Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

NDR Kinases Are Essential for Somitogenesis and Cardiac Looping during Mouse Embryonic Development

NDR Kinases Are Essential for Somitogenesis and Cardiac Looping during Mouse Embryonic Development

  • Debora Schmitz-Rohmer, 
  • Simone Probst, 
  • Zhong-Zhou Yang, 
  • Frédéric Laurent, 
  • Michael B. Stadler, 
  • Aimée Zuniga, 
  • Rolf Zeller, 
  • Debby Hynx, 
  • Brian A. Hemmings, 
  • Alexander Hergovich


Studies of mammalian tissue culture cells indicate that the conserved and distinct NDR isoforms, NDR1 and NDR2, play essential cell biological roles. However, mice lacking either Ndr1 or Ndr2 alone develop normally. Here, we studied the physiological consequences of inactivating both NDR1 and NDR2 in mice, showing that the lack of both Ndr1/Ndr2 (called Ndr1/2-double null mutants) causes embryonic lethality. In support of compensatory roles for NDR1 and NDR2, total protein and activating phosphorylation levels of the remaining NDR isoform were elevated in mice lacking either Ndr1 or Ndr2. Mice retaining one single wild-type Ndr allele were viable and fertile. Ndr1/2-double null embryos displayed multiple phenotypes causing a developmental delay from embryonic day E8.5 onwards. While NDR kinases are not required for notochord formation, the somites of Ndr1/2-double null embryos were smaller, irregularly shaped and unevenly spaced along the anterior-posterior axis. Genes implicated in somitogenesis were down-regulated and the normally symmetric expression of Lunatic fringe, a component of the Notch pathway, showed a left-right bias in the last forming somite in 50% of all Ndr1/2-double null embryos. In addition, Ndr1/2-double null embryos developed a heart defect that manifests itself as pericardial edemas, obstructed heart tubes and arrest of cardiac looping. The resulting cardiac insufficiency is the likely cause of the lethality of Ndr1/2-double null embryos around E10. Taken together, we show that NDR kinases compensate for each other in vivo in mouse embryos, explaining why mice deficient for either Ndr1 or Ndr2 are viable. Ndr1/2-double null embryos show defects in somitogenesis and cardiac looping, which reveals their essential functions and shows that the NDR kinases are critically required during the early phase of organogenesis.


The NDR (nuclear Dbf2-related) family of serine/threonine protein kinases represents a subclass of the AGC (protein kinase A (PKA)/PKG/PKC-like) kinases [1]. The mammalian genomes encode two highly related NDR kinases with 86% amino acid identity, called NDR1 and NDR2 (also termed STK38 and STK38L, respectively) [24]. Members of the NDR family are well conserved with important and in general essential roles in uni- and multi-cellular eukaryotes including yeast, fungi, plants, flies and mammals [1].

Studies in budding and fission yeast demonstrated that yeast NDR kinases are essential for survival of these unicellular organisms (summarized in [1]). Genetic inactivation of the Drosophila NDR kinase results in lethality during embryonic and/or larval development [5]. This lethality is rescued by expression of the human NDR1 kinase [6], suggesting that NDR kinases have conserved essential roles in multicellular organisms. However, Ndr1-deficient mice develop normally, are fertile and have normal life spans [7]. Similarly, it has been reported that mice deficient for Ndr2 are born at the expected Mendelian frequency [8]. These findings are surprising considering the vital functions of NDR kinases in other species [1] and tissue culture-based experiments, which suggest that mammalian NDR kinases are essential for cellular processes such as centrosome duplication [9, 10], ciliogenesis [11], apoptosis [7, 12, 13] and cell cycle progression [1419]. However in contrast to Ndr1-deficient mice [7], the currently available Ndr2-deficient mice [8] were generated by a gene-trap insertion in intron 9 of the murine Ndr2 gene, which results in expression of a NDR21-282::β-geo fusion protein [8]. Thus, analysis of complete loss-of-function Ndr2 mice is needed to firmly establish if inactivation of Ndr2 does really not alter viability. Therefore, to study the physiological importance of NDR1 and NDR2 kinases in vivo, we analyzed mice deficient for either Ndr1 or Ndr2 and double mutant mice. Significantly, our genetic analysis reveals that a single wild-type allele of Ndr1 or Ndr2 is able to sustain normal embryonic development, while complete inactivation Ndr1 and Ndr2 causes embryonic lethality. Ndr1/2-double null embryos displayed striking somite patterning defects and an early arrest in cardiac looping. The severe cardiac insufficiency appears to be the likely cause of the embryonic lethality at mid-gestation.


Ndr2-deficient mice are phenotypically normal

Ndr2-deficient mice were generated by deleting coding exon 2 (Fig 1A), which encodes the Ndr2 translation initiation codon [3]. Genotype analysis confirmed successful targeting of the Ndr2 gene (Fig 1B; data not shown). Western blotting showed that the NDR2 protein was absent in Ndr2-deficient mice (Fig 1C). Similar to Ndr1-deficient mice [7], a gene-dosage effect was observed such that NDR2 protein levels already decreased in heterozygote mice (Fig 1C). As previously reported for Ndr1-deficient mice [7], and in full agreement with the analysis of Ndr2 gene-trap allele [8], mice lacking the NDR2 protein were born at the expected Mendelian ratio, fertile and had a normal lifespan (Fig 1D; data not shown).

Fig 1. Generation and validation of Ndr2 knock-out mice.

(A) Genomic structure of the Ndr2 locus in the mouse and targeting vector for Ndr2 inactivation. Exons 1–4, and LoxP sites are indicated. Crosses with Cre-deleter mice removed exon 2, generating an Ndr2 loss-of-function allele. (B) Genotyping of wild-type (+/+), heterozygous (+/-) and homozygous Ndr2 knock-out (-/-) samples by PCR analysis. (C) Western blot analysis of NDR2 protein in colon lysates of wild-type (+/+), heterozygous (+/-) and homozygous Ndr2-deficient (-/-) littermates. (D) Genotype distribution of offspring from Ndr2 heterozygous intercrosses. Genotypes were determined by PCR analysis at weaning.

Increased hydrophobic motif phosphorylation of the remaining NDR isoform in Ndr-single KO tissues

Ndr1 and Ndr2 display partially overlapping expression patterns and in all mouse tissues examined so far at least one of the two NDR isoforms is expressed [24, 7, 8]. While NDR1 protein levels are highest in organs of the immune system (thymus, spleen and lymph nodes), NDR2 protein levels peak in the colon and brain [24, 7, 8]. Intriguingly, NDR2 protein levels are post-transcriptionally up-regulated upon ablation of Ndr1, suggesting a compensatory link between the two NDR isoforms [7]. More precisely, up-regulation of NDR2 occurs particularly in tissues with high NDR1 expression in the wild-type situation [7]. To address whether the inactivation of Ndr2 is also compensated by up-regulation of NDR1 protein, we analyzed thymus and colon tissue lysates of Ndr2 wild-type, heterozygous and deficient adult littermate mice (Fig 2A). While NDR1 protein levels in the thymus of Ndr2 heterozygous and deficient mice remained unchanged, NDR1 protein levels appeared to be increased in the colon of Ndr2-deficient mice (Fig 2A). This suggested that NDR1 compensates for loss of NDR2 in the colon, a tissue where NDR2 is normally highly expressed.

Fig 2. The remaining NDR isoform is upregulated in tissues of mice lacking one of the two Ndr genes.

(A) Western blot analysis of NDR1 and NDR2 expression in thymus and colon of wild-type (+/+), Ndr2 heterozygous (+/-) and Ndr2-deficient (-/-) mice. (B) Western Blot analysis of NDR1 and NDR2 proteins in brain, colon, heart, thymus, spleen and lymph nodes (LN) of wild-type (wt), Ndr1-deficient (ko 1) and Ndr2 deficient (ko 2) mice. Hydrophobic motif phosphorylation, which serves as a direct indicator of NDR kinase activity, was examined using anti-phospho-T444/T442 antibodies (detecting NDR1 and NDR2 equally well [65]). The upper band corresponds to T442-P of NDR2, the lower band corresponds to T444-P of NDR1 [65]. HSC-70 served as loading control. Asterisks indicate compensatory HM phosphorylation events.

Using tissue culture systems, human NDR kinases were shown to play roles in centrosome duplication, apoptosis and cell cycle progression [20]. In all three processes, the hydrophobic motif (HM) phosphorylation of human NDR1 on Thr444 is essential, since rescue-experiments with the NDR1 T444A phospho-acceptor mutant did not compensate for loss of the wild-type protein [10, 12, 14, 19]. These studies indicated that Thr444/Thr442 phosphorylation is essential for, and reflects, NDR1/2 kinase activities [20]. Therefore, we determined whether the up-regulation of the remaining NDR isoform in single mutants tissues was paralleled by an increase in HM phosphorylation, which is a direct sensor of NDR kinase activity [20]. We detected apparently increased HM phosphorylation of NDR2 in the colon, thymus, spleen and lymph nodes of Ndr1-deficient mice, where NDR2 HM phosphorylation is normally low (Fig 2B). Conversely, NDR1 HM phosphorylation appeared to be elevated in the colon when Ndr2 was inactivated (Fig 2B). In summary, our findings indicated that murine NDR1 and NDR2 may functionally compensate for each other in vivo, which would explain why mice lacking either Ndr1 or Ndr2 are viable and fertile.

NDR kinases are essential for normal development after embryonic day E8

To address whether NDR kinases play an essential role during murine embryonic development in vivo, we generated mice lacking both Ndr1 and Ndr2 (hereafter called Ndr1/2-double null). However, intercrossing Ndr1+/- and Ndr2+/- mice did not result in surviving Ndr1/2-double null mice (Table 1). Ndr1+/-Ndr2-/- and Ndr1-/-Ndr2+/- mice, which retained only one wild-type Ndr allele, were born fertile and did not display overt phenotypes (Table 1; data not shown), indicating that a single remaining wild-type allele is sufficient for normal development and reproduction, while complete loss of Ndr1/2 results in embryonic lethality.

Table 1. Ndr1/2-double null mice are embryonic lethal, but a single Ndr allele is sufficient to sustain normal development.

To gain insight into the essential embryonic functions of NDR kinases, we analyzed Ndr1/2-double null embryos. At embryonic day 10.5 (E10.5), Ndr1/2-double null embryos suffered from severe growth retardation and were resorbed (Table 2; data not shown), indicating that NDR kinases are essential prior to this developmental period. At E10.5 all Ndr1/2-double null embryos isolated were dead (Table 2). Analysis of younger embryos revealed viable Ndr1/2-double null embryos at expected Mendelian ratio up to E9.5 (Table 2). However, already at E8.5 Ndr1/2-double null embryos appeared smaller and developmentally delayed as judged by their somite numbers (Fig 3A, 3B and 3C). Wild-type littermates had on average ten somites, while Ndr1/2-double null embryos had only six to seven somites at E8.5 (Fig 3C). Somites of Ndr1/2-double null embryos appeared also smaller and less defined (Fig 3B).

Fig 3. NDR kinases are essential for growth, cardiac development and blood vessel remodeling from about embryonic day 8 onward in mouse embryos.

(A, B) Bright field images of wild-type (A) and Ndr1/2-double null (B) littermates at E8.5. Both embryos are of the 6-somite stage. Note that the Ndr1/2-double null somites are small and irregularly shaped. Scale bars correspond to 500μm. (C) Average somite numbers of wild-type and Ndr1/2-double null littermates at E8.5. Data correspond to the analysis of a total of 15 litters and are blotted as box and whisker chart illustrating the distribution of somite numbers per litter and genotype. Average somite numbers are indicated. (D, E) Distribution of Shh (D) and T/brachyury (E) transcripts in wild-type (left) and Ndr1/2-double null littermate embryos (right) at E8.5. Four animals per genotype were analyzed, and all embryos displayed the staining shown in Fig 3D and 3E. (F, G, H) Bright field images of wild-type (F) and Ndr1/2-double null (G, H) littermate embryos at E9.5. 56 Ndr1/2-double null and 163 control embryos at E9.5 were analyzed. White arrow in H points to the pericardial edema. Scale bars correspond to 500μm. (I, J) Bright field images of the yolk sacs of wild-type (I) and Ndr1/2-double null (J) littermate embryos at E9.5. All Ndr1/2-double null yolk sacs (n = 56) displayed defective vascular development as illustrated in Fig 3J.

The notochord, a rod-like structure underlying the neural tube, participates in somite and neural tube patterning by secreting the Sonic Hedgehog (SHH) morphogen [21]. While SHH is essential to maintain the notochord [22], its formation depends on the T-box transcription factor T/Brachyury [23]. Therefore, we analyzed the expression of Shh (Fig 3D) and T/Brachyury in wild-type and Ndr1/2-double null embryos at E8.5 (Fig 3E). This analysis showed that the expression of both genes remained unaltered in Ndr1/2-double null embryos at E8.5, which pointed to normal notochord architecture and functions in Ndr1/2-double null embryos (Fig 3D and 3E). Four animals per genotype were analyzed, and all embryos displayed the staining shown in Fig 3D and 3E.

By E9.5, the size differences between wild-type and Ndr1/2-double null embryos were about two-fold (Fig 3F, 3G and 3H). Moreover, 50% of Ndr1/2-double null embryos had still not turned (Fig 3G), while wild-type embryos completed the turning process between E8.5 and E9.0 [24] (data not shown). Furthermore, approximately 50% of Ndr1/2-double null embryos had developed pericardial edema (Fig 3H) as indicated by excessive fluid accumulation in the heart region due to cardiac malfunction. Despite this impairment, cardiac contractions were observed in several Ndr1/2-double null embryos at E9.5 (data not shown). The yolks sacs of Ndr1/2-double null embryos also differed strikingly from their wild-type counterparts. In contrast to yolk sacs of wild-type embryos that had undergone extensive remodeling of the vascular plexus with readily detectable macroscopic blood vessels (Fig 3I), large remodeled vessels were absent from yolk sacs of Ndr1/2-double null embryos at E9.5 (Fig 3J). Specifically, at E9.5 all Ndr1/2-double null yolk sacs (n = 56) displayed defective vascular development as shown in Fig 3J (compare Fig 3I and 3J). Since some red blood cells were detected in yolk sacs of Ndr1/2-double null embryos, primitive hematopoiesis appeared to have occurred to a certain extent in the absence of NDR kinases. The allantois of Ndr1/2-double null embryos was well developed and attached to the chorion in all cases (data not shown).

The CDK inhibitor p21/Cip1 is up-regulated in Ndr1/2-double null embryos

In the search for a possible molecular mechanism underlying the observed embryonic lethality, gene expression analyses comparing Ndr1/2-double null embryos with controls was done (S1 and S2 Tables). Although the phenotype was more severe at E9.5, the analyses focused on Ndr1/2-double null embryos at E8.5 in the hope to identify the primary defects caused by loss of the NDR kinases. Both Ndr1 and Ndr2 transcripts are broadly expressed at E8.5 as assessed by RNA in situ hybridization (S1 Fig). As embryonic development proceeds extremely fast, we focused our transcriptome analysis on embryos with seven to nine somites. The list of differentially expressed genes in Ndr1/2-double null embryos did not reveal any signature of apoptotic genes (S1 and S2 Tables). In line with these data, TUNEL analysis detected only few apoptotic cells in both wild-type and Ndr1/2-double null embryos at E8.5 (S2 Fig), indicating that the developmental delay was not due to increased apoptosis. Since in the intestinal epithelium of adult mice, NDR kinases were recently shown to regulate the growth promoting YAP proto-oncoprotein [25], we next investigated the expression of known YAP target genes in embryos [26] by comparing wild-type to Ndr1/2-double null embryos. However, this analysis revealed that the expression of YAP target genes is not altered in Ndr1/2-double null embryos at E8.5 (S3 Fig and S1 and S2 Tables).

Intriguingly, the microarray analysis (S1 and S2 Tables) revealed that Cdkn1a and Cdkn1b transcripts, which encode the cyclin-dependent kinase (CDK) inhibitors p21/Cip1 and p27/Kip1, were up-regulated about 1.5 fold in Ndr1/2-double null embryos (Fig 4A). Quantitative real-time PCR analysis confirmed the up-regulation of p21 in Ndr1/2-double null embryos, while the increase in p27 expression was not confirmed (Fig 4B). Moreover, Krüppel-like 6 (Klf6) transcripts were elevated in Ndr1/2-double null embryos (Fig 4A). As the transcription factor Klf6 directly activates p21 expression [27, 28], it is possible that their up-regulation is linked in Ndr1/2-double null embryos. Endogenous p21 has been shown to restrict cellular proliferation in vivo [29, 30], hence the up-regulation of p21 as cell cycle inhibitor indicates that the reduced size of Ndr1/2-double null embryos could be at least in part a consequence of impaired cell cycle progression.

Fig 4. The CDK inhibitor p21/Cip1 is up-regulated in Ndr1/2-double null embryos and required for survival.

(A) Changes in transcript levels between wild-type and Ndr1/2-double null embryos at E8.5 as revealed by microarray analysis (see S1 and S2 Tables). (B) Validation of the alterations in p21 and p27 expression in wild-type (control) and Ndr1/2-double null embryos by qRT-PCR (at E8.5). Data shown represent the average gene expression levels obtained by analyzing three independent embryos per genotype. Each embryo was analyzed in triplicate. Statistical analysis was performed using a two-tailed Student t-test assuming unequal variance. (C) Genotype distribution of offspring from Ndr1+/-;Ndr2-/-;p21+/- intercrosses. Embryos were isolated at E8.5 and genotyped. Top panel: p21 genotype of the Ndr1/2-double null embryos; bottom panel: Ndr1 genotype of the p21-null embryos. The p-values are indicative of the probabilities to obtain the observed genotype distribution by chance.

In this regard, we analyzed the mitotic index of Ndr1/2-double null and wild-type embryos based on phospho-H3 staining, revealing that the mitotic index does not appear to be affected by complete Ndr1/2 loss at E8.5 (S4 Fig). However, in a rapidly growing embryo, even minor changes in cell cycle duration may result in significant size differences. Thus, we developed a simple model to mathematically approximate the effect of increased cell cycle duration from E7.5 to E8.5 in mouse development (S5 Fig). This model revealed that a 20% increase in mean cell cycle duration during this period would suffice to generate the 1.5 fold size difference as observed between normal and Ndr1/2-double null littermates at E8.5 (Fig 3). Collectively, this suggests that the cell cycle progression in Ndr1/2-double null embryos deserves future investigations using highly sophisticated approaches.

p21 becomes essential for embryonic development in Ndr1/2-double null embryos

To further investigate the potential contribution of the transcriptional up-regulation of p21 to the developmental arrest of Ndr1/2-double null embryos, we asked whether concomitant loss of p21 would rescue the growth defect of Ndr1/2-double null embryos. Previous analysis had established that p21 KO animals are viable and fertile and do not show any overt developmental phenotype [31]. However, to our surprise, we were unable to obtain mice carrying a single wild-type Ndr1 single allele on a p21-deficient background (Ndr1+/-;Ndr2-/-;p21-/-). In contrast, mice carrying one wild-type Ndr1 single allele heterozygous for the p21 loss-of-function (Ndr1+/-;Ndr2-/-;p21+/-) were born at the expected Mendelian ratios (data not shown). These findings suggest that upon reduction of the Ndr gene dose to one functional copy, p21 becomes essential for normal embryonic development. We confirmed this finding by analyzing embryos from Ndr1+/-;Ndr2-/-;p21+/- intercrosses, which revealed that all of the eight Ndr1/2-double null (Ndr1-/-;Ndr2-/-) embryos isolated at E8.5 carried two wild-type p21 alleles (Fig 4C, top). Conversely, all of the nine p21-deficient embryos recovered at E8.5 were wild-type for Ndr1 (Fig 4C, bottom). Consequently, these findings point to an unexpected genetic dependency of p21 and Ndr1/2 kinases during embryonic development, hence additional studies are needed to gain insight into how the NDR- and p21-dependent signaling pathways interact during embryonic development.

Analysis of abnormal somite development in Ndr1/2-double null embryos

The microarray data also revealed a set of genes predominantly expressed in somites or being implicated in somitogenesis that were down-regulated in Ndr1/2-double null embryos, which includes the transcription factors Meox1, Meox2, Tbx6 and Mesogenin1 (Fig 5A). Mesogenin1 is essential for presomitic mesoderm maturation [32], Meox1 and Meox2 are essential for normal somitogenesis [33], and reduction of Tbx6 disrupts somite patterning [34, 35]. Therefore the expression of these genes was analyzed by whole mount RNA in situ hybridization in E8.5 wild-type and Ndr1/2-double null embryos (Fig 5B to 5D). In wild-type embryos (Fig 5B, left embryo), Meox1 expression demarcated the somite boundaries and revealed the even distances between somite pairs. In Ndr1/2-double null embryos (Fig 5B, right embryo), Meox1 expression was decreased, somite borders appeared fuzzy, distances between somites varied and the positions of the last formed somites was not well defined. Analysis of the Tbx6 and Mesogenin1 expression patterns confirmed their down-regulated expression in Ndr1/2-double null embryos (Fig 5C and 5D). Analysis of somite morphology revealed that the size of Ndr1/2-double null somites was significantly reduced (Fig 5E, six somites stage at E8.5). In summary, Ndr1/2 deficiency results in transcriptional down-regulation of genes involved in somite formation by E8.5. Somites of Ndr1/2-double null embryos were smaller, irregularly shaped and unevenly spaced along the anterior-posterior (AP) embryonic axis, which indicates that NDR kinases function in somite formation and spacing.

Fig 5. Somitogenesis is altered in Ndr1/2-double null embryos.

(A) Changes in gene expression between wild-type and Ndr1/2-double null embryos at E8.5 determined by microarray analysis (see S1 and S2 Tables). (B, C, D) Distribution of Meox1 (B), Tbx6 (C) and Mesogenin1 (D) transcripts in wild-type (wt) and Ndr1/2-double null embryos at E8.5. Four animals per genotype were analyzed for Meox1 staining, and two embryos per genotype were analyzed for Tbx6 and Mesogenin staining. All embryos displayed the staining patterns as shown in Fig 5B, 5C and 5D. (E) Hematoxylin/Eosin staining of transversal (left) and parasagittal (right) sections of wild-type (top panels) and Ndr1/2-double null (bottom panels) embryos at the 6-somite stage. Six embryos of each genotype were analyzed. PSM: presomitic mesoderm; SI, SII, SIII: last, second to last and third to last formed somite. Scale bars = 50μm. (F, G, H) Distribution of Snail1 (F), Axin2 (G) and Lnfg (H) transcripts in wild-type (wt) and Ndr1/2-double null embryos. Asterisk (*) indicates aberrant asymmetrical expression (right) of Lnfg in the last formed somite pair. Seven embryos were analyzed per genotype for Snail1 staining, and five embryos were analyzed per genotype for Axin2 staining. The expression patterns of Snail1 and Axin2 appeared indistinguishable between all mutant and control embryos. Nine mutant and four control embryos were analyzed for Lnfg staining. All four control embryos showed the expected symmetric expression pattern as illustrated in Fig 5H. In contrast, four of nine mutant embryos displayed strongly asymmetric Lnfg expression and one mutant embryo showed mild asymmetric expression.

Asymmetric expression of the Notch pathway component Lunatic Fringe in the last formed somite in Ndr1/2-double null embryos

Somitogenesis is a highly symmetrical process such that the left and the right somite of each pair form together. The so-called segmentation clock coordinates somite formation by ensuring the formation of somite pairs in a periodic fashion (reviewed in [36]). The segmentation clock is operated by cyclic expression of distinct members of the FGF, Wnt and Notch pathways [36]. Interestingly, we noted that the expression of the WNT antagonist Sfrp1 (secreted frizzled-related protein 1) was decreased in Ndr1/2-double null embryos (Fig 5A). In addition, the expression of three components of the Notch signaling pathway was also reduced in Ndr1/2-double null embryos, namely Lunatic fringe (Lnfg) and the Notch ligands Delta-like Dll1 and Dll3 (Fig 5A). Sfrp1 was previously shown to regulate A-P axis elongation and somite segmentation in conjunction with Sfrp2 in mouse embryos [37]. LNFG negatively regulates Notch signaling and Lnfg-null mice display defects in somitogenesis [38], while Dll1 and Dll3 are essential for somite formation [39, 40] and establishment of the inter-somitic boundaries [41]. Thus, the deregulation of these genes in Ndr1/2-double null embryos could be cause or consequence of the observed somitogenesis defects. Therefore, the expression of the Snail1 [42], Axin1 [43] and Lnfg genes was analyzed during somitogenesis (Fig 5F, 5G and 5H). The expression patterns of Snail1 (Fig 5F) and Axin2 (Fig 5G) were indistinguishable between all mutant and control embryos. In contrast, the Lnfg expression, which is a negative regulator of the Notch pathway, was altered in Ndr1/2-double null embryos at E8.5 (Fig 5H). In contrast to its normal symmetrical expression in wild-type embryos (Fig 5H, top panel), Lnfg expression was asymmetric in the last formed somite pair in 50% of Ndr1/2-double null embryos (Fig 5H, bottom panel). The asymmetric Lnfg expression pattern suggests that formation of the last somite pair occurred in a temporally discoordinate fashion. This indicates that NDR kinases are required for symmetric Lnfg expression and bilaterally coordinated somite formation (see discussion).

NDR kinases are essential for cardiac looping during mouse embryonic development

Aberrant somitogenesis is unlikely to account for embryonic lethality since heart development is not disrupted in mouse embryos lacking Meox1/2, which severely disrupts somites and results in the absence of the axial skeleton [33]. The heart is essential for survival for the embryo from early organogenesis onward [44]. The primitive heart tube forms around E8.0 [45, 46], begins to rhythmically contract at around the 3-somite stage and the onset of blood flow commences around 4 to 6 somites [47]. The development of the linear heart tube into the four-chambered adult heart occurs by cardiac looping and is the first morphologically distinct asymmetric structure during organogenesis. Cardiac looping is initiated between E8.0 and E8.5 [48] and is categorized into the heart looping stages (LS) zero to III [49]. At LS-0, the A/P axis of the heart is parallel with that of the neural tube and pharynx. At LS-I, the heart tube starts to display asymmetric development by adopting a tilted A/P axis in the left/right plane. At LS-II, a separate atrial chamber and atrioventricular sulcus are first apparent in the heart tube, while looping of the ventricular region is yet absent or minimal. At LS-III, overt ventricular looping begins together with asymmetrical atrial development. At this stage, the left ventricle expands, thereby occupying space in front of the atrial chamber and left sinus venosus.

Comparative analysis of developing hearts at E8.5, showed that while wild-type hearts had progressed to LS-III with prominent rightward looping (Fig 6Ai), the looping of Ndr1/2-double null hearts remained in stage LS-II (Fig 6Aii). In addition, Ndr1/2-double null hearts displayed a bulbous morphology and appeared less transparent than wild-type controls (data not shown), which pointed to either a thickened myocardium or a reduced heart lumen. To determine whether this striking heart phenotype was due to a developmental delay or arrest, E9.5 embryos were analyzed (Fig 6B and 6C). While the looping process had progressed in wild-type hearts (Fig 6Bi and 6Ci), the heart looping of Ndr1/2-double null embryos remained arrested at LS-II at E9.5 (Fig 6Bii and 6Cii). In agreement with this observation, no rightward looping of Ndr1/2-double null embryonic hearts was observed. In addition, Ndr1/2-double null embryos appeared smaller than their wild-type litter mates at E9.5, but organogenesis was not arrested at this stage (Fig 3). OPT (Optical Projection Tomography) analysis established that the lumen of the developmentally arrested Ndr1/2-double null embryonic hearts had not formed properly (Fig 6D and 6E). Indeed, analysis of histological sections revealed that the myocardium of Ndr1/2-double null embryonic hearts was thickened (Fig 6Fii, 6Gii and 6Hii) and the cardiac jelly and/or lumen contained additional cells (indicated by arrows in Fig 6Fii, 6Gii and 6Hii). Taken together, the pericardial edema (Fig 3H), arrest of cardiac looping (Fig 6A, 6B and 6C) and defects in the heart lumen (Fig 6D to 6H) indicated that these cardiac defects are the likely cause of the embryonic lethality of Ndr1/2-double null embryos during early mouse organogenesis.

Fig 6. Murine NDR kinases are essential for cardiac looping.

(A) OPT 3D reconstruction of wild-type (Ai) and Ndr1/2-double null (Aii) embryos at E8.5. Blue: anatomy. Red: Nkx2.5 whole mount in situ hybridization. Embryo axis orientation: a: anterior, p: posterior, l: left, r: right. Two Ndr1/2-double null and two control embryos were examined. Using bright field microscopy ten Ndr1/2-double null and ten control embryos were analysed at E8.5 to confirm the observed phenotype (data not shown). (B, C) Bright field images of wild-type (Bi, Ci) and Ndr1/2-double null (Bii, Cii) developing hearts at E9.5. B: frontal view; C: lateral view. Scale bars = 100μm. Embryo axis orientation: a: anterior, p: posterior, l: left, r: right, d: dorsal, v: ventral. Five Ndr1/2-double null and five control embryos were analyzed. (D, E) OPT virtual section of wild-type (Di, Ei) and Ndr1/2-double null (Dii, Eii) embryos shown in 6A. Panel D: coronal plane; panel E: transversal plane. Labels: a: anterior, p: posterior, d: dorsal, v: ventral. Arrows point to the heart. Two Ndr1/2-double null and two control embryos were analyzed for OPT as shown in 6D and 6E. (F, G, H) Hematoxylin and Eosin stained transversal sections of a wild-type (Fi, Gi, Hi) and Ndr1/2-double null (Fi, Gi, Hi) hearts at the 6-somite stage. The myocardium (MC) and headfolds (HF) are indicated in (Fi) and (Fii). Arrows in (Fii), (Gii) and (Hii) point to remaining cells in the cardiac jelly and lumen. Note the similar section plan between the embryos shown in (E) and (G). Three Ndr1/2-double null and three control embryos were analyzed. (J) Scheme showing the approximate level of the sections within the embryo. The distance between sections is about 30μm.


Here, we investigated the essential roles of the murine NDR1 and NDR2 kinases. As previously reported for Ndr1-deficient mice [7], mice lacking Ndr2 develop normally and are fertile. This is likely due to functional compensation as the levels and HM phosphorylation of the other NDR isoform were up-regulated in mice lacking only one of the two Ndr genes (this study and ref. [7]). We now establish that complete genetic inactivation of both Ndr genes in mice causes embryonic lethality around E10. In particular, our analysis establishes that NDR kinases are essential for mouse embryonic heart and somite development. The small and irregular somite morphology in Ndr1/2-double null embryos is accompanied by downregulation of genes functioning in somitogenesis such as Meox1/2 [33]. However, the observed somite defects observed in Ndr1/2-double null embryos are less severe than the ones observed following genetic inactivation of Lnfg and the Notch Delta-like ligands Dll1, Dll3 in mice [3840]. Interestingly, the normally symmetric expression of Lnfg transcripts becomes asymmetric in the last formed somite pair in Ndr1/2-double null embryos. The unilateral posterior expanded expression of Lnfg is indicative of temporal heterochrony in the formation of left and right somites. This indicates that NDR kinases are part of the mechanism by which somites normally escape the already existing left-right asymmetry along the primary embryonic axis [36, 50]. Possibly NDR kinases play a role in the conserved ‘clock-and-wavefront’ mechanism controlling somitogenesis [51] and/or also contribute to the retinoic acid-mediated coordination of somitogenesis and left-right patterning [5255]. Therefore, future research into the underlying molecular and cellular mechanisms is warranted.

Additional evidence in favor of a possibly more general role of NDR kinases downstream of establishing L/R asymmetry [36] is their essential role during cardiac looping [46, 56], which arrests at an early stage in Ndr1/2-double null embryos (this study). In addition, the thickened myocard and remaining cells in the cardiac jelly and lumen will likely interfere with normal blood flow and hamper normal embryo growth and organogenesis of Ndr1/2-double null embryos, resulting in their death during mid-gestation. Since remodeling of the yolk sac vasculature depends on hemodynamic forces exerted by blood flow [47] the observed defects in the yolk sac vasculature are likely secondary to the heart defects in Ndr1/2-double null embryos.

Much progress has been made in deciphering the transcriptional networks that govern the patterning of the vertebrate heart [56]. However, we did not identify changes in the expression of major regulators of cardiac development in Ndr1/2-double null embryos at E8.5, therefore the underlying molecular alteration resulting in arrest of cardiac looping remain unknown. In general, the mechanism underlying cardiac looping are not well defined [49, 57], but studies indicate that changes in myocardial cell shape, actin re-arrangements and extra-cellular matrix remodeling are key events during cardiac looping [5861]. In this context, it is noteworthy that over-expressed human NDR2 associates with actin [4] and that one of the yeast NDR kinases interacts with the actin cytoskeleton [1]. Thus, the murine NDR kinases might function during cardiac looping by impacting on the underlying cytoskeleton re-arrangements. Consequently, more in depth molecular analysis will be needed to gain a better understanding of the possibly common and/or distinct roles of NDR kinases during mouse embryonic somitogenesis and cardiac looping.

It has been previously established that MST1/2 kinases function as direct upstream kinases of NDR1 and NDR2 in mammalian cells in culture [10, 12]. The genetic analysis of the Mst1/2 [6264] and Ndr1/2 kinases in mice (this study) reveals striking similarities with respect to their genetic requirement and phenotypes: (a) a single wild-type allele of either Ndr1/2 or Mst1/2 is sufficient to sustain normal embryonic development, while complete inactivation of either the Ndr1/2 or Mst1/2 genes causes mid-gestational embryonic lethality; (b) Ndr1/2-double null and Mst1/2-null embryos are growth-retarded and developmentally delayed by E8.5; and (c) both types of null embryos display pericardial edema and a defective yolk sac vasculature (this study and refs. [6264]). These similarities in embryonic mutant phenotypes is in agreement with the notion that NDR kinases might act as down-stream effectors of MST1/2 signaling during mouse embryonic development.

Taken together, our genetic analysis points to essential functions of mouse NDR kinases during early embryonic growth, temporally and spatially symmetric formation of somite pairs, early heart looping and chamber development.

Materials and Methods

Ethics statement (for animal experiments)

All studies with mice were approved by the Swiss Cantonal Veterinary Office of both Basel and Argovia. All mouse experimental analysis was performed in strict compliance with the animal welfare and ethic regulations and 3R principles as defined by the Swiss Federal laws governing animal research (Animal Welfare Act; Animal Welfare Ordinance; Animal Experimentation Ordinance).

Study design

To investigate the role of murine NDR kinases in embryonic development, we compared Ndr1/2-double null mouse embryos and control littermates ranging in developmental age from E8.5 to E10.5 using different approaches, namely gross morphological analyses via bright field microscopy, RNA in situ hybridization, histological analyses (H&E and TUNEL), Optical Projection Tomography (OPT), microarray analyses and quantitative real-time PCR. All methods are described in detail in the respective sections below.

Animal experiments

Results described here were from ex-vivo analysis of embryos post-mortem. Timed mating of naïve mice were performed to calculate correct Embryo age. When possible after timed mating, females were group housed. Breeding strategy for analysis of DKO embryonic lethality was optimized for DKO generation with single KO controls. None of the animals received study specific treatment. To obtain embryos, pregnant females were sacrificed by cervical dislocation prior to removal of embryos.

Targeting of the murine Ndr2 locus and mouse breeding

We introduced loxP sites up- and downstream of exon 2 of Ndr2 via homologous recombination in Ola129 ES cells. Two independent ES cell clones (validated by Southern blotting, PCR and DNA sequencing) were expanded and aggregated with E2.5 morulas followed by re-implantation into pseudo-pregnant foster mothers. Chimeric offspring were crossed with the Meox2-Cre delete strain (B6.129S4-Meox2tm1(cre)Sor/J) to delete Ndr2 constitutively (B6CF2.129P2-NDR2tm1/BAH-FMI). Ndr1 loss-of-function (B6.129P2-NDR1tm/BAH-FMI) mice have been described previously [7]. Mice were housed in Optimal Hygiene (Conventional) Conditions in Ventirack cages on Lignocel BK8-15 bedding with Rodent chow and water ad libitum and cage changes performed in Change Stations. Room conditions are monitored and maintained at 22+/-2°C temperature and 45–65% humidity with a 12 hour light/dark cycle. Kleenex tissue or nestlets are provided for enrichment. Mice are routinely group housed. Housing capacity is dependent upon cage type and mouse size. Mice are routinely monitored for ill-health/injury/adverse effects. Phenotypes of viable NDR GM mice have been assessed and do not require special conditions or interventions. Breeding strategy for analysis of Ndr1/2-double null (B6.129P2-NDR1tm/BAH-FMI NDR2tm1/BAH-FMI) embryonic lethality was optimized for DKO generation with single KO controls.

Sample sizes for animal experiments

Numbers of embryos analyzed and replicates performed to generate each data point are as follows: for gross morphological analysis (Fig 3), 15 litters with Ndr1/2-double null and control embryos at E8.5 as well as 56 Ndr1/2-double null and 163 control embryos at E9.5 were analyzed; for WISH (Figs 3 and 5); four animals per genotype were analyzed for Shh and T/Brachyury staining (Fig 3D and 3E), four animals per genotype were analyzed for Meox1 staining (Fig 5B), two embryos per genotype were analyzed for Tbx6 and Mesogenin staining (Fig 5C and 5D), seven embryos were analyzed per genotype for Snail1 staining (Fig 5F), five embryos were analyzed per genotype for Axin2 staining (Fig 5G), and nine Ndr1/2-double null and four control embryos were analyzed for Lnfg staining (Fig 5H); for H&E stainings of somite sections (Fig 5E) six Ndr1/2-double null and six control embryos were analyzed; for gross morphological analysis of the heart (Fig 6C and 6D) five Ndr1/2-double null and five control embryos at E9.5 were analyzed; for OPT analyses (Fig 6A, 6D and 6E) two Ndr1/2-double null and two control embryos were examined; and for H&E stainings of heart sections (Fig 6F, 6G, and 6H) three Ndr1/2-double null and three control embryos were analyzed. One representative series of analysis is shown for each Ndr1/2-double null and control embryos. Unless otherwise stated in the main text and/or figure legends, all embryos analyzed displayed the phenotypes/staining shown in the corresponding figure panels.


The wild-type and loss-of-function Ndr2 alleles were distinguished using a common forward primer: 5’gctgggataggtggataaatgg3’ and the following reverse primers: 5’gcttaagtcttaagctcaacctc3’ for wild-type yielding a PCR product of 424 bp and 5’gcctgcattgcagtccttagc3’ for the loss-of-function allele yielding a PCR product of 843 bp. Genotyping of the wild-type and loss-of-function Ndr1 alleles was done as described [7].

Antibodies and immunoblotting

The following rabbit polyclonal antibodies were used for Western blotting: total NDR1 and NDR2 [7]; phospho-T444/T442 [65]. The anti-actin antibody (sc-1616) was obtained from Santa Cruz, the HSC70 antibody (Clone 1B5) from Stressgen. Western blotting analysis was done as described previously [7].

Microarray analysis

Microarray analysis used total mRNA prepared from male mouse embryos at the 7–9 somite stage. The pooled mRNAs from three Ndr1/2-double null and control littermates were compared. RNA was processed using the WT cDNA Synthesis & Amplification kit and cDNAs labeled using the WT Terminal Labeling kit from Affymetrix (Affymetrix, Santa Clara, CA) according to manufacturer's instructions. GeneChip Mouse Gene 1.0 ST arrays were hybridized according to the "GeneChip Whole Transcript (WT) Sense Target Labeling Assay Manual" (Affymetrix, Santa Clara, CA). The Affymetrix Fluidics protocol FS450_0007 was used for washing. Scanning was done using the Affymetrix GCC Scan Control v. 3.0.1 on a GeneChip Scanner 3000 with autoloader (Affymetrix). Probe sets were summarized and probe set-level values normalized with the “justRMA” function from R (version 2.10.0); the Bioconductor (version 2.5) package using the CDF environment MoGene-1_0-st-v1.r3.cdf (as provided by Bioconductor) and annotated from Netaffx ( Differentially expressed genes were identified using the empirical Bayes method (F test) as part of the LIMMA package and adjusted with the false discovery rate method as described [66]. Hierarchical clustering and visualization was done in R. Probe sets with a log2 average contrast signal of at least 5, a P value of <0.05, and an absolute log2 fold-change of >0.263 (1.2-fold in linear space) were selected. This lead to the identification of 701 transcriptionally up-regulated and 183 down-regulated genes in Ndr1/2-double null embryos (S1 and S2 Tables).

Quantitative Real-time PCR (qRT-PCR)

qRT-PCR was performed using RNA extracted from embryos (see above). cDNA was generated from 1μg of total RNA using the M-MuLV reverse transcriptase (NEB) and random hexamer primers. Quantitative RT-PCR to detect p21, p27, Ctgf, Acta2 and Tagln expression levels was done using SYBR green in an ABI Prism 7000 detection system (Applied Biosystems). The primer sequences for amplifying Ctgf, Acta2 and Tagln were taken from ref. [43]. Primer sequences for p21 and p27 were obtained from the Harvard Primer Bank. All data shown are the average of analyzing three independent embryos per genotype. To determine the statistical significance of the observed differences in gene expression, a two-tailed T-test was performed assuming unequal variance.

Whole-mount in situ hybridization and TUNEL analysis

Whole-mount in situ hybridization was performed according to ref. [67]. The following DIG-labeled riboprobes were used to detect transcripts: Axin2 [43]; Lunatic Fringe [68]; Meox1 [69]; Mesogenin1 [32]; Snai1 [70]; Sonic hedgehog [71]; T/brachyury [72]; Tbx6 [73]. Ndr1 and Ndr2 riboprobe were generated by PCR using mouse cDNA and the primers: 5’cgatatctattgaaatcaagag3’ and 5’ttccccttcattctgatcaacttg3’ (for Ndr1; amplifying the nucleotides corresponding to 1416 to 1930 of NM_134115); and 5’ggaaagaccagcagctattcc3’ and 5’tgcagttctggctggattagtg3’ (for Ndr2; amplifying the nucleotides corresponding to 1305 to 1850 of NM_172734). TUNEL analysis was performed on paraffin sections with the ApoAlert DNA Fragmentation Assay Kit (Clontech) as defined by the manufacturer using the Venata Biobench machine.

Optical Projection Tomography

Optical Projection Tomography (OPT, [74]) was used to generate virtual optical sections of wild-type and Ndr1/2-double null embryos. Samples were fixed overnight in 4% PFA, 0.2% glutaraldehyde in PBS and washed extensively. Then they were embedded in 1% low melting point agarose (Sigma), dehydrated in methanol and cleared in benzyl alcohol-benzyl benzoate. An OPT 3001M scanner (Bioptonics, MRC Technology) was used to acquire high-resolution images (1024x1024 pixels) of the sample anatomy using the GFP1 filter (425/40nm, 475nm LP). No filter (bright field) was used to acquire whole mount in situ hybridization signals. SkyScan software was used to scan the sample and NRecon software to reconstruct the 3D topology. Virtual sections of the 3D reconstructed embryos were obtained using the DataViewer software.

Supporting Information

S1 ARRIVE Checklist. Completed “ARRIVE Guidelines Checklist” for reporting data regarding animal research in this manuscript.


S1 Fig. Ndr1 and Ndr2 transcripts are broadly expressed in mouse embryos at E8.5.

Whole mount in situ hybridization to Ndr1 (top) and Ndr2 (bottom) transcripts in wild-type embryos at E8.5. Ndr1 and Ndr2 expression was analyzed in three wild-type embryos each.


S2 Fig. Wild-type and Ndr1/2-double null embryos show low and comparable levels of apoptosis at E8.5.

Detection of apoptotic cells by the TUNEL method using FITC-labeled nucleotides in wild-type (left) and Ndr1/2-double null (right) embryo. Apoptotic cells are shown in green and DNA is stained in blue. Four wild-type and four Ndr1/2-double null embryos were analyzed.


S3 Fig. YAP targets are expressed normally in Ndr1/2-double null embryos at E8.5.

RNA was isolated from control and Ndr1/2-null embryos at E8.5 as described in Materials and Methods. Purified total RNA was used for gene expression analysis by qRT-PCR. Data shown represent the average transcript levels in three independent embryos per genotype. Each embryo was analyzed in triplicate. Statistical analysis was performed using a two-tailed T-test assuming unequal variance.


S4 Fig. Mitotic index analysis of wild-type and Ndr1/2-double null embryos at E8.5.

(A, B) At E8.5 mitotic cells in wild-type (A) and Ndr1/2-double null embryos (B) were visualized on paraffin sections with a specific anti-phospho Histone 3 antibody. Nuclei were counterstained by DAPI. (C) Quantification of the mitotic index in wild-type and Ndr1/2-double null embryos at E8.5. The mitotic index was defined as the percentage of phospho-H3 positive cells per embryo. Four embryos per genotype were analyzed with five independent sections per embryo being quantified. In total, more than 40,000 cells were analyzed per genotype. Error bars indicate the standard error of the mean (SEM).


S5 Fig. Moderate increases of cell cycle duration over a short time period can potentially cause significant growth retardation of the mouse embryo at E8.5.

Illustration of a mathematical model to approximate the effect of an increase in cell cycle duration on embryo growth at E8.5. The model is based on the simplifying assumption that all cells in the embryo divide at the same, constant rate twt from E7.5 to E8.5. This leads to an exponential equation where Xt = X0 * 2t/t. X0 is the total cell number of the embryo at t0, t is the cell cycle duration in hours and Xt the number of cells after t hours. We subsequently introduce the ratio “Q” of Xt, wild type over Xt, mutant to describe relative growth retardation as a function of the increase in t in the mutant. Q is plotted as a function of increasing cell cycle duration in the mutant after a period of 24 hours (t = 24). We observed earlier that wild-type embryos were approximately 1.5 fold bigger than Ndr1/2-double null littermates at E8.5 (Fig 3). According to our model, an increase of cell cycle duration from 6.7 hrs* to 8 hrs (intersection of dashed and solid red line) over 24 hours would suffice to generate a 1.5 fold difference at E8.5. *approximate cell cycle duration of 6.7 hrs at E7-7.5 was taken from Snow, J. Embryol. Exp. Morphol (1977) 42, 293–303.


S1 Table. List of upregulated genes in Ndr1/2-double null embryos (at E8.5).

Transcript levels were compared between control and Ndr1/2-double null embryos. Pooled transcripts obtained from three Ndr1/2-double null and three control littermate embryos were compared. Only genes whose expression is significantly altered are listed (p ≤ 0.05). A detailed description of the applied statistical analyses is provided in the Materials and Methods section.


S2 Table. List of downregulated genes in Ndr1/2-double null embryos (at E8.5).

Transcript levels were compared between control and Ndr1/2-double null embryos. Pooled transcripts obtained from three Ndr1/2-double null and three control littermate embryos were compared. Only genes whose expression is significantly altered are listed (p ≤ 0.05). A detailed description of the applied statistical analyses is provided in the Materials and Methods section.



We thank Joanna Lisztwan and Jacques Camonis for careful reading of this manuscript. We thank Jean-Francois Spetz and the team of the Transgenic Mouse Facility at the Friedrich Miescher Institute for Biomedical Research (FMI) for their assistance in generating the Ndr2 KO mouse line. The authors are grateful for discussions with all other Hemmings lab members.

Author Contributions

Conceived and designed the experiments: DS-R SP Z-ZY RZ BAH AH. Performed the experiments: DS-R SP FL DH. Analyzed the data: DS-R SP Z-ZY FL AZ RZ AH. Contributed reagents/materials/analysis tools: SP MS AZ RZ DH. Wrote the paper: DS-R RZ AH.


  1. 1. Hergovich A, Stegert MR, Schmitz D, Hemmings BA. NDR kinases regulate essential cell processes from yeast to humans. Nature reviews Molecular cell biology. 2006;7(4):253–64. Epub 2006/04/12. pmid:16607288.
  2. 2. Devroe E, Erdjument-Bromage H, Tempst P, Silver PA. Human Mob proteins regulate the NDR1 and NDR2 serine-threonine kinases. J Biol Chem. 2004;279(23):24444–51. Epub 2004/04/07. M401999200 [pii]. pmid:15067004.
  3. 3. Stegert MR, Tamaskovic R, Bichsel SJ, Hergovich A, Hemmings BA. Regulation of NDR2 protein kinase by multi-site phosphorylation and the S100B calcium-binding protein. J Biol Chem. 2004;279(22):23806–12. Epub 2004/03/24. M402472200 [pii]. pmid:15037617.
  4. 4. Stork O, Zhdanov A, Kudersky A, Yoshikawa T, Obata K, Pape HC. Neuronal functions of the novel serine/threonine kinase Ndr2. J Biol Chem. 2004;279(44):45773–81. Epub 2004/08/17. M403552200 [pii]. pmid:15308672.
  5. 5. Geng W, He B, Wang M, Adler PN. The tricornered gene, which is required for the integrity of epidermal cell extensions, encodes the Drosophila nuclear DBF2-related kinase. Genetics. 2000;156(4):1817–28. Epub 2000/12/05. pmid:11102376; PubMed Central PMCID: PMC1461384.
  6. 6. He Y, Fang X, Emoto K, Jan YN, Adler PN. The tricornered Ser/Thr protein kinase is regulated by phosphorylation and interacts with furry during Drosophila wing hair development. Mol Biol Cell. 2005;16(2):689–700. Epub 2004/12/14. doi: E04-09-0828 [pii] pmid:15591127; PubMed Central PMCID: PMC545904.
  7. 7. Cornils H, Stegert MR, Hergovich A, Hynx D, Schmitz D, Dirnhofer S, et al. Ablation of the kinase NDR1 predisposes mice to the development of T cell lymphoma. Science signaling. 2010;3(126):ra47. Epub 2010/06/17. pmid:20551432.
  8. 8. Rehberg K, Kliche S, Madencioglu DA, Thiere M, Muller B, Meineke BM, et al. The serine/threonine kinase Ndr2 controls integrin trafficking and integrin-dependent neurite growth. The Journal of neuroscience: the official journal of the Society for Neuroscience. 2014;34(15):5342–54. Epub 2014/04/11. pmid:24719112.
  9. 9. Hergovich A, Lamla S, Nigg EA, Hemmings BA. Centrosome-associated NDR kinase regulates centrosome duplication. Mol Cell. 2007;25(4):625–34. Epub 2007/02/24. doi: S1097-2765(07)00043-3 [pii] pmid:17317633.
  10. 10. Hergovich A, Kohler RS, Schmitz D, Vichalkovski A, Cornils H, Hemmings BA. The MST1 and hMOB1 tumor suppressors control human centrosome duplication by regulating NDR kinase phosphorylation. Curr Biol. 2009;19(20):1692–702. Epub 2009/10/20. doi: S0960-9822(09)01698-4 [pii] pmid:19836237.
  11. 11. Chiba S, Amagai Y, Homma Y, Fukuda M, Mizuno K. NDR2-mediated Rabin8 phosphorylation is crucial for ciliogenesis by switching binding specificity from phosphatidylserine to Sec15. The EMBO journal. 2013;32(6):874–85. Epub 2013/02/26. pmid:23435566; PubMed Central PMCID: PMC3604723.
  12. 12. Vichalkovski A, Gresko E, Cornils H, Hergovich A, Schmitz D, Hemmings BA. NDR kinase is activated by RASSF1A/MST1 in response to Fas receptor stimulation and promotes apoptosis. Current biology: CB. 2008;18(23):1889–95. Epub 2008/12/09. pmid:19062280.
  13. 13. Zhou Y, Adolfs Y, Pijnappel WW, Fuller SJ, Van der Schors RC, Li KW, et al. MICAL-1 is a negative regulator of MST-NDR kinase signaling and apoptosis. Molecular and cellular biology. 2011;31(17):3603–15. Epub 2011/07/07. pmid:21730291; PubMed Central PMCID: PMC3165550.
  14. 14. Cornils H, Kohler RS, Hergovich A, Hemmings BA. Human NDR kinases control G(1)/S cell cycle transition by directly regulating p21 stability. Molecular and cellular biology. 2011;31(7):1382–95. Epub 2011/01/26. pmid:21262772; PubMed Central PMCID: PMC3135299.
  15. 15. Chiba S, Ikeda M, Katsunuma K, Ohashi K, Mizuno K. MST2- and Furry-mediated activation of NDR1 kinase is critical for precise alignment of mitotic chromosomes. Curr Biol. 2009;19(8):675–81. Epub 2009/03/31. doi: S0960-9822(09)00807-0 [pii] pmid:19327996.
  16. 16. Oh HJ, Kim MJ, Song SJ, Kim T, Lee D, Kwon SH, et al. MST1 limits the kinase activity of aurora B to promote stable kinetochore-microtubule attachment. Current biology: CB. 2010;20(5):416–22. Epub 2010/02/23. pmid:20171103.
  17. 17. Du Z, Tong X, Ye X. Cyclin D1 promotes cell cycle progression through enhancing NDR1/2 kinase activity independent of cyclin-dependent kinase 4. The Journal of biological chemistry. 2013;288(37):26678–87. Epub 2013/07/31. pmid:23897809; PubMed Central PMCID: PMC3772214.
  18. 18. Chakraborty A, Prasanth KV, Prasanth SG. Dynamic phosphorylation of HP1alpha regulates mitotic progression in human cells. Nat Commun. 2014;5:3445. pmid:24619172; PubMed Central PMCID: PMC3982596.
  19. 19. Cornils H, Kohler RS, Hergovich A, Hemmings BA. Downstream of human NDR kinases: impacting on c-myc and p21 protein stability to control cell cycle progression. Cell Cycle. 2011;10(12):1897–904. Epub 2011/05/20. pmid:21593588.
  20. 20. Hergovich A. Regulation and functions of mammalian LATS/NDR kinases: looking beyond canonical Hippo signalling. Cell Biosci. 2013;3(1):32. Epub 2013/08/30. pmid:23985307.
  21. 21. Stemple DL. Structure and function of the notochord: an essential organ for chordate development. Development. 2005;132(11):2503–12. pmid:15890825.
  22. 22. Chiang C, Litingtung Y, Lee E, Young KE, Corden JL, Westphal H, et al. Cyclopia and defective axial patterning in mice lacking Sonic hedgehog gene function. Nature. 1996;383(6599):407–13. Epub 1996/10/03. pmid:8837770.
  23. 23. Wilkinson DG, Bhatt S, Herrmann BG. Expression pattern of the mouse T gene and its role in mesoderm formation. Nature. 1990;343(6259):657–9. Epub 1990/02/15. pmid:1689462.
  24. 24. Kaufman HL. The Atlas of Mouse Development. Revised ed. London: Academic Press; 1992 1999.
  25. 25. Zhang L, Tang F, Terracciano L, Hynx D, Kohler R, Bichet S, et al. NDR Functions as a Physiological YAP1 Kinase in the Intestinal Epithelium. Current biology: CB. 2015;25(3):296–305. Epub 2015/01/21. pmid:25601544.
  26. 26. Ota M, Sasaki H. Mammalian Tead proteins regulate cell proliferation and contact inhibition as transcriptional mediators of Hippo signaling. Development. 2008;135(24):4059–69. Epub 2008/11/14. pmid:19004856.
  27. 27. Narla G, Heath KE, Reeves HL, Li D, Giono LE, Kimmelman AC, et al. KLF6, a candidate tumor suppressor gene mutated in prostate cancer. Science. 2001;294(5551):2563–6. Epub 2001/12/26. [pii]. pmid:11752579.
  28. 28. Narla G, Kremer-Tal S, Matsumoto N, Zhao X, Yao S, Kelley K, et al. In vivo regulation of p21 by the Kruppel-like factor 6 tumor-suppressor gene in mouse liver and human hepatocellular carcinoma. Oncogene. 2007;26(30):4428–34. Epub 2007/02/14. doi: 1210223 [pii] pmid:17297474.
  29. 29. Kippin TE, Martens DJ, van der Kooy D. p21 loss compromises the relative quiescence of forebrain stem cell proliferation leading to exhaustion of their proliferation capacity. Genes Dev. 2005;19(6):756–67. pmid:15769947; PubMed Central PMCID: PMC1065728.
  30. 30. Pechnick RN, Zonis S, Wawrowsky K, Pourmorady J, Chesnokova V. p21Cip1 restricts neuronal proliferation in the subgranular zone of the dentate gyrus of the hippocampus. Proc Natl Acad Sci U S A. 2008;105(4):1358–63. pmid:18172194; PubMed Central PMCID: PMC2234143.
  31. 31. Deng C, Zhang P, Harper JW, Elledge SJ, Leder P. Mice lacking p21CIP1/WAF1 undergo normal development, but are defective in G1 checkpoint control. Cell. 1995;82(4):675–84. Epub 1995/08/25. pmid:7664346.
  32. 32. Wittler L, Shin EH, Grote P, Kispert A, Beckers A, Gossler A, et al. Expression of Msgn1 in the presomitic mesoderm is controlled by synergism of WNT signalling and Tbx6. EMBO Rep. 2007;8(8):784–9. Epub 2007/08/02. doi: 7401030 [pii] pmid:17668009; PubMed Central PMCID: PMC1978083.
  33. 33. Mankoo BS, Skuntz S, Harrigan I, Grigorieva E, Candia A, Wright CV, et al. The concerted action of Meox homeobox genes is required upstream of genetic pathways essential for the formation, patterning and differentiation of somites. Development. 2003;130(19):4655–64. Epub 2003/08/20. [pii]. pmid:12925591.
  34. 34. Watabe-Rudolph M, Schlautmann N, Papaioannou VE, Gossler A. The mouse rib-vertebrae mutation is a hypomorphic Tbx6 allele. Mech Dev. 2002;119(2):251–6. Epub 2002/12/05. doi: S0925477302003945 [pii]. pmid:12464437.
  35. 35. White PH, Farkas DR, McFadden EE, Chapman DL. Defective somite patterning in mouse embryos with reduced levels of Tbx6. Development. 2003;130(8):1681–90. Epub 2003/03/07. pmid:12620991.
  36. 36. Dequeant ML, Pourquie O. Segmental patterning of the vertebrate embryonic axis. Nat Rev Genet. 2008;9(5):370–82. Epub 2008/04/17. doi: nrg2320 [pii] pmid:18414404.
  37. 37. Satoh W, Gotoh T, Tsunematsu Y, Aizawa S, Shimono A. Sfrp1 and Sfrp2 regulate anteroposterior axis elongation and somite segmentation during mouse embryogenesis. Development. 2006;133(6):989–99. Epub 2006/02/10. doi: dev.02274 [pii] pmid:16467359.
  38. 38. Zhang N, Gridley T. Defects in somite formation in lunatic fringe-deficient mice. Nature. 1998;394(6691):374–7. Epub 1998/08/05. pmid:9690472.
  39. 39. Hrabe de Angelis M, McIntyre J 2nd, Gossler A. Maintenance of somite borders in mice requires the Delta homologue DII1. Nature. 1997;386(6626):717–21. Epub 1997/04/17. pmid:9109488.
  40. 40. Kusumi K, Sun ES, Kerrebrock AW, Bronson RT, Chi DC, Bulotsky MS, et al. The mouse pudgy mutation disrupts Delta homologue Dll3 and initiation of early somite boundaries. Nat Genet. 1998;19(3):274–8. Epub 1998/07/14. pmid:9662403.
  41. 41. Dunwoodie SL, Henrique D, Harrison SM, Beddington RS. Mouse Dll3: a novel divergent Delta gene which may complement the function of other Delta homologues during early pattern formation in the mouse embryo. Development. 1997;124(16):3065–76. Epub 1997/08/01. pmid:9272948.
  42. 42. Dale JK, Malapert P, Chal J, Vilhais-Neto G, Maroto M, Johnson T, et al. Oscillations of the snail genes in the presomitic mesoderm coordinate segmental patterning and morphogenesis in vertebrate somitogenesis. Dev Cell. 2006;10(3):355–66. Epub 2006/03/07. doi: S1534-5807(06)00075-X [pii] pmid:16516838.
  43. 43. Aulehla A, Wehrle C, Brand-Saberi B, Kemler R, Gossler A, Kanzler B, et al. Wnt3a plays a major role in the segmentation clock controlling somitogenesis. Dev Cell. 2003;4(3):395–406. Epub 2003/03/15. doi: S1534580703000558 [pii]. pmid:12636920.
  44. 44. Copp AJ. Death before birth: clues from gene knockouts and mutations. Trends Genet. 1995;11(3):87–93. Epub 1995/03/01. doi: S0168-9525(00)89008-3 [pii] pmid:7732578.
  45. 45. Harvey RP, Biben C, Elliott DA. Transcriptional control and pattern formation in the developing heart: studies on NK-2 class homeodomain factors. In: Harvey RP, Rosenthal N, editors. Heart Develoment. San Diego: Academic Press; 1999. p. 111–29.
  46. 46. Tam PP, Schoenwolf GC. Cardiac fate maps: lineage allocation, morphogenetic movement, and cell commitment In: Harvey RP, Rosenthal N, editors. Heart Development. San Diego: Academic Press; 1999. p. 3–17.
  47. 47. Lucitti JL, Jones EA, Huang C, Chen J, Fraser SE, Dickinson ME. Vascular remodeling of the mouse yolk sac requires hemodynamic force. Development. 2007;134(18):3317–26. Epub 2007/08/28. doi: 134/18/3317 [pii] pmid:17720695.
  48. 48. Harvey RP. Cardiac looping—an uneasy deal with laterality. Semin Cell Dev Biol. 1998;9(1):101–8. Epub 1998/05/08. doi: S1084-9521(97)90188-9 [pii] pmid:9572119.
  49. 49. Biben C, Harvey RP. Homeodomain factor Nkx2-5 controls left/right asymmetric expression of bHLH gene eHand during murine heart development. Genes Dev. 1997;11(11):1357–69. Epub 1997/06/01. pmid:9192865.
  50. 50. Brend T, Holley SA. Balancing segmentation and laterality during vertebrate development. Seminars in cell & developmental biology. 2009;20(4):472–8. Epub 2008/12/17. pmid:19084074.
  51. 51. Gomez C, Ozbudak EM, Wunderlich J, Baumann D, Lewis J, Pourquie O. Control of segment number in vertebrate embryos. Nature. 2008;454(7202):335–9. Epub 2008/06/20. doi: nature07020 [pii] pmid:18563087.
  52. 52. Kawakami Y, Raya A, Raya RM, Rodriguez-Esteban C, Belmonte JC. Retinoic acid signalling links left-right asymmetric patterning and bilaterally symmetric somitogenesis in the zebrafish embryo. Nature. 2005;435(7039):165–71. Epub 2005/05/13. doi: nature03512 [pii] pmid:15889082.
  53. 53. Sirbu IO, Duester G. Retinoic-acid signalling in node ectoderm and posterior neural plate directs left-right patterning of somitic mesoderm. Nat Cell Biol. 2006;8(3):271–7. Epub 2006/02/21. doi: ncb1374 [pii] pmid:16489341; PubMed Central PMCID: PMC2805411.
  54. 54. Vermot J, Gallego Llamas J, Fraulob V, Niederreither K, Chambon P, Dolle P. Retinoic acid controls the bilateral symmetry of somite formation in the mouse embryo. Science. 2005;308(5721):563–6. Epub 2005/02/26. doi: 1108363 [pii] pmid:15731404.
  55. 55. Vermot J, Pourquie O. Retinoic acid coordinates somitogenesis and left-right patterning in vertebrate embryos. Nature. 2005;435(7039):215–20. Epub 2005/05/13. doi: nature03488 [pii] pmid:15889094.
  56. 56. Harvey RP. Patterning the vertebrate heart. Nat Rev Genet. 2002;3(7):544–56. Epub 2002/07/03. nrg843 [pii]. pmid:12094232.
  57. 57. Shiratori H, Hamada H. The left-right axis in the mouse: from origin to morphology. Development. 2006;133(11):2095–104. Epub 2006/05/05. doi: dev.02384 [pii] pmid:16672339.
  58. 58. Manasek FJ, Burnside MB, Waterman RE. Myocardial cell shape change as a mechanism of embryonic heart looping. Dev Biol. 1972;29(4):349–71. Epub 1972/12/01. doi: 0012-1606(72)90077-2 [pii]. pmid:4120601.
  59. 59. Wang DZ, Reiter RS, Lin JL, Wang Q, Williams HS, Krob SL, et al. Requirement of a novel gene, Xin, in cardiac morphogenesis. Development. 1999;126(6):1281–94. Epub 1999/02/18. pmid:10021346.
  60. 60. Linask KK, Han M, Cai DH, Brauer PR, Maisastry SM. Cardiac morphogenesis: matrix metalloproteinase coordination of cellular mechanisms underlying heart tube formation and directionality of looping. Dev Dyn. 2005;233(3):739–53. Epub 2005/04/22. pmid:15844197.
  61. 61. Lu W, Seeholzer SH, Han M, Arnold AS, Serrano M, Garita B, et al. Cellular nonmuscle myosins NMHC-IIA and NMHC-IIB and vertebrate heart looping. Dev Dyn. 2008;237(12):3577–90. Epub 2008/08/13. pmid:18697221.
  62. 62. Oh S, Lee D, Kim T, Kim TS, Oh HJ, Hwang CY, et al. Crucial role for Mst1 and Mst2 kinases in early embryonic development of the mouse. Mol Cell Biol. 2009;29(23):6309–20. Epub 2009/09/30. doi: MCB.00551-09 [pii] pmid:19786569; PubMed Central PMCID: PMC2786698.
  63. 63. Song H, Mak KK, Topol L, Yun K, Hu J, Garrett L, et al. Mammalian Mst1 and Mst2 kinases play essential roles in organ size control and tumor suppression. Proc Natl Acad Sci U S A. 2010;107(4):1431–6. Epub 2010/01/19. doi: 0911409107 [pii] pmid:20080598; PubMed Central PMCID: PMC2824397.
  64. 64. Zhou D, Conrad C, Xia F, Park JS, Payer B, Yin Y, et al. Mst1 and Mst2 maintain hepatocyte quiescence and suppress hepatocellular carcinoma development through inactivation of the Yap1 oncogene. Cancer Cell. 2009;16(5):425–38. Epub 2009/11/03. doi: S1535-6108(09)00337-7 [pii] pmid:19878874.
  65. 65. Hergovich A, Bichsel SJ, Hemmings BA. Human NDR kinases are rapidly activated by MOB proteins through recruitment to the plasma membrane and phosphorylation. Mol Cell Biol. 2005;25(18):8259–72. Epub 2005/09/02. doi: 25/18/8259 [pii] pmid:16135814; PubMed Central PMCID: PMC1234321.
  66. 66. Wettenhall JM, Smyth GK. limmaGUI: a graphical user interface for linear modeling of microarray data. Bioinformatics. 2004;20(18):3705–6. Epub 2004/08/07. pmid:15297296.
  67. 67. Haramis AG, Brown JM, Zeller R. The limb deformity mutation disrupts the SHH/FGF-4 feedback loop and regulation of 5' HoxD genes during limb pattern formation. Development. 1995;121(12):4237–45. Epub 1995/12/01. pmid:8575323.
  68. 68. Evrard YA, Lun Y, Aulehla A, Gan L, Johnson RL. lunatic fringe is an essential mediator of somite segmentation and patterning. Nature. 1998;394(6691):377–81. Epub 1998/08/05. pmid:9690473.
  69. 69. Mankoo BS, Collins NS, Ashby P, Grigorieva E, Pevny LH, Candia A, et al. Mox2 is a component of the genetic hierarchy controlling limb muscle development. Nature. 1999;400(6739):69–73. Epub 1999/07/14. pmid:10403250.
  70. 70. Sefton M, Sanchez S, Nieto MA. Conserved and divergent roles for members of the Snail family of transcription factors in the chick and mouse embryo. Development. 1998;125(16):3111–21. Epub 1998/07/22. pmid:9671584.
  71. 71. Echelard Y, Epstein DJ, St-Jacques B, Shen L, Mohler J, McMahon JA, et al. Sonic hedgehog, a member of a family of putative signaling molecules, is implicated in the regulation of CNS polarity. Cell. 1993;75(7):1417–30. Epub 1993/12/31. doi: 0092-8674(93)90627-3 [pii]. pmid:7916661.
  72. 72. Herrmann BG. Expression pattern of the Brachyury gene in whole-mount TWis/TWis mutant embryos. Development. 1991;113(3):913–7. Epub 1991/11/01. pmid:1821859.
  73. 73. Chapman DL, Agulnik I, Hancock S, Silver LM, Papaioannou VE. Tbx6, a mouse T-Box gene implicated in paraxial mesoderm formation at gastrulation. Dev Biol. 1996;180(2):534–42. Epub 1996/12/15. doi: S0012-1606(96)90326-7 [pii] pmid:8954725.
  74. 74. Sharpe J, Ahlgren U, Perry P, Hill B, Ross A, Hecksher-Sorensen J, et al. Optical projection tomography as a tool for 3D microscopy and gene expression studies. Science. 2002;296(5567):541–5. Epub 2002/04/20. pmid:11964482.