integrity: BestKeeper—Excel-based tool using pair-wise correlations. *Biotech. Lett.* **26**, 509–515 (2004).

34. Thisse, C., Thisse, B., Schilling, T. F. & Postlethwait, J. H. Structure of the zebrafish snail1 gene and its expression in wild-type, spadetail and no tail mutant embryos. *Development* **119**, 1203–1215 (1993).

35. Furthauer, M., Thisse, C. & Thisse, B. A role for FGF-8 in the dorsoventral patterning of the zebrafish gastrula. *Development* **124**, 4253–4264 (1997).

36. Deniziak, M. et al. Loss of selenoprotein N function causes disruption of muscle architecture in the zebrafish embryo. *Exp. Cell Res.* **313**, 156–167 (2007).
37. Sinha, D. K. et al. Photocontrol of protein activity in cultured cells and zebrafish with one- and two-photon illumination. *Chembiochem* 11, 653–663.37 (2010).

38. Herrgen, L., Schröter, C., Bajard, L., & Oates, A. C. *Zebrafish* 243–254 (Humana Press, 2009).

## Acknowledgements

We thank A. Oates and D. Soroldini for their help and support with time-lapse microscopy on zebrafish embryos. We further acknowledge C. Gauron and M. Volovitch for their help in the construction of transgenic fish and L. Jullien for his support with cyclofen and its derivatives. We thank them all and A. Goldbeter and V. Hakim for constructive criticism during the conduction of this work. This work was partially supported by grants ANR-10-LABX-54 MEMO LIFE and ANR-11-IDEX-0001-02 PSL* Research University and PSL grants SuperLINE and MicroGUT. The gene expression analysis was carried out on the high throughput qPCR-HD-Genomic Paris Centre core facility and was supported by grants from the Région Ile de France. Animal protocols followed CNRS guidelines.

## Author contributions

W.Z. and D.B. planned and analyzed the experiments W.Z. and P.S. performed most of the experiments. W.Z., B.D., V.C., and M.De. performed the RT-qPCR experiments, S.V., V.M., and M.Di. developed some of the zebrafish lines used here. W.Z., P.S., B.D., and D.B. wrote the paper.

## Competing interests

The authors declare no competing interests.

## Additional information

**Supplementary information** The online version contains supplementary material available at https://doi.org/10.1038/s42003-022-03053-0.

**Correspondence** and requests for materials should be addressed to Bertrand Ducos or David Bensimon.

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<figure><img src="image_11.png" /></figure>

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