www.nature.com/scientificreports OPEN Rapamycin attenuates pathological hypertrophy caused by an absence of trabecular formation Received: 1 February 2018 1,3 2,3 4 1,3 1,3 Nicole D. Fleming , Leigh A. Samsa , David Hassel , Li Qian & Jiandong Liu Accepted: 15 May 2018 Cardiac trabeculae are mesh-like muscular structures within ventricular walls. Subtle perturbations in Published: xx xx xxxx trabeculation are associated with many congenital heart diseases (CHDs), and complete failure to form trabeculae leads to embryonic lethality. Despite the severe consequence of an absence of trabecular formation, the exact function of trabeculae remains unclear. Since ErbB2 signaling plays a direct and essential role in trabecular initiation, in this study, we utilized the erbb2 zebrafish mutant as a model to address the function of trabeculae in the heart. Intriguingly, we found that the trabeculae-deficient erbb2 mutant develops a hypertrophic-like (HL) phenotype that can be suppressed by inhibition of Target of Rapamycin (TOR) signaling in a similar fashion to adult mammalian hearts subjected to mechanical overload. Further, cell transplantation experiments demonstrated that erbb2 mutant cells in an otherwise wildtype heart did not undergo hypertrophy, indicating that erbb2 mutant HL phenotypes are due to a loss of trabeculae. Together, we propose that trabeculae serve to enhance contractility and that defects in this process lead to wall-stress induced hypertrophic remodeling. e Th function of the heart is intimately linked to its structure. In order to meet an increasing physiological demand of the growing embryo, the developing vertebrate heart undergoes extensive chamber topological remodeling to increase total cardiac output. Most notably is the formation of cardiac trabeculae, the mesh-like luminal projec- 1–6 tions within ventricular myocardium . Cardiac trabeculation is a complex and tightly regulated morphogenetic process that involves cardiomyocyte (CM) apical constriction followed by CM depolarization and remodeling 7,8 of myocardial cell-cell adhesion . These highly coordinated cellular events ultimately lead to CM delamination and emergence of trabeculae . Despite substantial progress in our understanding of the cellular and molecular basis of cardiac trabeculation, the exact function of trabeculae in the heart remains unclear. Cardiac trabeculation is essential for life, as subtle perturbations in trabeculation are associated with many congenital heart diseases 2,9–11 (CHDs), and complete failure to form trabeculae leads to embryonic lethality across different species . Yet, how loss of trabeculae leads to a lethal phenotype remains an open question. Although the fundamental cellular and morphological changes associated with cardiac trabeculation occur mostly in the myocardium, this process requires crosstalk at the molecular level between endocardial and myo- 2,3,5,12–14 cardial cells . Nrg/ErbB signaling constitutes one of the most important signaling pathways required for cardiac trabeculation, and is a key node for this crosstalk. Neuregulins, expressed on endocardial cells, are part of the epidermal growth factor receptor ligand family and signal to the myocardial cells through its ErbB4-ErbB2 5,13,15,16 receptor complex and are essential for trabeculation in multiple model systems . Mouse embryos deficient of Nrg1, ErbB2 or ErbB4 all fail to form trabeculae . Likewise, loss of Nrg/ErbB2 signaling in zebras fi h embryos results in a complete absence of trabecular formation . By taking advantage of the unique attributes of zebras fi h embryos, Liu et al., demonstrated that pharmacological inhibition of ErbB2 signaling right before cardiac trabec- ulation completely blocked this process from occurring, suggesting an immediate and direct effect of Nrg/ErbB2 signaling on trabecular formation. As such, the zebras fi h erbb2 mutant is advantageous to investigate the cellular and functional consequences when the heart loses its normal internal cardiac trabecular structure. In this study, we found that erbb2 mutant ventricles exhibit an increase in ventricular cardiomyocyte cross-sectional area and myob fi ril size. This cardiac phenotype is reminiscent of hypertrophic growth of an adult Department of Pathology and Laboratory Medicine, University of North Carolina at Chapel Hill, Chapel Hill, NC, 27519, USA. Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, NC, 27519, 3 4 USA. McAllister Heart Institute, University of North Carolina at Chapel Hill, Chapel Hill, NC, 27519, USA. Department of Internal Medicine III-Cardiology, Im Neuenheimer Feld 350, University of Heidelberg, Heidelberg, 69120, Germany. Correspondence and requests for materials should be addressed to J.L. (email: firstname.lastname@example.org) SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 1 www.nature.com/scientificreports/ mammalian heart subjected to mechanical overload. Consistently, we found that the expression of hypertrophic marker gene, nppa, was elevated in erbb2 mutants compared to controls. Intriguingly, inhibition of Target of Rapamycin (TOR) signaling by rapamycin suppressed erbb2 mutant hypertrophic-like (HL) growth phenotypes and rescued cardiac function. Additionally, cell transplantation experiments indicate the erbb2 mutant HL phe- notypes are due to a loss of cardiac trabeculae. Together, our findings suggest that trabeculae serve to enhance contractility for efficient cardiac function and that defects in this process lead to wall-stress induced pathological hypertrophic remodeling. Results erbb2 mutant hearts exhibit hypertrophic-like phenotypes. While the embryonic heart requires car- 17,18 diac contraction to initiate trabecular formation , failure of cardiac trabeculation could cause the developing heart to suffer not only structural defects, but also mechanical disturbance that might lead to further myocardial st61 damages. We have previously reported that larvae homozygous for the erbb2 allele encoding a premature stop −/− codon, from here on referred to as erbb2 or erbb2 mutants, develop progressive systolic and diastolic dysfunc- 2 2 tion . The reduction in fractional shortening in erbb2 mutant hearts observed in Liu et al. is a probable conse- quence of the loss of trabeculation, suggesting that cardiac trabeculae are important for proper cardiac function and overall workload efficacy of the ventricle. To evaluate the underlying cardiomyocyte defects associated with st61 the cardiac dysfunction observed in erbb2 mutant hearts, we bred the erbb2 allele onto Tg(myl7:mKateCAAX) and Tg(myl7:Cypher-EGFP) transgenic backgrounds to label the CM plasma membrane and Z-band of cardiac sarcomere, respectively (Fig. 1A). −/− Using these genetically encoded fluorescent protein labels, we assessed cardiomyocyte structure in erbb2 larvae by confocal microscopy compared to control larvae carrying at least one copy of the wildtype erbb2 allele. This technique allowed us to measure the outer compact myocardial wall thickness, distance between sarcom- eres, and Z-line length at the trabeculation stages (Fig. 1A). When comparing outer compact myocardial wall, we observed a significant, albeit rather mild, increase in the myocardial wall thickness in erbb2 mutant ventri - cles compared to control ventricles at 3 days post fertilization (dpf ), when trabeculae are small in the ventricle (Supplementary Fig. S1A-1B’). At 5 and 7 dpf, when the control heart becomes extensively trabeculated, the dif- ference in the outer compact myocardial wall thickness between the two genotypes was even greater. For instance, at 5 and 7 dpf, the outer compact myocardial wall thickness increased by 75% and 88% in erbb2 mutant ventricles relative to control ventricles, respectively (Fig. 1B-C’,F; Supplementary Fig. S1E-F’). In contrast, it only increased by 23% at 3 dpf (Fig. 1F). Since the zebras fi h ventricular compact myocardial wall is one-cell thick , the compact myocardial wall thickness is equivalent to compact CM cross-sectional area. We also measured Z-band size as an indicator of ventricular sarcomere thickness. Cardiac remodeling in response to mechanical overload also includes the addition of sarcomeres in parallel to existing sarcomeres . Consistent with the compact wall thick- ness phenotype, Z-band length increased in the erbb2 mutant hearts by 5 dpf. Though comparable at 3 dpf, with control hearts, ventricular sarcomere thickness of erbb2 mutant hearts became significantly increased on 5 dpf and 7 dpf by 26.2% and 27.6%, respectively (Fig. 1D-E”’,G; Supplementary Fig. S1C-D” and 1G-H”). Suggesting that sarcomeric function is normal, and that the sarcomeres are structurally intact, the distance between Z-bands was unchanged in erbb2 mutants (Fig. 1H). Taken together, these data suggest that erbb2 mutant ventricles that lack trabeculae exhibited an increase in ventricular CM cross-sectional area and myofibril size, a phenotype indicative of the cellular changes that underlie biomechanical overload-induced cardiac hypertrophy . Next, we addressed whether the HL phenotypes exhibited by erbb2 mutant were pathological. At the molec- ular level, pathological cardiac hypertrophy is typically associated with upregulation of marker genes, such as 22–24 natriuretic peptide precursor A (nppa) . nppa is conserved in zebrafish and its embryonic expression has been well characterized . During cardiac development, as cardiac trabeculae start to form, nppa expression is down-regulated in the ventricular compact myocardium, and becomes restricted in cardiac trabeculae . To eval- uate whether nppa was upregulated in erbb2 mutants, we first selected putative erbb2 mutants based on a super- numerary neuromast phenotype detectable by 3 dpf with vital dye MitoTracker. nppa expression was observed in erbb2 control hearts (Supplementary Fig. S1I-I’). Interestingly, though erbb2 mutant ventricles are completely devoid of cardiac trabeculae, whole mount in situ hybridization revealed robust nppa expression in the ventricu- lar compact myocardium (Supplementary Fig. S1J-J’). More importantly, RT-PCR analysis of isolated control and mutant hearts demonstrated that the expression of nppa was dramatically upregulated in erbb2 mutants com- pared to controls (Fig. 1I), suggesting a pathological nature of erbb2 mutant hypertrophic phenotypes. Inhibition of TOR signaling attenuates erbb2 mutant hypertrophic-like phenotype. To identify signaling pathways essential for erbb2 mutants to develop HL phenotypes, we performed a targeted small mol- 20,27–30 ecule screen to inhibit signaling pathways known to be involved in regulating cardiac hypertrophy . We treated control and erbb2 mutant larvae carrying plasma membrane and sarcomere reporters with 1% DMSO or small molecules at 2.5 dpf, just prior to emergence of the first trabeculae, then assessed ventricular compact wall thickness and cardiac sarcomere structure at 5 and 7 dpf (Fig. 2A). Inhibition of TOR signaling with rapamycin at a concentration of 1 µM suppressed the increased compact myocardial wall thickness and Z-band length pheno- types in erbb2 mutant at both 5 dpf (Fig. 2B-I’ and R-S) and 7 dpf (Fig. 2J-Q’ and R-S). Narrowing in on the TOR pathway, we observed similar changes to compact myocardial wall thickness and myob fi ril length when TOR was inhibited via 0.5 µ M Rapamycin (Supplementary Fig. S2A–C) or 0.5 µ M Torin 1 (Supplementary Fig. S2D–F), another potent inhibitor of the TOR pathway. Notably, rapamycin treatment did not cause any compact myo- cardium and sarcomere defects in control hearts, nor did it have any effect on distance between Z-lines in the mutant hearts (Fig. 2T). Together, our data strongly indicates inhibition of TOR signaling by rapamycin treatment suppressed erbb2 mutant HL phenotypes. Thus, erbb2 mutant hearts develop hypertrophy in a TOR-dependent manner. SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 2 www.nature.com/scientificreports/ Figure 1. erbb2 mutant develops HL phenotypes (A) Schematic of method utilized for obtaining compact −/− myocardial wall and myob fi ril measurements. (B,C) Mid-chamber confocal sections of control and erbb2 hearts, respectively. (B’,C’) Magnified high-resolution images of compact myocardial wall and trabecular regions marked by dotted box in B, C. Yellow arrows point to length of CM along compact myocardial wall. White arrows point to trabeculae. (D,E) Maximal projection of confocal Z-stacks of ventricle. (D’-D”’, E’-E”’) Magnified high-resolution images of compact myocardium outlined in white in D and E revealing sarcomere −/− structures of two CMs in control and erbb2 ventricles, respectively. (F–H) Quantification of compact myocardial wall thickness (n = 6–10), Z-line length (n = 9–10), and distance between Z-lines (n = 8–10), at 3, 5, −/− and 7 dpf from control and erbb2 hearts. (I) Expression of nppa in whole hearts isolated from erbb2 control −/− or erbb2 larvae (n = 10–15). Data are represented as mean ± SEM. *p ≤ 0.05, **p = 0.0025, ***p = 0.0004 and ****p < 0.0001 by Student’s t test. v, ventricle; a, atrium. Rapamycin treatment improves impaired heart function in erbb2 mutant. e a Th bove experiments −/− indicate that inhibition of TOR signaling by rapamycin suppressed HL phenotypes in erbb2 larvae hearts. We next wanted to test if this attenuation of HL phenotypes translated into an enhancement or even further deteri- oration of cardiac function (Fig. 3A). Consistent with previous studies , we found that erbb2 mutants exhibited progressive cardiac dysfunction. At 3 dpf, the ventricular fractional shortening (FS) of erbb2 mutants is com- parable to that of control animals, but the mutant displayed significantly reduced FS at 5 dpf, which declined even further at 7 dpf (Fig. 3B). Consequently, erbb2 mutant animals started to die at 7 dpf (Fig. 3C). However, no significant difference on heart rate was observed between control and erbb2 mutants (Fig. 3D). Interestingly, upon treatment with rapamycin from 2.5 dpf onwards, the erbb2 mutant hearts displayed significantly improved ventricular FS at 5 dpf compared to DMSO-treated erbb2 mutant hearts (p = 0.0499). Though, this improvement in heart function is not sustainable over time (Fig. 3E). Furthermore, we did not notice any significant difference in heart rate between DMSO and rapamycin-treated groups (Fig. 3F). Together, these findings suggest that the TOR pathway is an important regulator of the HL phenotype and inhibition of TOR signaling delayed disease progression of the erbb2 mutant hearts. SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 3 www.nature.com/scientificreports/ Figure 2. Inhibition of TOR signaling attenuates erbb2 mutant HL phenotypes (A) Schematic of experimental −/− design. (B,D,F,H,J,L,N,P) Mid-chamber confocal sections of control and erbb2 hearts treated with DMSO or rapamycin at 5 and 7 dpf. (B’,D’,F’,H’,J’,L’,N’,P’) Magnified high-resolution images of compact myocardial wall and trabecular regions marked by dotted box in (B,D,F,H,J,L,N,P). Yellow arrows point to length of CM along compact myocardial wall. White arrows point to trabeculae. (C-C’,E-E’,G-G’,I-I’) Magnified high-resolution images of compact myocardium revealing sarcomere structures of CMs at 5 dpf. (K-K’,M-M’,O-O’,Q-Q’) Magnified high-resolution images of compact myocardium revealing sarcomere structures of CMs at 7 dpf. (R–T) Quantification of compact myocardial wall thickness (n = 7–15), Z-line length (n = 5–10), and distance −/− between Z-lines (n = 5–12) at 5 and 7 dpf from DMSO or rapamycin-treated control and erbb2 hearts. Data are represented as mean ± SEM. **p = 0.0035, ***p = 0.0003, and ****p < 0.0001 by Student’s t test. erbb2 mutant HL phenotype results from the absence of trabecular formation. As the erbb2 mutant HL phenotypes are reminiscent of hypertrophic growth of an adult heart subjected to mechanical over- load , we hypothesize that these HL phenotypes could be due to mechanical disturbance as a result of the absence SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 4 www.nature.com/scientificreports/ Figure 3. Rapamycin treatment improves impaired heart function in erbb2 mutant (A) Schematic of −/− experimental design. (B) Quantification of ventricular fractional shortening of control and erbb2 larvae at 3, −/− 5, and 7 dpf (n = 10). (C) Quantification of percent survival over ~2 weeks of control and erbb2 clutchmates from N = 3 tanks of 50 embryos each. (D) Quantification of heart rate in beats per minute of control and −/− erbb2 larvae at 3, 5, and 7 dpf (n = 9–10). (E) Quantification of ventricular fractional shortening of DMSO −/− or rapamycin-treated control and erbb2 larvae at 3, 5, and 7 dpf (n = 9–16). (F) Quantification of heart rate −/− in beats per minute of DMSO or rapamycin-treated control and erbb2 larvae at 3, 5, and 7 dpf (n = 4–11). Data are represented as mean ± SEM. *p = 0.0499, ***p ≤ 0.001, and ****p < 0.0001 by Student’s t test. Note: −/− Asterisk in E indicates a significant difference from 5 dpf rapamycin–treated erbb2 . No significant differences were observed between groups on 3 or 7 dpf. of trabecular formation. Yet, it is also possible that the HL phenotypes could result from a loss of erbb2 func- tion cell-autonomously in the cardiomyocytes. To distinguish these possibilities, we generated genetic mosaic embryos whereby erbb2 mutant or control cells were transplanted into wildtype embryos. The host embryos were allowed to develop until 5 dpf before monitoring CM cross-sectional area and myofibril size of the trans- −/− planted cells. In these experiments, we transplanted blastomeres from erbb2 or control donors that carried Tg(myl7:mKateCAAX), Tg(myl7:Cypher-EGFP) transgenes into Tg(myl7:rasGFP); Tg(myl7:Cypher-EGFP) hosts. Transplanted donor cardiomyocytes were labeled in red by Tg(myl7:mKateCAAX), and thus, were readily dis- tinguishable from the host derived cells (Fig. 4A). Noteworthy, the transplanted mKateCAAX-positive control cells populated both the compact and trabecular layers (Fig. 4B-B”’). The mKateCAAX-positive erbb2 mutant cells failed to contribute to the trabeculae and were found exclusively in the compact layer (Fig. 4E-E”’). Most importantly, we found that the cross-sectional area of the transplanted erbb2 mutant cardiomyocytes was not significantly die ff rent from that of the transplanted control cardiomyocytes (Fig. 4B-B”’,E-E”’ and H) and their neighboring compact cardiomyocytes (Fig. 4I-J). Similarly, there was no significant difference in Z-line length (Fig. 4C-D,F-G and K) or the distance between Z-lines (Fig. 4L) between transplanted control and erbb2 mutant cardiomyocytes. u Th s, these data suggest that ErbB2 does not directly regulate compact ventricular myocardial wall thickness, and that erbb2 mutant HL phenotype is caused by the absence of trabecular formation. Discussion In this study, we sought to investigate the molecular mechanisms that impact the remodeling process when the heart loses its normal internal cardiac trabecular structure. We present in vivo evidence that cardiac trabeculae have an important physiological function during embryonic heart development. Interestingly, we found erbb2 mutant ventricles exhibit an increase in ventricular CM cross-sectional area and myofibril size, likely due to an absence of trabecular formation (Fig. 5), suggesting that trabeculae-deficient ventricles undergo hypertrophy to stabilize the workload/cardiac output imbalance in the heart. It has been speculated that cardiac trabeculae serve to increase cardiac output and facilitate the exchange of 1,2,5,6 oxygen and nutrients prior to formation of the coronary vasculature . Nevertheless, there have been very few studies that examine exactly how trabeculae help the heart function in an efficient manner. Mice lacking Nrg1 , ErbB4, or ErbB2 fail to form trabeculae and thus die at approximately E10.5 . The early embryonic lethality of these systems disallows for detailed characterization of the trabeculae-deficient hearts at a cellular level. Zebras fi h SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 5 www.nature.com/scientificreports/ Figure 4. erbb2 mutant HL phenotypes result from the absence of trabecular formation (A) Schematic of transplantation experiment resulting in transplanted blastomeres from Tg(myl7:mKateCAAX);Tg(myl7:Cyp −/− her-EGFP) erbb2 control or erbb2 donors into Tg(myl7:rasGFP); Tg(myl7:Cypher-EGFP) wild-type hosts. −/− (B-B”,E-E”) Mid-chamber confocal sections of control and erbb2 donor CMs, respectively, in wild-type host ventricle. (B”’,E”’) Magnified high-resolution images of compact myocardial wall and trabecular regions marked by dotted box in B”, E”. Yellow arrows point to length of donor CM (yellow line) along compact myocardial wall. White arrow heads point to length of host CM (white line) along compact myocardial wall. White arrows point to trabeculae. (C,F) Maximal projection of confocal Z-stacks of ventricle. (D,G) Magnified high-resolution images −/− of compact myocardium, revealing sarcomere structures of control and erbb2 donor CMs, respectively, in wild- −/− type host ventricle at 5 dpf. (H–J) Quantification of cross-sectional area of erbb2 control donor and erbb2 donor −/− CMs (H), erbb2 control donor and host CMs (I), and erbb2 donor and host CMs at 5 dpf (J). (K) Quantification −/− of Z-line length of erbb2 control donor and erbb2 donor CMs at 5 dpf. (L) Quantification of distance between −/− Z-lines of erbb2 control donor and erbb2 donor CMs at 5 dpf. Data are represented as mean ± SEM. SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 6 www.nature.com/scientificreports/ Figure 5. Schematic diagram illustrating that trabeculae-deficient erbb2 mutants undergo TOR-dependent pathological hypertrophy. embryos do not require a functional circulatory system during the first week of life and thus can survive very 31,32 severe cardiac defects . Thus, we took advantage of the zebras fi h erbb2 mutant that lacks trabeculae to decipher the consequence of an absence of trabecular formation and found that trabeculae-deficient hearts exhibited HL phenotypes reminiscent of those of an adult mammalian heart subjected to mechanical overload. As an organism grows, the heart undergoes morphological changes to meet the demand of increase workload. Our findings thus suggest that trabeculae serve to enhance contractility and that defects in this process lead to wall-stress induced pathological hypertrophic remodeling. Pathological cardiac hypertrophy is induced by mechanical pressure-overload . The intracellular signaling activated by the mechanical stress imposed on the myocardium induces extensive structural and physiological changes to offset the mechanical stress. Currently, there are no viable methods to directly measure the intra- ventricular radial wall stress “felt” by cardiomyocytes. To circumvent this gap of knowledge, future studies are needed to focus on using 3D computational models of the function in the zebras fi h heart to extract quantitative assessments of radial wall stress. Specifically, numerical simulations can be used to compare radial wall stresses generated during contraction of the control and erbb2 mutant hearts to readily obtain spatial and temporal dis- tributions of radial wall stresses. Recent studies have identified multiple cell signaling pathways to be involved in cardiac hypertrophy, includ- 20,27–30 ing TOR . Signaling through the TOR pathway has been shown to be an important regulator of normal 21,27 cardiac growth and pathological hypertrophy . We examined signaling pathways that could attenuate the hypertrophic response in erbb2 mutant hearts. Our small-molecule pharmacological studies indicated that inhi- bition of TOR signaling suppressed erbb2 mutant HL growth phenotype (Fig. 5). The TOR pathway has been implicated as a potential therapeutic target for cardiomyopathies because inhibition by rapamycin, a specific 33,34 inhibitor of TORC1, has been shown to be cardio-protective . In human patients, rapamycin treatment fol- lowing heart transplantation significantly reduced left ventricular hypertrophy . Intriguingly, in mice, pharma- cological administration of rapamycin prevents cardiac hypertrophy induced by transverse aortic constriction and reverses hypertrophic cardiomyopathy in a model of CHD LEOPARD syndrome . These findings suggest a common pathological signaling pathway of CHD-associated hypertrophic cardiomyopathy across zebrafish, mouse and humans. In this present study, we also provide evidence suggesting that erbb2 mutant hearts undergo pathological hypertrophy probably due to mechanical overload because they lack trabeculae rather than to deficiency in ErbB2 signaling. Our study cannot completely rule out the possibility that HL phenotypes are manifested as a SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 7 www.nature.com/scientificreports/ consequence of ErbB2 deficiency and are independent of the absent of trabecular formation. In fact, previous studies have shown that various trabeculation-deficient zebrafish embryos that have impaired flow and cardiac 3,7,17,36 contractions display distinct differences in CM behavior and formation of protrusions . Because of the trans- parency of the zebras fi h embryos and the ease of genetic manipulation, the unique HL phenotype caused by the absence of trabeculae in ErbB2-deficient larvae will provide us a great opportunity to use zebras fi h as a model to assess molecular events and mechano-transduction signaling pathways involved in CHD-associated hypertrophic cardiomyopathy. In addition, the small size and permeability of zebras fi h embryos also enable high-throughput small molecule screens to identify novel suppressors of disease phenotypes. The zebrafish erbb2 mutant thus could serve as an in vivo platform for phenotype-based drug screen to identify novel small molecules capable of suppressing CHD-associated hypertrophic cardiomyopathy. Materials and Methods Zebrafish husbandry and strains. All animals were maintained at the aquaculture facility of the University of North Carolina at Chapel Hill in accordance with Institutional Animal Care and Use Committee approved 37 st61 38 sd11 39 protocols . We used the following transgenic and mutant lines: erbb2 mutants, Tg(myl7:mKateCAAX) , xu061 40 s883 19 Tg(myl7:Cypher-EGFP) , Tg(myl7:ras-GFP) . Confocal imaging and analysis. Zebrafish embryos were anesthetized using 1X Tricaine (Sigma) and mounted with 1% low-melting agarose (Sigma) in embryo medium or system water for optimal visualization of the heart. Heartbeat was ceased before imaging using 5–10X Tricaine (Sigma). Images were obtained with an Olympus Fluoview 1000MPE, multiphoton, upright confocal microscope equipped with a 20X XLPlan (NA 1.0) water immersion objective with 3.0X, 2.5X, or 10X digital zoom and 1024 × 1024 pixels resolution. Confocal z-stacks were collected using the Fluoview software with a 2.50 µ m or 1.05 µ m step size acquisition through the heart tissue. 488 nm and 599 nm lasers were used to excite GFP and RFP. Each channel was acquired sequentially to avoid bleed through and signal attenuation due to increasing depth was taken into account by using the soft- ware’s brightness correction algorithm. Confocal images were collected for a minimum of 5 embryos for each condition. Data was analyzed using ImageJ software. Compact myocardial wall and sarcomere measurements. ImageJ software was used to analyze confocal z-stacks of heart tissue. For ventricular compact myocardial length, a line (total of 12 lines) was drawn from one end of the plasma membrane to the next of individual cardiomyocytes through different mid-chamber z-stacks to obtain an average measurement from a minimum of 5 embryos. An average measurement of distance between sarcomeres was obtained by drawing a line (N = 20) from the middle of one Z-line to the middle of the neighboring Z-line for a minimum of 5 embryos. To obtain sarcomere Z-line length, Z-lines of individual cardio- myocytes were outlined and average length of Z-lines and area of cardiomyocytes were recorded for a minimum of 5 cardiomyocytes. Cardiac function measurements. Embryos were genotyped using MitoTracker Red (Life Technologies) and immobilized with 0.5X Tricaine (Sigma). Embryos were mounted using 1% low-melting agarose (Sigma) and oriented for optimal observation of hearts at 3, 5, and 7 dpf. After agarose solidified, embryos were incu- bated with fresh egg water for 20 minutes to remove any residual Tricaine and renew normal cardiac contrac- tion. A Leica M205C fluorescence stereomicroscope and software were used to visual and record live imaging of Tg(myl7:mKateCAAX); Tg(myl7:Cypher-EGFP) positive hearts at 120X or 200X magnification. For each condition, heartbeats per minute were obtained from 15-second movies. Additional details are as previously 39 2 described . Assessment of fractional shortening was performed as previously described . Briefly, for each embryo, the average diameter at end systole (fully contracted ventricle) and end diastole (fully dilated ventricle), during three cardiac cycles, was obtained using VirtualDub software (available at http://www.virtualdub.org ) and ImageJ . +/− Survival curve. Zebras fi h embryos from interbreeding erbb2 Tg(myl7:mKateCAAX); Tg(myl7:Cypher-EGFP) fish were screened at 3 dpf using MitoTracker Red to identify erbb2 control and mutant embryos. Survival was recorded daily from N = 3 tanks of 50 embryos each per genotype. Chemical inhibition of hypertrophic pathways. Pharmacological inhibitors were stored in DMSO (Fisher Scientific) stocks. Embryos were treated with drugs, 0.5 µ M or 1 µ M rapamycin (Santa Cruz Biotech) or 0.5 µ M Torin 1 (Cayman Chemical), diluted in egg water (1.5 mL stock salts added to 1 L distilled water) and supplemented with 0.003% 1-phenyl 2-thiourea (PTU) (Sigma) and DMSO to 1% final. Control embryos were incubated with 1% DMSO vehicle. Embryos were dechorionated and treated with DMSO, rapamycin or Torin 1 at 2.5 dpf until 5 dpf and 7dpf. Whole heart isolations and quantitative RT-PCR. At 3, 5, and 7 dpf, zebrafish embryos were eutha- nized and hearts were isolated with forceps using a Leica M205C fluorescence stereomicroscope and placed in lysis buffer prior to RNA isolation. At least 10 hearts were pooled per sample and RNA was extracted using a RNeasy Plus Mini kit (Qiagen). cDNA synthesis was performed immediately following RNA isolation protocol using iScript cDNA synthesis kit (Invitrogen). Quantitative RT-PCR was performed using cDNA, Sybr Green reagent (Roche) and gene-specific primers in triplicates using an Applied Biosystem Viia7 RT-PCR machine (Life Technologies). The primer sequences used in this study are provided in Supplementary Table S1. The delta-delta CT method was used to normalize desired genes to the endogenous housekeeping gene vmhc and determine the relative fold change gene expression. SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 8 www.nature.com/scientificreports/ 42,43 Whole-mount in situ hybridization. In situ hybridization was performed as previously described . Briefly, genotyped zebras fi h embryos were fixed with 4% paraformaldehyde in 1X PBS at 5 dpf and placed in 4 °C cold room overnight. Embryos were then washed in 1X PBS (3 × 10 minutes), incubated for 30 minutes in 100% methanol then stored in 100% methanol at −20 °C. Zebras fi h embryos were rehydrated in PBST and incubated in proteinase K (20 mg/ml diluted in PBT 2:2000) for 45 minutes then post-fixed in 4% PFA. The tail of erbb2 mutant embryos were removed using fine forceps, and both control and mutant embryos were placed in the same tube to ensure consistent handling throughout the staining process. Hybridization with probe of interest was done over- night in a 65–70 °C water bath. Following washes, embryos were incubated with anti-DIF-AP antibody (Roche) overnight at 4 °C. Subsequent color development was achieved following addition of NBT/BCIP. Embryos were then stored in stop solution at 4 °C overnight. Next, embryos were transferred to 100% glycerol and placed at 4 °C overnight. Embryos were mounted in 100% glycerol for imaging. Whole-mount embryos were visualized using a Leica MZ16F fluorescence stereomicroscope with Retiga 2000R camera and images were collected using the QCapture software. Cell Transplantation. Mosaic embryos were obtained using erbb2 control or mutant Tg(myl7:mKateCAAX); Tg(myl7:Cypher-EGFP) and Tg(myl7:ras-GFP);Tg(myl7:Cypher-EGFP) double transgenic lines. Cells were removed from donor embryos and transplanted into the marginal zone of stage-matched host embryos. Embryos were visualized using a Leica S6D microscope. Cells were transplanted using borosilicate thin wall capillary glass tubing needles (Warner Instruments) and a CellTram vario (Eppendorf ) apparatus that allowed for precise con- trol of pressure transmission with oil. Host embryos with mKateCAAX-expressing cells were allowed to develop st61 until 5 dpf. Donor embryos from in-crossing erbb2 heterozygotes were kept to determine genotype of donor 38 17 cells as previously described . Embryos were mounted for imaging, as previously described , for observing com- pact myocardial wall and sarcomere measurements. Statistical Analysis. e d Th ata shown in the graphs are represented as mean ± SEM. Statistical significance was determined between groups with a two-tailed Student’s t-test. References 1. Sedmera, D., Pexieder, T., Vuillemin, M., Thompson, R. P. & Anderson, R. H. Developmental patterning of the myocardium. Anat. Rec. 258, 319–337 (2000). 2. Liu, J. et al. A dual role for erbb2 signaling in cardiac trabeculation. Dev. 137, 3867–3875 (2010). 3. Peshkovsky, C., Totong, R. & Yelon, D. Dependence of cardiac trabeculation on neuregulin signaling and blood flow in zebrafish. Dev. Dyn. 240, 446–456 (2011). 4. Staudt, D. & Stainier, D. Uncovering the molecular and cellular mechanisms of heart development using the zebrafish. Annu. Rev. 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S. & Eliceiri, K. W. NIH Image to ImageJ: 25 years of image analysis. Nat. Methods. 9, 671–675 (2012). 42. Thisse, C. & Thisse, B. High-resolution in situ hybridization to whole-mount zebras fi h embryos. Nat. Protoc. 3, 59–69 (2008). 43. Liu, J. & Stainier, D. Y. Tbx5 and Bmp signaling are essential for proepicardium specification in zebras fi h. Circ. Res. 106, 1818–1828 (2010). Acknowledgements We thank Drs. Yelon, Xu and Stainier for fish stocks. We are grateful for the expert technical assistance from the UNC Microscopy Core, and the UNC ZAC facility for animal care. We thank members of the Liu lab and the Qian lab for helpful discussions and critical reviews of the manuscript. N.D.F. was supported by National Science Foundation Graduate Research Fellowship NSF-DGE-1144081, and is currently supported by American Heart Association (AHA) Pre-doctoral Fellowship 17PRE33660515 and The Children’s Heart Foundation (CHF) Congenital Heart Defect Research Award. This study was supported by AHA Scientist Development Grant 13SDG17060010, the Ellison Medical Foundation (EMF) New Scholar Grant AG-NS-1064-13, and NIH/NHLBI R01HL128331 to L.Q., NIH/NHLBI R00HL109079, R56HL133081 and AHA Grant-in-Aid 15GRNT25530005 to J.L. Author Contributions N.D.F. designed and performed the majority of the experiments, analyzed the data and wrote the manuscript. L.A.S. assisted in the experimental design and provided intellectual input. N.D.F. and D.H. analyzed fractional shortening data. D.H., L.Q., and J.L. provided intellectual input and supervised the work. All authors provided feedback on the manuscript. Additional Information Supplementary information accompanies this paper at https://doi.org/10.1038/s41598-018-26843-1. Competing Interests: The authors declare no competing interests. Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations. Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Cre- ative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not per- mitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/. © The Author(s) 2018 SCientifiC RepO R TS | (2018) 8:8584 | DOI:10.1038/s41598-018-26843-1 10
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