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Tbx5 is a key transcription factor for vertebrate heart and forelimb development that causes Holt-Oram syndrome when mutated in humans. The classic zebrafish mutant for tbx5a named heartstrings (hst) features recessive absence of pectoral fins and a spectrum of heart defects, most-prominently featuring the name-giving stretched heart tube. The mutation of the hst allele is a stop codon that is predicted to result in a truncated Tbx5a protein that might feature residual activity. Here, using CRISPR-Cas9 mutagenesis, we generated zebrafish strains for two new tbx5a frameshift alleles in the first coding exon: tbx5a c.21_25del and tbx5a c.22_31del, abbreviated as tbx5aΔ5Δ5 and tbx5aΔ10Δ10. Homozygous and trans-heterozygous combinations of these new tbx5a alleles cause fully penetrant loss of pectoral fins and heart defects including changes in cardiac marker expression akin to hst mutants. Nonetheless, distinct from hst mutants, homozygous and trans-heterozygous combinations of these tbx5a frameshift mutants do not readily manifest the stretched hst heart phenotype. Our observation points out the importance and value of comparing phenotypes from different classes of mutant alleles per gene.
The T-box transcription factor Tbx5 is expressed in the anterior lateral plate mesoderm (ALPM) and contributes to cardiac and forelimb formation. Mutations in the human TBX5 gene cause Holt-Oram Syndrome (HOS) with concomitant heart and arm malformations that Tbx5-mutant mice recapitulate.
Zebrafish homozygous for the tbx5a allele heartstrings (hstm21m21, or short hst) and morpholino-mediated tbx5a knockdown mimic HOS phenotypes with defects in heart and pectoral fin formation. Most-prominently, hst embryos form a stretched heart tube that inspired the mutant’s name. Nonetheless, while the molecular heart and fin phenotypes are robust, the heartstrings phenotype is variable with penetrance and expressivity linked to the genetic background.
The molecular lesion in hst is an ENU-induced stop codon in the second-last coding exon; theoretically, hst mRNA can translate into a C-terminally truncated Tbx5a protein with residual or dominant-negative activity. Similarly, tbx5a morpholino knockdown causes the heartstrings phenotype with variable penetrance. Here, using CRISPR-Cas9 we generated new mutant tbx5a alleles with frameshifts in the first coding exon. Our alleles cause recessive phenotypes that recapitulate key defects of hst mutants, but do not develop the classic heartstrings phenotype. Our observation underlines the importance of allele comparisons in the design and interpretation of genome editing experiments.
Generation of new frameshift alleles for tbx5a in zebrafish with defined molecular lesions. Subsequent phenotypic analysis and comparison to previously reported tbx5a-mutant phenotypes in zebrafish.
To generate putative tbx5a null alleles in zebrafish, we employed Cas9 ribonucleoprotein complex (RNP)-mediated mutagenesis using our established sgRNA[tbx5ccAccA] that targets the first coding exon (Fig. 1A). This sgRNA targets the coding sequence in the first coding exon downstream of the conserved translation initiation codon. We targeted the first exon to introduce frameshift and subsequent stop codons early in the open reading frame to avoid potential translation of N-terminal Tbx5a protein remnants that could retain function. Further indicating that targeting this region could result in loss-of-function alleles, the corresponding amino acid sequence is highly conserved between zebrafish and humans (indicating functional conservation) and human HOS patients have been identified with frameshift-introducing nucleotide insertions at similar positions within TBX5.
Maximized mutagenesis using Cas9 RNPs with sgRNA[tbx5ccA] cause recognizable tbx5a loss-of-function phenotypes in F0 crispants. We injected the sgRNA complexed with Cas9 protein as solubilized RNPs at sub-optimal concentration to achieve viable mosaicism (see Methods for details) in the multicolor Tg(lmo2:dsRED2;drl:EGFP;myl7:mCyan) reporter background, subsequently abbreviated as RGB. In RGB embryos, dsRED2 labels endothelial, hematopoietic, and endocardial progenitors (lmo2) in red, EGFP marks all lateral plate mesoderm lineages (drl) including pectoral fins in green, and AmCyan reveals the differentiated cardiomyocytes (myl7) in blue; consequently, RGB enables in vivo imaging of all cardiovascular and additional LPM lineages over the first 3 days of development.
From F0 outcrosses that transmitted mutant tbx5a alleles, we genotyped adult F1 zebrafish for the presence of mutated tbx5a alleles by tail clipping, PCR, sequencing, and CrispRVariants analysis. From the recovered germline alleles, we kept heterozygous strains for the lesions c.21_25del and c.22_31del (hence forward abbreviated as tbx5aΔ5Δ5 and tbx5aΔ10Δ10) (Fig. 1A, B). These alleles generate out-of-frame mutations starting from base +21 or base +22, respectively, and result in premature stop codons shortly after the conserved initiation codon.
We in-crossed adult F1 heterozygotes for tbx5aΔ5Δ5 and tbx5aΔ10Δ10 and inter-crossed parents for each allele to assess F2 homozygous and trans-heterozygous embryos for developmental phenotypes at 3 dpf. We found that all combinations of the alleles resulted in Mendelian ratios of heart defects (Fig. 1E-H,U) and concomitant, completely penetrant loss of pectoral fins (Fig. 1I-L, U). The cardiac defects for the allele combinations included: cardiac edema with blood accumulation at the inflow tract region (Fig. 1F,H, white asterisks), heart mis-looping (Fig. 1G), and misshapen atrial and ventricular chambers (Fig. 1F-H, N-P, R-T), with n=49/306 for tbx5aΔ5Δ5, n=55/231 for tbx5aΔ10Δ10, n=108/417 for tbx5aΔ5/Δ10Δ5/Δ10 (Fig. 1U). Clutch values including mortality (from now on abbreviated as death rate D.R.) were: for tbx5aΔ5Δ5 clutch 1, n=29 D.R.=20.7%; clutch 2, n=144 D.R.=11.1%; clutch 3, n=133, D.R.=24.1%. For tbx5aΔ10Δ10 clutch 1, n=78 D.R.=7.7%; clutch 2, n= 65, D.R.=12.3%; clutch 3, n=88, D.R.=0%. For tbx5aΔ5/Δ10Δ5/Δ10 clutch 1, n=58, D.R.=22.4%; clutch 2, n=170, D.R.=3.5%, clutch 3, n=147, D.R.=7.5%.
While cardiac defects were fully penetrant in homozygous and trans-heterozygous mutants, the expressivity of the cardiac phenotype was highly variable, ranging from inflow tract defects (Fig. 1F) to mis-looped chambers (Fig. 1G). Live imaging using selective plane illumination microscopy (SPIM) allowed optical sectioning (Fig. 1M-P) and imaging of the whole heart (Fig. 1Q-T, side view), revealing additional details of the chamber defects. We detected atrium mis-positioning (Fig. 1N,O), freely floating and rounded-up ventricles within the pericardial cavity (Fig. 1N-P, R-T), and thinner cardiac walls (Fig. 1P) compared to wildtype or heterozygous siblings that develop a regularly formed ventricle anchored within the pericardium (Fig. 1M,Q). mRNA expression of versican a (vcana) in homozygous tbx5aΔ5Δ5 mutants was expanded in tbx5a-mutant hearts (Fig. 1V,W). All these phenotypes are well-documented for both tbx5a morphants in which tbx5a mRNA is downregulated via morpholino injection and in embryos homozygous for the classic tbx5a allele hst.
Nonetheless, in contrast to the reported morpholino and hst mutant phenotypes, we never detected the most-severe form of the hst phenotype consisting of a string-shaped heart tube and a deformed head. We readily observed this phenotype using translation-blocking tbx5a morpholino injections (n=30/106) (Fig. 1D), in line with previous reports of variable expressivity. The presence of the hst phenotype itself has previously also been linked to the genetic background, suggesting that the hst phenotype is a variation of the tbx5a loss-of-function phenotype. Taken together, homozygous and trans-heterozygous combinations of our new tbx5a frameshift alleles recapitulate morphological and molecular phenotypes of tbx5a morphants and the classic hst mutant with exception of the heartstrings phenotype. This observation suggests that either our frameshift alleles are not null and possibly hypomorphs, or alternatively that the existing hst allele and morpholino injections result in hypomorphic or dominant-negative conditions arising from truncated residual protein or lower protein concentration.
The introduction of CRISPR-Cas9 for genome editing has provided the zebrafish field with an easily accessible tool for generating mutant alleles for any gene of choice. Targeted mutagenesis using CRISPR-Cas9 requires careful assessment of targeted candidate gene loci to generate loss-of-function alleles. In contrast to classic forward genetic screens that by definition start from a mutant phenotype linked to a molecular lesion, non-homologous end joining (NHEJ)-based mutagenesis of a candidate locus can result in non-phenotypic lesions. Potential causes of the lack of phenotypes in de novo generated mutants include i) translation from downstream start codons, leading to truncated protein products with retained functions that are difficult to assess beforehand; ii) the unpredictable efficiency of nonsense-mediated mRNA decay (NMD) activated in case of premature stop codons; iii) use of alternative, cryptic splice sites to generate functional, translatable mRNA; iv) gene compensation caused by activation of alternative pathways mitigating the phenotype severity. Compensatory mechanisms in mutants have recently been reported in zebrafish for the egfl7 gene, and the role of compensation in mutant phenotype expressivity and variability in a broader context remains to be assessed.
Of note, the classic hst mutant still features detectable tbx5a mRNA, and we also detect tbx5a transcript by mRNA ISH in tbx5aΔ5Δ5- and tbx5aΔ10Δ10-mutant embryos (Fig. 1X,Y, and data not shown).The tbx5aΔ5Δ5 and tbx5aΔ10Δ10 lesions are situated in close proximity to the tbx5a translation initiation codon; while several possibly initiating ATGs are situated downstream and before the T-box, the amino acid sequence at the N-terminus where our alleles are introduced show conservation from teleosts to mammals (E.C., C.M., data not shown). In addition, frameshift mutations in similar positions within human TBX5 have been recovered from HOS patients. The full penetrance of concomitant pectoral fin loss and cardiac defects further suggest that no efficient alternative starting codon downstream of the two mutations provides a fully compensating protein product, nor that tbx5b would functionally compensate for the function of tbx5a. We do acknowledge the possibility that tbx5b could act redundant or could compensate for the heartstrings phenotype, clarification of which will require double mutants for both Tbx5-encoding genes in zebrafish.
We have generated two new frameshift alleles for tbx5a that recapitulate key phenotypes of the published hst allele and of morpholino knockdown, with exception of the heartstrings phenotype. While the frameshifts are predicted to form only short out-of-frame proteins, the alleles cannot be conclusively verified as true null alleles. Altogether, our observation underlines the value of analyzing several individual alleles of a candidate gene to assess gene function.
Due to the unavailability of a Tbx5a-specific antibody or a genetic deletion of the entire tbx5a locus, we cannot verify the absence of Tbx5a protein in our mutants or if the tbx5aΔ5Δ5 and tbx5aΔ10Δ10 lesions are bona fide null alleles. Moreover, we did not assess the possible redundant function of the tbx5a paralog tbx5b, which is suggested to have a function in pectoral fin specification and heart development.
The absence of the classical hst phenotype in our frameshift allele combinations could result from N-terminally truncated protein products from the tbx5aΔ5Δ5 and tbx5aΔ10Δ10 alleles, which hence would represent hypomorphic alleles. Such products could arise from downstream translation starting off suitable Methionine start codons after the introduced deletion. Nonetheless, the amino acid sequence between the deletions in tbx5aΔ5Δ5 and tbx5aΔ10Δ10 and the following Methionine codons is conserved across vertebrate species, hinting at functional domains.
Generation of tbx5b mutants in the tbx5aΔ5Δ5 and tbx5aΔ10Δ10 background to discriminate the possible contribution of tbx5b to the tbx5a null mutant phenotype. Further, complementation analysis with tbx5a alleles that feature bigger deletions are required to evaluate if tbx5aΔ5Δ5 and tbx5aΔ10Δ10 are null alleles or hypomorphs.
Zebrafish (Danio rerio) were maintained, collected and staged essentially as described. Embryos were raised in temperature-controlled incubators without light cycle at 28°C or as specified in the text. MO-tbx5a injection was performed as described using the translation-blocking morpholino sequence 5’-CCTGTACGATGTCTACCGTGAGGC-3’ (Gene Tools). tbx5a sgRNA design, synthesis, and injection was performed as described, using the therein published sgRNA sequence sgRNA[tbx5ccAccA] 5’-GGGAGAGTTTTGGAGCC-3’.
F1 animals were genotyped and alleles recovered as described by amplifying the locus using PCR primers forward 5’-CCACCTGAATAATGTTTGTGC-3’ and reverse 5’-CGGGGATTTGCTGACGGCTG-3’ and sequencing with primer 5’- GCAATCTGAACTAAACTGCA-3’. The F1 founders harboring the desired alleles were further crossed both into wildtype or RGB backgrounds. The F2 generation was genotyped again to establish the two strains tbx5aΔ5Δ5 and tbx5aΔ10Δ10 in wildtype and transgenic backgrounds.
The panel plot describing the tbx5a alleles was generated using the CrispRVariantsLite software (http://imlspenticton.uzh.ch:3838/CrispRVariantsLite/) from Sanger sequencing data of the alleles.
Each clutch was assessed for mortality at 24 hpf and phenotype percentages at 3 dpf were calculated on living embryos. Statistical parameters and analysis were assayed with GraphPad Prism 6, Student’s t-test was performed on at least three independent clutches for each allele combination and a p-value less than 0.0001 was considered significant. Embryos for imaging were raised in E3 with 1-phenyl 2-thiourea (PTU) 200 µM final and treated at the moment of imaging with tricaine pH= 7 3% final and 20 mM 2,3-butanedione monoxime (BDM, Sigma Aldrich) to temporarily stop heartbeat.
The triple-transgenic reporter transgenic strain RGB (Red, Green, Blue) was generated by crossing together the transgenic insertions lmo2:loxP-dsRED2-loxP-EGFP, drl:EGFP, and myl7:loxP-AmCyan-loxP-ZsYellow and propagation by repeated in- and out-crosses followed by thorough screening.
Fluorescent stereomicroscopy of RGB of wildtype, tbx5aΔ5Δ5, tbx5aΔ10Δ10, and tbx5aΔ5/Δ10Δ5/Δ10 was performed with a Leica M205 FA equipped with 1x magnification lens at 100x magnification. Samples for SPIM imaging were mounted in 0.5% low melting agarose and imaged with a 20x magnification lens plus a 10x illumination source in a Zeiss Z.1 (ZMB, UZH). Image stacks were processed with ImageJ 1.50d and Gimp2.8.
The in situ probes for versican a (vcana) and tbx5a were generated cloning-free by adding the T7 promoter sequence to the reverse primer; primers used were (T7 promoter underlined):
- vcana fw 5’- AGCTGACCCAGACATTGAGG-3’,
- vcana rev 5’-TAATACGACTCACTATAGGGTCTTGCAGGTGAAAGTGAGG-3’,AATACGACTCACTATAGGGTCTTGCAGGTGAAAGTGAGG-3’,
- tbx5a fw 5’-GGCGGACAGTGAAGACACCTT-3’,
- tbx5a rev 5’-TAATACGACTCACTATAGGGCATGATGCTGACGCTGTGCA-3’.AATACGACTCACTATAGGGCATGATGCTGACGCTGTGCA-3’.
The PCR templates were purified with a QIAquick Gel Extraction kit. The in situ probes were transcribed using T7 RNA Polymerase (Roche) and DIG RNA labeling Mix (Roche) according to manufacturer instructions. Probe quality was assessed via MOPS gel electrophoresis under denaturizing conditions. Whole-mount in situ hybridization (ISH) was performed using standard protocols with bleaching post-hybridization.
This work was supported by the Canton of Zürich and a project grant from the Swiss Heart Foundation; a Swiss National Science Foundation (SNSF) professorship (PP00P3_139093) and a Marie Curie Career Integration Grant from the European Commission (CIG PCIG14-GA-2013-631984) to C.M.; a UZH URPP “Translational Cancer Research” Seed Grant to A.B.; and a SNSF R'Equip Grant (316030_150838/1).
The authors like to thank Dr. Nadia Mercader for insightful discussions, Dr. Stephan Neuhauss and Kara Dannenhauer for assistance with zebrafish husbandry, the ZMB team at UZH for critical imaging support, and all members of the Mosimann lab for support and input.
Zebrafish for embryo production were kept in the UZH Irchel campus zebrafish facility (Tierhaltungsnummer 150). All experiments use zebrafish embryos up to 5 dpf/120 hours. Experiments with zebrafish embryos up to the age of 120 hours are not considered animal experiments by Swiss law (Art. 112 Bst. d) and the revised Directive 2010/63/EU (outlined in Strähle et al., Reprod Toxicol. 2012 Apr;33(2):128-32.), as confirmed by the animal ethics office at UZH.