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The AP-1 Transcription Factor c-Jun Prevents Stress-Imposed Maladaptive Remodeling of the Heart

  • Renata Windak,

    Affiliation Institute of Cell Biology, Eidgenössische Technische Hochschule Zurich (ETHZ), Zurich, Switzerland

  • Julius Müller,

    Affiliation Institute of Cell Biology, Eidgenössische Technische Hochschule Zurich (ETHZ), Zurich, Switzerland

  • Allison Felley,

    Affiliation Experimental Cardiology Unit, Department of Medicine, University of Lausanne Medical School, Lausanne, Switzerland

  • Alexander Akhmedov,

    Affiliation Cardiovascular Research, Institute of Physiology, University of Zurich, Zurich, Switzerland

  • Erwin F. Wagner,

    Affiliation Genes, Development and Disease Group, F-BBVA Cancer Cell Biology Programme, Spanish National Cancer Research Centre (CNIO), Madrid, Spain

  • Thierry Pedrazzini,

    Affiliation Experimental Cardiology Unit, Department of Medicine, University of Lausanne Medical School, Lausanne, Switzerland

  • Grzegorz Sumara , (RR); (GS)

    Affiliations Institute of Cell Biology, Eidgenössische Technische Hochschule Zurich (ETHZ), Zurich, Switzerland, Institut de Génétique et de Biologie Moléculaire et Cellulaire (IGBMC), Institut National de la Santé et de la Recherche Médicale, Centre National de la Recherche Scientifique, Université de Strasbourg, Illkirch, France

  • Romeo Ricci (RR); (GS)

    Affiliations Institute of Cell Biology, Eidgenössische Technische Hochschule Zurich (ETHZ), Zurich, Switzerland, Institut de Génétique et de Biologie Moléculaire et Cellulaire (IGBMC), Institut National de la Santé et de la Recherche Médicale, Centre National de la Recherche Scientifique, Université de Strasbourg, Illkirch, France, Laboratoire de Biochimie et de Biologie Moléculaire, Nouvel Hôpital Civil, Hôpitaux Universitaires de Strasbourg, Université de Strasbourg, Strasbourg, France


Systemic hypertension increases cardiac workload and subsequently induces signaling networks in heart that underlie myocyte growth (hypertrophic response) through expansion of sarcomeres with the aim to increase contractility. However, conditions of increased workload can induce both adaptive and maladaptive growth of heart muscle. Previous studies implicate two members of the AP-1 transcription factor family, junD and fra-1, in regulation of heart growth during hypertrophic response. In this study, we investigate the function of the AP-1 transcription factors, c-jun and c-fos, in heart growth. Using pressure overload-induced cardiac hypertrophy in mice and targeted deletion of Jun or Fos in cardiomyocytes, we show that c-jun is required for adaptive cardiac hypertrophy, while c-fos is dispensable in this context. c-jun promotes expression of sarcomere proteins and suppresses expression of extracellular matrix proteins. Capacity of cardiac muscle to contract depends on organization of principal thick and thin filaments, myosin and actin, within the sarcomere. In line with decreased expression of sarcomere-associated proteins, Jun-deficient cardiomyocytes present disarrangement of filaments in sarcomeres and actin cytoskeleton disorganization. Moreover, Jun-deficient hearts subjected to pressure overload display pronounced fibrosis and increased myocyte apoptosis finally resulting in dilated cardiomyopathy. In conclusion, c-jun but not c-fos is required to induce a transcriptional program aimed at adapting heart growth upon increased workload.


Systemic arterial hypertension, valvular pathologies as well as myocardial infarction represent exceedingly frequent clinical manifestations contributing to heart failure and/or malignant ventricular arrhythmias [1]. Initially, these abnormalities and associated mechanical stress as well as hormonal changes induce an orchestrated signaling network in the heart that underlies myocyte growth through expansion of sarcomeres to increase contractility as well as activation of stress and fetal gene programs. In the long term, however, these mechanisms may trigger pathologic remodeling of the myocardium ultimately leading to heart dilation and reduced cardiac performance [2], [3]. Cardiomyocyte apoptosis/necrosis and progressive interstitial fibrosis are hallmarks that contribute to ventricular wall thinning and chamber dilation [4]. The latter alterations are also frequently found in dilated and hypertrophic cardiomyopathies of genetic origin that are caused by mutations in sarcomeric genes that constitute the contractile apparatus of cardiac muscle cells [5].

The Mitogen-Activated-Protein-Kinase (MAPK) family represents an essential signaling module in heart that converts extracellular stimuli, in particular mechanical stress and hormonal inputs, into subsequent cellular responses [6], [7]. MAPK signaling consists of a kinase cascade with a tripartite build-up that typically culminates in dual phosphorylation and activation of p38, c-Jun N-terminal kinases and extracellular-signal-regulated kinases (ERKs) [8]. Loss- and gain-of-function experiments in mice addressing single components of the MAPK signaling cascade revealed distinct phenotypes in heart. Enhanced signaling through ERKs led to concentric cardiac hypertrophy with maintained cardiac function [9], [10]. Increased p38 and JNK activity in heart, obtained by cardiomyocyte-specific constitutive expression of their respective upstream kinases, resulted in cardiac fibrosis and ventricular dilation in early adulthood [11][13]. In contrast, loss of JNK and p38 signaling led to increased cardiac growth at baseline, as well as in response to pressure-overload [14], [15]. Another recent study has demonstrated that specific loss of JNK1 promoted cardiomyocyte apoptosis and transient cardiac deterioration in the early response to pressure overload [16]. Interestingly, heart-restricted deletion of p38α in mice caused proliferation of adult mammalian cardiomyocytes [17].

MAPK signaling converges into early immediate activation of several transcription factors including myocyte enhancer factor 2 (MEF2) as well as Activator Protein-1 (AP-1). The role of MEF2 in cardiac development and stress adaptation has been extensively explored [18]. In contrast, the role of AP-1 in these processes remains largely unknown. AP-1 comprises a homo or heterodimeric complex that is composed of basic leucine zipper (bZIP) proteins that are subdivided into families of the Jun (c-jun, junB and junD), Fos (c-fos, fosB, fra-1 and fra-2) and the activating transcription factor ATF (ATFa, ATF2, LRF1/ATF3, ATF4 and B-ATF) [19]. Early-immediate up-regulation of AP-1 in response to cardiac hypertrophic stimuli has been reported already in nineties [20][23]. But only recently, first evidence for a requirement of AP-1 in the adult heart in vivo has been provided using mice that lack and/or ectopically express junD and fra-1, respectively [24], [25]. Preceding in vitro studies have mainly focused on the role of c-jun and c-fos in cardiomyocyte growth, two principal factors that are activated by JNK and ERK, respectively. In several of these studies, c-jun and c-fos have been suggested to be required for induction of fetal gene expression and cardiomyocyte hypertrophy in response to different stimuli [26][31]. However, studies confirming a requirement of these two transcription factors in these processes in vivo are still lacking.

We now provide genetic evidence in vivo, employing striated muscle-restricted deletion of Jun and Fos in mice, that both transcription factors are not essential for postnatal cardiac hypertrophy as well as heart growth in response to mechanical pressure overload. Remarkably however, we found that deletion of Jun but not of Fos resulted in progressive myocardial fibrosis, cardiomyocyte apoptosis and changes in sarcomeric organization. These alterations were exacerbated in response to mechanical pressure overload resulting in premature heart failure. Conclusively, while c-fos appears to be redundant in heart function, c-jun specifically counteracts pathologic remodeling of the heart subjected to pressure overload.

Materials and Methods

Ethics statement

All procedures involving animals were approved by the “Veterinäramt des Kantons Zürich” (approval number 150/2006), and conform to the relevant regulatory standards.

Generation of JunΔmu and FosΔmu mice

Floxed Jun and Fos mice (Junf/f and Fosf/f mice) have been generated by the laboratory of Prof Erwin F. Wagner as previously described [32], [33]. Mice harboring deletion of Jun or Fos in striated muscle (JunΔmu or FosΔmu) were obtained by crossing Junf/f or Fosf/f mice with mice carrying Cre recombinase under the control of the creatine kinase promoter (MCK-Cre) [34]. Resulting experimental mice were in a mixed 129/Ola-C57BL/6 background and littermates were used for experiments.

Mouse experiments

Age- (8- to 12-week-old) and weight- (22–26 g) matched mice in a mixed 129/Ola-C57BL/6 background were subjected to transverse-aortic constriction (TAC) through constriction of the descending aorta using a 27 Gauge needle as previously described [35]. Mice were anesthetized with ketamin/xylazine (2 mg/20 g and 0.2 mg/20 g, respectively) i.p. and analgized with Temgesic (0.003 mg/20 g) i.m. Mice were monitored for 6 weeks after surgery, sacrificed and heart and body weights were determined. Heart functions were assessed by echocardiography 5.5 weeks after surgery. The numbers of experimental animals are indicated in respective figure legends. Reproducibility of the induction of pressure overload by TAC performed by experimenters was previously verified [36].

Southern blotting and PCR

Genomic DNA was extracted from heart, skeletal muscle and liver of Fosf/f and FosΔmu mice, and from heart, skeletal muscle and kidney of Junf/f and JunΔmu mice, according to a standard protocol. 20 μg of genomic DNA was digested with XbaI yielding a 6.9 kb fragment for the floxed Jun allele and a 3.3 kb fragment for the deleted Jun allele. For detection of the bands, a 0.6 kb BamHI fragment from the Jun promoter region was used as a probe [37]. 20 μg of genomic DNA was digested with HindIII yielding a 6.3 kb fragment for the floxed Fos allele and a 2.9 kb fragment for the deleted Fos allele. For detection of the bands, a 0.8 kb BamHI/XbaI EGFP fragment was used as a probe. PCR analysis of genomic DNA isolated from various organs of Jun+/+, Junf/f and JunΔmu yielded a 297 bp band corresponding to the wild type alleles, a 344 bp band for the floxed alleles and a 450 bp for the deleted alleles. PCR analysis of genomic DNA isolated from various organs of Fos+/+, Fosf/f and FosΔmu yielded a 333 bp band corresponding to the wild type alleles, a 433 bp band for the floxed alleles and a 1042 bp for the deleted alleles.


Echocardiography was performed as previously described [38]. Briefly, echocardiographic measurements of mice were carried out using an ATL HDI 5000 ultrasound device (Philips Medical Systems) equipped with a 12 MHz phase array linear transducer (L-12-5). M-mode images were used for measurements of IVSd, IVSs, LVPWd, LVPWs, LVIDd, and LVIDs. Fractional shortening (FS) and Ejection Fraction (EF) were calculated using the formulas: FS (%)  =  [(LVIDd – LVIDs)/LVIDd] ×100; EF (%)  =  [(LV Vold – LV Vols)/LV Vold] ×100.

Mouse neonatal cardiomyocyte culture

Mouse neonatal hearts were isolated as previously described [24]. Briefly, cardiac ventricles were fragmented, digested with ADS buffer containing collagenase (Worthington Biochemical Corp.) and pancreatin (Sigma), and plated in plating medium containing 65% DMEM (Animed), 17% M199 (Animed), 10% Horse Serum (Invitrogen), 5% Fetal Calf Serum (Invitrogen), 2% L-Glutamine (Animed), 1% PS (Invitrogen). After 24 h, medium was changed to maintenance medium (86% DMEM, 10% M199, 1% Horse Serum, 2% L-Glutamine, 1% PS).

Histology and TUNEL Assay

Hearts were fixed in a 4% formalin solution (Medite) for 24 h at +4°C, embedded in paraffin, and cross-sections of 5 µm thickness were prepared. Sections were stained with H&E or Elastin van Gieson using standard protocols. Sections were also used for TUNEL assays (terminal deoxynucleotide transferase-mediated dUTP nick end labeling) (Roche) to assess the number of apoptotic cells. The staining was performed according to the manufacturer's instructions. The number of apoptotic cells on sections was related to the total heart area on the respective slides. Three independent sections per mouse were analyzed.

Immunofluorescence and immunochistochemistry

Immunofluorescence and immunohistochemistry on paraffin sections, as well as immunofluorescence on isolated mouse neonatal cardiomyocytes were performed according to standard protocols. The following antibodies were used: α-c-Jun (BD Transduction Laboratories), α-Collagen IV (Cedarlane), α-Periostin (Abcam), α-Actinin 1 (Sigma), α-Titin (kind gift of Dr. E. Ehler, Randall Institute, King's College London, England), α-β-Catenin (kind gift of Dr. E. Ehler Randall Institute, King's College London, England).

Western blotting

Western blotting using total heart extracts was performed according to standard procedures. The following antibodies were used: α-c-fos (Santa Cruz), α-c-jun (Santa Cruz), α-GFP (Santa Cruz), α-phospho-Smad2 (Cell Signaling), α-Smad2 (Cell Signaling), α-Periostin (Abcam), α-Myotilin (Santa Cruz), α-Tubulin (Sigma), α-GAPDH (Sigma), α-Actin (Sigma).

Gelatin zymography

Gelatin zymography of total heart proteins was performed as previously described with minor adaptations [39]. Briefly, samples (100 µg of proteins) were mixed with Laemmli sample loading buffer without β-mercaptoethanol and without boiling were loaded on 10% SDS-polyacrylamide gels containing 2 mg/ml gelatin type A from porcine skin (Sigma). After electrophoresis, gels were washed 2 times for 30 minutes in 2.5% Triton X-100 to allow proteins to renature, and then for 10 minutes in 100 mM Tris-HCl pH 7.4. Gels were then incubated at 37°C overnight in developing buffer (50 mM Tris-HCl, pH 7.5, 10 mM CaCl2, 1 µmol/L ZnCl2). Last, to reveal zones of lysis, gels were stained for 30 minutes with 0.5% Coomassie blue R250 and destained for 4 hours with 40%:10% v:v methanol:acetic acid, and then with 5%:7.5% v:v methanol:acetic acid until the stacking gel became colorless.

Quantitative RT-PCR

RNA was purified from total hearts using TRIzol Reagent (Invitrogen) according to manufacturer's instructions. 5 µg of RNA was used as a template to synthesize cDNA, using Ready-To-Go You-Prime First-Strand Beads (Amersham). Quantitative RT-PCR reactions were set up as recommended by the manufacturer (Roche) and were run and analyzed using the Roche LightCycler 480 system.

Affymetrix gene expression profiling

Affimetrix gene expression profiling was performed in collaboration with Functional Genomic Center Zürich. Total RNA was extracted from the hearts of 10 weeks old Junf/f (n = 2) and JunΔmu (n = 2) mice using TRIzol Reagent (Invitrogen). The quality of the RNA was determined with a NanoDrop ND 1000 (NanoDrop Technologies) and a Bioanalyzer 2100 (Agilent). 1 μg of RNA was reverse-transcribed into double-stranded cDNA with One-Cycle cDNA Synthesis Kit (Affymetrix), purified using a Sample Cleanup Module (Affymetrix) and then in vitro transcribed in presence of biotinlabeled nucleotides using IVT Labeling Kit (Affymetrix). Then, biotinylated cRNA was purified and its quality and quantity was determined, as described above. 5 μg of biotin-labeled cRNA was fragmented randomly to 35–200 bp and hybridized to GeneChip® GeneChip Mouse Genome 430 2.0 Arrays. The fluorescent intensity emitted by the labeled target was measure in Affymetrix GeneChip Scanner 3000 (Affymetrix). Raw data processing was performed using the Affymetrix AGCC software. Genes with significant expression difference between 2 knock-out mice and 2 wt were selected, based on the average knock-out versus wild-type value greater than 1.3 fold change with a p-value cutoff of 0.05 (using Student's t-test) or differential expression of selected genes which were confirmed by quantitative RT-PCR. The full data set is available in Gene Expression Omnibus data repository, accession number: GSE47898.

Statistical analysis

Averaged data are presented as means ±SEM. Statistical significance was calculated using an ANOVA with post-hoc Tukey's test and Student unpaired t test. Significance was accepted at the level of p<0.05.


Eccentric cardiac hypertrophy upon pressure overload in mice lacking c-Jun in cardiomyocytes

Based on in vitro studies, the AP-1 transcription factor c-jun has been suggested to be important in growth and function of the adult heart [40]. To study its role in cardiomyocytes in vivo, we generated striated muscle-restricted conditional Jun knockout mice using mice carrying floxed alleles of Jun that have been crossed to Muscle Creatine Kinase (MCK)-Cre transgenic mice [33], [34]. Southern blotting and PCR confirmed the appearance of deleted alleles in hearts and skeletal muscles of floxed Jun mice that were Cre-positive but not in non-muscle tissues. Cre-negative mice did not reveal any deletion in hearts and skeletal muscles (Figure 1A and B). An floxed band (flox) was present in all samples as recombination was not complete due to the fact that only 30 to 40% of cells in heart and skeletal muscle are muscle cells. Quantitative RT-PCR and Western Blotting, respectively, verified attenuated levels of Jun mRNA and reduced abundance of c-jun protein in hearts of Cre-positive floxed mice compared to Cre-negative floxed control mice (Figure 1C and D). Furthermore, nuclear localization of c-jun protein was detected in isolated primary neonatal cardiomyocytes of floxed control mice (here and after referred to as Junf/f mice) but not of conditional Jun knockout mice (here and after referred to as JunΔmu mice) confirming efficient deletion of Jun in cardiomyocytes in vivo (Figure 1E).

Figure 1. Generation of JunΔmu mice.

(a) Southern blot analysis of genomic DNA from total heart, skeletal muscle and kidney extracts. Deleted band (Δ band) occurs only in samples from MCK-cre positive heart and skeletal muscle. (b) PCR analysis of genomic DNA. PCR in samples from Jun+/+ (+/+), Junf/f (f/f) and JunΔmu (f/f Cre) mice yielded a 297 bp band corresponding to the wild type allele, a 344 bp band for the floxed allele and a 450 bp for the Δ allele. (c) Quantitative RT-PCR. Jun mRNA levels are down-regulated in total heart extracts from JunΔmu mice. (d) Western blot analysis of c-Jun protein levels in total heart extracts of indicated genotypes. (e) Immunofluorescence of isolated mouse neonatal cardiomycoytes. Nuclear localization of c-Jun can be observed in plated neonatal Junf/f cardiomyocytes, but not JunΔmu cardiomyocytes.

JunΔmu mice were born at Mendelian frequency and presented with normal general health, viability, fecundity, body composition and body weight as compared to control mice (Table S1). To test if in the absence of c-jun in cardiomyocytes, hearts of these animals presents increased susceptibility to the pressure induced heart failure, we subjected mice to mild transaortic constriction (TAC), a widely used model to induce pressure overload and cardiac growth [41].

Heart to body weight (H/BW) ratios significantly and similarly increased in JunΔmu and Junf/f mice upon TAC compared to sham-operated littermates (Figure 2A). H/BW ratios correlated with the average cross sectional area of cardiomyocytes in situ confirming a similar growth response in heart upon TAC (Figure S1 A and B). However, histological cross-sections revealed that hearts of JunΔmu mice were markedly dilated 6 weeks after TAC compared to hearts of Junf/f that presented with concentric myocardial growth (Figure 2B). No differences between hearts cross sections of sham-operated mice of both genotypes were detected. These observations could be confirmed by echocardiography (Table 1). Indeed, hearts of both genotypes showed significant muscle growth in response to TAC as an increase in left ventricular posterior wall (LVPW) thicknesses was observed. In comparison to sham-operated mice, left ventricular internal dimensions (LVID) were significantly decreased upon TAC in Junf/f mice. In contrast, they were markedly increased in JunΔmu mice indicating concentric and eccentric hypertrophy, respectively. As a consequence, cardiac performance was impaired in TAC-operated JunΔmu mice as significant decreases in fractional shortening (FS) and ejection fraction (EF) were observed compared to sham-operated JunΔmu mice and TAC-operated Junf/f mice. No differences in echocardiographic parameters were detected between sham-operated mice of both genotypes.

Figure 2. Eccentric cardiac hypertrophy in cJunΔmu mice upon TAC.

(a) H/BW ratios increase of JunΔmu and Junf/f mice before and after TAC. Data are presented as values ± SEM. (****) p<0.0001; n = 11–12 per group. (b) Histological analyses. H&E staining shows TAC-induced concentric growth of the heart in Junf/f mice and the heart dilation in JunΔmu mice. (c) Relative expression of indicated hypertrophic markers in hearts isolated from sham or TAC operated Junf/f and JunΔmu mice assessed by quantitative RT-PCR. Data are presented as values ± SEM. (*) p<0.05, (**) p<0.01; n = 5 per group.

Table 1. Echocardiographic analyses in JunΔmu mice after TAC.

Left ventricular remodeling upon TAC entails induction of hypertrophic marker genes such as for example atrial natriuretic factor (Anf), brain natriuretic peptide (Bnp), myosin heavy polypeptide 7 (Myh7) and skeletal muscle alpha-actin (Acta1). Quantitative RT-PCR revealed that mRNAs of Anf and Bnp were significantly increased in TAC-operated hearts of both Junf/f and JunΔmu mice (Figure 2C). Importantly, cardiac expression of Anf and Bnp was significantly greater in JunΔmu compared to Junf/f mice upon TAC. Interestingly, Anf and Bnp were also significantly enhanced in sham-operated hearts of JunΔmu mice compared to hearts of Junf/f mice. In contrast, Acta1 was expressed at significantly lower levels in hearts of JunΔmu mice at baseline, and remained low in hearts of JunΔmu mice compared to hearts of Junf/f mice in response to pressure-overload (Figure 2C). Myh7 was expressed at significantly lower levels in native hearts of JunΔmu mice, but was significantly and similarly induced in hearts of both JunΔmu and Junf/f mice upon TAC (Figure 2C). These data suggest that deletion of Jun in cardiomyocytes resulted in basal changes in expression of hypertrophic marker genes without obvious morphological signs of cardiac hypertrophy and dysfunction. Expression of these genes remained dramatically altered upon left ventricular pressure-overload and was associated with maladaptive hypertrophy.

Normal cardiac function in mice lacking Fos in cardiomyocytes

The AP-1 transcription factor c-fos has also been extensively discussed as a key player in cardiac function [40]. To study its role in cardiomyocytes in vivo, we used Fos floxed mice and crossed them to MCK-Cre transgenic mice. Southern blotting, PCR and Western blotting confirmed efficient and specific deletion of Fos in striated-muscle cells (Figure S2 A, B and C). The floxed Fos allele is generated in the way that its removal leads to GFP expression [33] that was also detected by Western Blotting in hearts of Cre-positive floxed mice (Figure S2 C). FosΔmu mice were born at Mendelian frequency and presented with normal general health, viability, fecundity, body composition and body weight as compared to Fosf/f mice (Table S2). We subsequently subjected mice to TAC. H/BW ratios significantly and equally increased in both Fosf/f and FosΔmu mice after TAC compared to sham-operated mice (Figure S3 A). Histological analyses of heart cross sections displayed an apparent increase in heart size after TAC compared to sham-operated mice of both genotypes. Importantly, no ventricular dilation could be seen in pressure-overloaded FosΔmu and Fosf/f mice (Figure S3 B). These findings were in line with our subsequent analyses by echocardiography. Sonographic assessment revealed significant and comparable increases of cardiac wall dimensions upon TAC in FosΔmu and Fosf/f mice. FS and EF were maintained in both genotypes after TAC (Table S3). Quantitative RT-PCR revealed significant and similar increases of the mRNA of hypertrophy marker genes in hearts of both genotypes compared to sham-operated mice. We observed a tendency towards enhanced induction of these genes in response to TAC in FosΔmu compared to Fosf/f mice, which was however only reaching significance for Myh7 (Figure S3 C). Thus, deletion of Fos in cardiomyocytes does not alter cardiac development, postnatal heart growth as well as cardiac hypertrophy in response to mechanical pressure overload.

Impaired myocardial remodeling in hearts lacking Jun in cardiomyocytes

In the following, we addressed cellular mechanisms underlying premature heart failure in JunΔmu mice upon mechanical pressure overload. Enhanced myocyte loss and cardiac fibrosis are key factors promoting progression of cardiac hypertrophy to heart failure [42], [43]. An Elastin van Gieson (EvG) stain that allowed for a better differential analysis of nuclei, connective tissue, muscle and elastic fibers revealed widespread myocardial fibrosis in hearts of JunΔmu mice, while no foci of apparent collagen deposition were detectable in hearts of Junf/f 6 weeks after TAC. Fibrosis in hearts of JunΔmu mice was evident already at baseline (in 12 weeks old JunΔmu mice) but was markedly aggravated upon TAC (Figure 3A). Interstitial fibrosis was associated with increased amounts of collagen type I (Col1a1), collagen type III (Col3a1) and fibronectin (Fn) (Figure 3B), all of which are commonly recognized as fibrotic markers in heart [44][47]. At baseline, JunΔmu mice showed significant up-regulation of Col1a1, Col3a1 and Fn mRNA levels in native hearts, when compared to Junf/f mice (Figure 3B). TAC further enhanced the expression of these genes in hearts of JunΔmu mice but not in hearts of Junf/f mice confirming interstitial fibrosis. Myocardial fibrosis is frequently accompanied by enhanced cardiomyocyte apoptosis. Indeed, TUNEL staining confirmed significantly increased numbers of apoptotic cardiomyocytes in JunΔmu mice upon TAC, when compared to sham-operated mice as well as TAC-operated Junf/f mice. Interestingly, already at baseline, JunΔmu mice showed significantly more TUNEL positive nuclei in hearts than Junf/f mice. The numbers of apoptotic nuclei in the hearts of Junf/f mice did not change upon TAC after 6 weeks (Figure 3C and D).

Figure 3. JunΔmu mice display impaired myocardial remodeling.

(a) Histological analyses. EvG staining reveals mild spontaneous fibrosis in hearts of JunΔmu mice, being markedly enhanced after TAC. (b) Relative expression of indicated fibrotic markers assessed by quantitative RT-PCR in hearts isolated from sham or TAC operated JunΔmu and Junf/f mice. Data are presented as values ± SEM. (*) p<0.05, (**) p<0.01, (***) p<0.001; n = 5 per group. (c) TUNEL staining of heart cross sections. TAC does not induce apoptosis in hearts of Junf/f mice. JunΔmu mice show slightly more apoptotic cardiomyocytes already at baseline, while the apoptotic rate markedly increased in hearts of JunΔmu mice upon TAC. (d) Quantification of TUNEL positive nuclei does in sham or TAC operated animals of indicated genotypes. Data are presented as values ± SEM. (*) p<0.05, (**) p<0.01.

Several matrix metalloproteinases (Mmps) that have been identified within the myocardium are dysregulated in heart failure and transcriptional regulation of Mmps by AP-1 transcription factors has been reported [43]. Cardiac mRNA levels of Mmp2 and Mmp14 were significantly upregulated in JunΔmu mice upon TAC compared to TAC-operated Junf/f and sham-treated mice of both genotypes (Figure S4 A). Mmp9 mRNA levels were slightly increased in native hearts of JunΔmu compared to Junf/f mice, however its levels in hearts of TAC operated JunΔmu mice were not altered compared to TAC operated Junf/f hearts (Figure S4 A). Other cardiac Mmps, Mmp1, Mmp13 and Mmp3 were not found deregulated (data not shown). Gelatin zymography assays confirmed that mRNA expression patterns correlated with activities of Mmp2 and Mmp9 in hearts of both genotypes (Figure S4 B).

Fibrosis and impairment of the heart function is often associated with aging. To test if deletion of Jun in heart accelerates aging of this organ, we stained cross sections of hearts isolated from one year old JunΔmu mice and Junf/f control animals with EvG staining. We observed minimal progression of fibrosis in hearts of JunΔmu mice while fibrotic remodeling was absent in hearts of control animals (Figure S5). Consistently, heart function of one year old JunΔmu mice was comparable to the aged matched control animals as revealed by echocardiography analyzes (Table S4).

Overall, cardiomyocyte-specific deletion of Jun resulted in deleterious myocardial remodeling that involved increased fibrosis associated with enhanced degradation of extracellular matrix protein and programmed cell death leading to premature heart failure under stress conditions. Although our data indicate that deficiency of Jun in heart of mice is not sufficient to provoke failure of this organ up to the age of one year, we cannot exclude that further aging would result in the impairment of cardiac function in these animals.

Upregulation of extracellular matrix and downregulation of cytoskeletal genes in hearts of JunΔmu mice

In an attempt to identify specific genes that might be globally affected in the absence of c-jun in cardiomyocytes, we compared gene expression in non-stimulated hearts from Junf/f and JunΔmu mice using Affymetrix™ oligonucleotide expression arrays. We performed these analyzes in non-stimulated conditions as hearts from JunΔmu mice already presented a mild phenotype (increased fibrosis and altered expression hypertrophic markers) but did not present functional defects. We obtained a list of 543 genes, with 211 genes up-regulated and 332 genes down-regulated, for which differential expression was greater or lesser than 1.3 fold in hearts of JunΔmu mice when compared to hearts of Junf/f mice. Importantly, we analyzed 33 genes by QPCR on the mRNA isolated from hearts of Junf/f and JunΔmu mice and confirmed deregulation of 18 of them (Table S5). Consistent with marked fibrosis in hearts of JunΔmu mice, we found several extracellular matrix genes expression of which was increased compared to hearts of c-Junf/f mice. Among other extracellular matrix genes, upregulation of periostin, connective tissue growth factor (Ctgf) and WNT1 inducible signaling pathway protein 1 (Wisp1) were most interesting, since their involvement in triggering myocardial fibrosis and heart failure has been previously established [48][52]. Quantitative RT-PCR confirmed that all genes were expressed at significantly higher levels in sham-operated hearts of JunΔmu mice than in hearts of Junf/f mice (Figure 4 A–C). Although periostin, Ctgf and Wisp1 expression was significantly enhanced upon TAC in hearts of both Junf/f and JunΔmu mice when compared to sham-operated mice, their expression in TAC-operated hearts of JunΔmu mice was markedly higher than in hearts of Junf/f mice subjected to the same procedure. Enhanced periostin expression in sham- and TAC-operated JunΔmu mice could also be confirmed at the protein level by Western blotting (Figure 4 B). Moreover, immunofluorescence revealed marked deposition of periostin in the interstitium of the myocardium of JunΔmu mice, while its accumulation was not detectable in hearts of Junf/f mice (Figure 4 C).

Figure 4. Upregulation of extracellular matrix proteins and downregulation expression of sarcomeric associated proteins in hearts of JunΔmu mice.

(a) Expression of indicated genes in hearts of sham or TAC operated mice of indicated genotypes. Data are presented as values ± SEM. (*) p<0.05, (**) p<0.01, (***) p<0.001, (****) p<0.0001; n = 5 per group. (b) Western blot analyses of Periostin abundancein hearts from sham and TAC operated JunΔmu and Junf/f mice. Tubulin was used as a loading control for the extracts. (c) Immunoflorescence staining for Periostin in cross sections of hearts from sham and TAC operated animals of indicated genotypes.

Most remarkably, 38 of deregulated candidates in hearts from JunΔmu mice were associated with muscle contraction and cytoskeleton organization. Among them myosin binding protein C 2 (Mybpc2), myotilin and β-tropomyosin 2 draw our attention as they are accessory components of the sarcomere [53][55]. Sarcomeres are the principle components of the cardiac contractile machinery composed of thick and thin filaments [56]. Importantly, sarcomeric organization increases upon hypertrophic stimuli and its disorganization is often associated with advanced cardiac hypertrophy and heart failure [57]. We studied in details the expression of Mybpc2, myotylin and β-tropomyosin 2 by QPCR in hearts from control Junf/f and JunΔmu mice. Expression of all 3 genes was markedly downregulated in unstimulated hearts from JunΔmu mice compared to unstimulated hearts from Junf/f. Moreover, their expression was markedly induced in hearts from Junf/f mice subjected to TAC but not in JunΔmu mice on which the same intervention was performed (Figure 4 D).

Thus, loss of c-Jun in cardiomyocytes leads to deregulation of several genes that are required for organization of the sarcomere. c-Jun is also required for their induction upon TAC.

c-jun regulates sarcomere organization

In our microarray expression analysis several genes that encode for components of the thick and thin filaments were found to be deregulated in hearts in the absence of Jun in cardiomyocytes. We therefore hypothesized that deletion of c-jun in cardiomyocytes affects sarcomere organization. The cultured cardiomyocyte system is particularly suited to assess sarcomere organization since morphological changes can be easily recognized since it provides much higher resolution compared to the in vivo system [57]. We therefore isolated neonatal cardiomyocytes from JunΔmu and Junf/f mice and performed immunofluorescent stainings using phalloidin that binds F-actin, as well as antibodies against α-actinin 1 that localizes to the Z-disc and against M-band titin. Phalloidin staining revealed a marked disarray of polymerized actin fibers and the sarcomeric structure appeared rudimentary in cardiomyocytes isolated from neonatal JunΔmu mice. In contrast, actin fibers were assembled in a more organized fashion into sarcomeres in control cardiomyocytes (Figure 5A). Sarcomeric α-actinin 1 and M-band titin stainings displayed a punctuated, thin and rudimentary sarcomeric structure in cardiomyocytes lacking Jun (Figure 5B), while control cells showed well-organized sarcomeres. To better describe the observed phenotype, we defined four categories of cytoskeleton organization (Figure 5C). 47% of c-jun-deficient cardiomyocytes presented poorly organized cytoskeleton compared to 11.5% of control cells. Conversely, 27.9% and 37.5% of control cardiomyocytes presented fully or well organized cytoskeleton while only 7.7% and 17.3% of c-Jun deficient cells fell into these 2 categories, respectively. Similar numbers of c-jun-deficient and control cardiomyocytes (27.9 and 23.1% respectively) presented moderately organized cytoskeleton. Overall, the quantification revealed decreased number of cells presenting organized and increased disorganized cytoskeleton in the absence of c-jun (Figure 5C).

Figure 5. Altered sarcomeric structure of isolated neonatal JunΔmu cardiomyocytes.

(a) Immunofluorescent staining. Phalloidin staining shows defects in structural organization of JunΔmu cardiomyocytes as compared to Junf/f cardiomyocytes. (b) Immunofluorescent staining. alpha actinin (αActinin) and titin staining show disruption of Z-line and M-band struture in JunΔmu cardiomyocytes as compared to Junf/f cardiomyocytes. (c) Relative percent of cardimyocytes presenting different cytoskeleton organization: blue bars – fully organize cytoskeleton, red – well organized, yellow – moderately and green – poorly organized cytoskeleton.

These results thus support a requirement of c-jun in cytoskeletal remodeling in cardiomyocytes and provide evidence that changes in expression profile of genes involved in cytoskeleton organization in c-jun-deficient cardiomyocytes result in functional changes observed in mice.


Our data demonstrate that c-Jun is necessary for maintenance of proper organization of cytoskeleton and sarcomeric structure in cardiomyocytes and protects the heart from pathologic remodeling and thus from heart dilation and heart failure, in particular under stress conditions.

c-jun and c-fos are members of the AP-1 transcription factor family. Both transcription factors have been previously shown to be upregulated upon mechanical and pharmacological hypertrophic stimuli [23], [24], [58]. However, functional relevance for this regulation has not been evidenced thus far. Our results indicate that c-jun is required for maintaining heart function during a hypertrophic response, while c-fos is dispensable. The fact that we did not observe any functional alteration in mice lacking c-fos in hearts during hypertrophic response might be explained by rapid upregulation of another member of the AP-1 family, fra-1 upon hypertrophic stimuli [24]. In fact, a previous study demonstrated that fra-1 can rescue bone development defects of c-fos-deficient mice indicating that the function of these 2 proteins might be partially redundant [59]. Moreover, fra-1 deficiency in heart does not alter the hypertrophic response [24], further supporting the possibility that functions of c-fos and fra-1 might be redundant in heart.

Previous studies implicated c-jun N-terminal kinase (JNK) in maintaining heart function after mechanical pressure overload [16], [60]. JNK activates c-jun transcriptional activity by promoting its phosphorylation [8]. Interestingly, deletion of JNK1 or the upstream kinase Mitogen-activated protein kinase kinase kinase (MEKK1) resulted in a maladaptive response to TAC. Specifically, in the absence of JNK1 or MEKK1 hearts subjected to TAC prematurely decompensated due to an increase in cardiomyocytes apoptosis. We obtained similar results in hearts of JunΔmu mice subjected to TAC as compared to control hearts. Therefore, our results indicate that the MEKK1–JNK1 signaling cascade might promote heart function upon TAC, at least partially, by activating c-jun.

In an attempt to globally identify targets of c-jun in heart, we have also performed expression arrays. Among other putative targets of c-jun, we identify extracellular matrix proteins periostin, Wisp1 and Ctgf being increased in the absence of c-jun in hearts. Expression of these 3 genes was further enhanced in c-Jun deficient hearts subjected to TAC. Importantly, expression of these genes has been previously implicated in the regulation of heart function [48][52]. In particular periostin has been broadly discussed in the context of heart function. Whether it promotes cardiomyocytes proliferation and cardiac healing after infarction remains the matter of debate [48], [52], [61]. Importantly, however, periostin was shown to promote heart dilation [51]. Therefore the increase of periostin expression and protein levels in c-jun-deficient hearts might contribute to heart failure. Unfortunately, with present data, we cannot answer if c-Jun directly promotes periostin, Wisp1 and Ctgf expression, or whether increased expression of these three genes was an indirect consequence of heart dysfunction caused by loss of c-jun in cardiomyocytes.

Expression arrays revealed that genes involved in regulation of sarcomere organization constitute a group of other potential c-jun transcriptional targets. Particularly, expression of Mybpc2, myotilin and β-tropomyosin 2 were found downregulated in the hearts of JunΔmu mice compared to hearts of Junf/f mice. Moreover, expression of these genes in JunΔmu hearts was not increased upon TAC like in hearts from control animals. Likewise, based on our results we cannot determine whether c-jun regulates these genes in a direct or indirect fashion. However, the c-jun-dependent control of genes involved in regulation of sarcomere organization prompted us to investigate the cytoskeleton and sarcomere structure functionally. Remarkably, c-jun-deficient cardiomyocytes presented disarrangement of sarcomeres and cytoskeleton. Disarrangement of sarcomeres is a hallmark of advanced heart hypertrophy and heart failure, while rapid hypertrophic stimuli increase cytoskeleton and sarcomeres organization [57]. Here, we thus identified a new transcription factor required for proper expression of components of the sarcomeric machinery and therefore for sarcomere function.

In addition to the identification of new cellular functions of c-jun in regulation of sarcomeres organization, our work revealed that deletion of c-jun in cardiomyocytes is associated with increased rate of apoptosis and fibrosis in heart. Depending on the cell type, c-jun has been reported to prevent or to promote apoptosis. In neuronal cells c-jun is required for induction of apoptosis. In contrast, c-jun is necessary for survival of hepatoblasts, hepatic tumor cells and its deletion potentiates UV and TNFα induced apoptosis of mouse embryonic fibroblasts [19], [37], [62][64]. Major mechanism of c-jun mediated suppression of apoptosis is by attenuating expression of pro-apoptotic protein p53 and its target gene noxa [37]. Interestingly, recent studies point towards p53 as a central molecule in mediating cardiomyocyte apoptosis and heart failure (for review see [65]). Although in our study deletion of Jun in heart was restricted to cardiomyocytes, based on our results we cannot define whether deletion of Jun promotes apoptosis of cardiomyocytes directly or rather cardiomyocytes deficient for this protein secrete factor/-s which promotes apoptosis of the neighboring cells in heart. Defined role of c-jun in suppressing apoptosis in other cell types in cell autonomous manner would implicate that c-jun might suppress apoptosis of cardiomyocytes directly. Based on our results we cannot point out the potential pro-apoptotic factor secreted by Jun deficient cardiomyocytes. Secreted proteins identified in our study as being upregulated in the absence of c-jun in cardiomyocytes (Periostin, Wisp1 and Ctgf) had been implicated previously as a factors rather protecting cells from apoptosis [66][71] and their increased expression in the absence of c-jun might represent mechanism to counteract apoptosis of the heart cells. Similarly, in our system we cannot define whether fibrosis observed in the absence of c-jun in cardiomyocytes is a consequence of increased apoptosis of these cells or rather increased secretion of fibrogenic mediators by c-jun deficient cardiomyocytes.

In conclusion, our study led to the identification of c-jun as a new transcription factor preventing cytoskeleton dysfunction, loss of cardiomyocytes and cardiac fibrosis, which constitute hallmarks of maladaptive cardiac growth leading to heart dilation and failure.

Supporting Information

Figure S1.

Quantification of cardiomyocyte cross-sectional area. (A) Immunochistochemical staining of heart cross-sections for collagen IV. (B) Quantification of cardiomyocyte cross-sectional area (CSA). Cardiomyocytes from Junf/f and JunΔmu mice showed a similar increase in cross-sectional area (CSA) after TAC. Data are presented as values ± SEM. (**) p<0.01; 5 mice per group were analyzed 1000 cardiomyocytes per mouse were quantified.


Figure S2.

Generation of FosΔmu mice. (A) Southern blot analysis of genomic DNA from total heart, skeletal muscle and liver extracts. Deleted band (Δ) occurs only in MCK-cre positive samples from heart and skeletal muscle, while floxed band (flox) is present in all samples. (B) PCR analysis of genomic DNA. PCR in samples from Fos+/+ (+/+), Fosf/f (f/f) and FosΔmu (f/f Cre) mice yielded a 333 bp band corresponding to the wild type alleles, a 433 bp band for the floxed alleles and a 1042 bp for the deleted alleles. (C) Western blot analysis of c-Fos protein levels in total heart extracts. Significant decrease of c-Fos is seen in hearts from FosΔmu mice as compared to Fosf/f mice. Expression of Cre-recombinase in the heart leads to expression of GFP. Actin was used as a loading control.


Figure S3.

FosΔmu mice show concentric heart hypertrophy upon TAC. (A) H/BW ratio increases significantly in both Fosf/f and cFosΔmu mice upon TAC. Data are presented as values ± SEM. (*) p<0.05; n = 4–6 per group. (B) Histological analyses. H&E staining of heart cross-sections shows slight increase in left-ventricle wall thickness in both TAC-operated groups. (C) Relative expression of hypertrophic markers assessed by quantitative RT-PCR. Anf, Bnp, Acta1, and Myh7 are re-expressed in hypertrophied hearts of Fosf/f and FosΔmu mice. (*) p<0.05, (**) p<0.01, (***) p<0.001, (****) p<0.0001; n = 4–6 per group.


Figure S4.

TAC-induced cardiac fibrosis in JunΔmu mice is associated with enhanced MMPs expression and activity. (A) Relative expression of myocardial MMPs (as indicated) assessed by quantitative RT-PCR, in sham and TAC operated mice from indicated genotypes. Data are presented as values ± SEM. (*) p<0.05, (**) p<0.01; n = 5 per group. (B) Gelatin zymography on total heart protein extracts. TAC-operated JunΔmu mice show greatly increased activity of MMP-2 (arrow at 66 kDa), and slightly decreased activity of MMP-9 (arrow at 92 kDa) in hearts as compared to sham-operated mice and TAC-operated Junf/f mice. No difference in MMP-2 and MMP-9 activity in hearts is observed between TAC operated Junf/f mice, when compared to sham-operated controls, as well as sham-operated Junf/f and JunΔmu mice.


Figure S5.

Hearts of one year old JunΔmu mice present spontaneous fibrosis. (A) Normal H/BW ratio of one year old JunΔmu mice. (B) Histological analyses. EvG staining reveals spontaneous fibrosis in hearts of one year old JunΔmu mice.


Table S1.

Body and organs weights in adult JunΔmu mice and corresponding control mice.


Table S2.

Body and organs weights in adult FosΔmu mice and corresponding control mice.


Table S3.

Echocardiographic analyses in FosΔmu mice after TAC.


Table S4.

Echocardiographic assessment of heart function in one year old JunΔmu and corresponding control mice.



We would like to thank Prof. Thomas F. Luscher and Dr. Christian M. Matter for their support during the initial phase of this study, Dr. Izabela Sumara for the help with immunoflorescence techniques and Dr. Olga Sumara for her critical comments to the manuscript.

Author Contributions

Conceived and designed the experiments: RR GS RW. Performed the experiments: RW JM AF AA GS. Analyzed the data: RW JM AF AA GS. Contributed reagents/materials/analysis tools: EFW TP. Wrote the paper: RR GS.


  1. 1. Hill JA, Olson EN (2008) Cardiac plasticity. N Engl J Med 358: 1370–1380.
  2. 2. Olson EN (2004) A decade of discoveries in cardiac biology. Nat Med 10: 467–474.
  3. 3. Hoshijima M, Chien KR (2002) Mixed signals in heart failure: cancer rules. J Clin Invest 109: 849–855.
  4. 4. Chien KR (1999) Stress pathways and heart failure. Cell 98: 555–558.
  5. 5. Morita H, Seidman J, Seidman CE (2005) Genetic causes of human heart failure. J Clin Invest 115: 518–526.
  6. 6. Liang Q, Molkentin JD (2003) Redefining the roles of p38 and JNK signaling in cardiac hypertrophy: dichotomy between cultured myocytes and animal models. J Mol Cell Cardiol 35: 1385–1394.
  7. 7. Heineke J, Molkentin JD (2006) Regulation of cardiac hypertrophy by intracellular signalling pathways. Nat Rev Mol Cell Biol 7: 589–600.
  8. 8. Chang L, Karin M (2001) Mammalian MAP kinase signalling cascades. Nature 410: 37–40.
  9. 9. Bueno OF, De Windt LJ, Tymitz KM, Witt SA, Kimball TR, et al. (2000) The MEK1-ERK1/2 signaling pathway promotes compensated cardiac hypertrophy in transgenic mice. EMBO J 19: 6341–6350.
  10. 10. Sanna B, Bueno OF, Dai YS, Wilkins BJ, Molkentin JD (2005) Direct and indirect interactions between calcineurin-NFAT and MEK1-extracellular signal-regulated kinase 1/2 signaling pathways regulate cardiac gene expression and cellular growth. Mol Cell Biol 25: 865–878.
  11. 11. Liao P, Georgakopoulos D, Kovacs A, Zheng M, Lerner D, et al. (2001) The in vivo role of p38 MAP kinases in cardiac remodeling and restrictive cardiomyopathy. Proc Natl Acad Sci U S A 98: 12283–12288.
  12. 12. Petrich BG, Molkentin JD, Wang Y (2003) Temporal activation of c-Jun N-terminal kinase in adult transgenic heart via cre-loxP-mediated DNA recombination. FASEB J 17: 749–751.
  13. 13. Petrich BG, Gong X, Lerner DL, Wang X, Brown JH, et al. (2002) c-Jun N-terminal kinase activation mediates downregulation of connexin43 in cardiomyocytes. Circ Res 91: 640–647.
  14. 14. Liang Q, Bueno OF, Wilkins BJ, Kuan CY, Xia Y, et al. (2003) c-Jun N-terminal kinases (JNK) antagonize cardiac growth through cross-talk with calcineurin-NFAT signaling. EMBO J 22: 5079–5089.
  15. 15. Braz JC, Bueno OF, Liang Q, Wilkins BJ, Dai YS, et al. (2003) Targeted inhibition of p38 MAPK promotes hypertrophic cardiomyopathy through upregulation of calcineurin-NFAT signaling. J Clin Invest 111: 1475–1486.
  16. 16. Tachibana H, Perrino C, Takaoka H, Davis RJ, Naga Prasad SV, et al. (2006) JNK1 is required to preserve cardiac function in the early response to pressure overload. Biochem Biophys Res Commun 343: 1060–1066.
  17. 17. Engel FB, Schebesta M, Duong MT, Lu G, Ren S, et al. (2005) p38 MAP kinase inhibition enables proliferation of adult mammalian cardiomyocytes. Genes Dev 19: 1175–1187.
  18. 18. Potthoff MJ, Olson EN (2007) MEF2: a central regulator of diverse developmental programs. Development 134: 4131–4140.
  19. 19. Eferl R, Wagner EF (2003) AP-1: a double-edged sword in tumorigenesis. Nat Rev Cancer 3: 859–868.
  20. 20. Parker TG, Schneider MD (1991) Growth factors, proto-oncogenes, and plasticity of the cardiac phenotype. Annu Rev Physiol 53: 179–200.
  21. 21. Schneider MD, McLellan WR, Black FM, Parker TG (1992) Growth factors, growth factor response elements, and the cardiac phenotype. Basic Res Cardiol 87 Suppl 233–48.
  22. 22. Komuro I, Kaida T, Shibazaki Y, Kurabayashi M, Katoh Y, et al. (1990) Stretching cardiac myocytes stimulates protooncogene expression. J Biol Chem 265: 3595–3598.
  23. 23. Sadoshima J, Izumo S (1997) The cellular and molecular response of cardiac myocytes to mechanical stress. Annu Rev Physiol 59: 551–571.
  24. 24. Ricci R, Eriksson U, Oudit GY, Eferl R, Akhmedov A, et al. (2005) Distinct functions of junD in cardiac hypertrophy and heart failure. Genes Dev 19: 208–213.
  25. 25. Hilfiker-Kleiner D, Hilfiker A, Kaminski K, Schaefer A, Park JK, et al. (2005) Lack of JunD promotes pressure overload-induced apoptosis, hypertrophic growth, and angiogenesis in the heart. Circulation 112: 1470–1477.
  26. 26. Omura T, Yoshiyama M, Yoshida K, Nakamura Y, Kim S, et al. (2002) Dominant negative mutant of c-Jun inhibits cardiomyocyte hypertrophy induced by endothelin 1 and phenylephrine. Hypertension 39: 81–86.
  27. 27. Taimor G, Schluter KD, Best P, Helmig S, Piper HM (2004) Transcription activator protein 1 mediates alpha- but not beta-adrenergic hypertrophic growth responses in adult cardiomyocytes. Am J Physiol Heart Circ Physiol 286: H2369–2375.
  28. 28. Bishopric NH, Jayasena V, Webster KA (1992) Positive regulation of the skeletal alpha-actin gene by Fos and Jun in cardiac myocytes. J Biol Chem 267: 25535–25540.
  29. 29. Kovacic-Milivojevic B, Gardner DG (1992) Divergent regulation of the human atrial natriuretic peptide gene by c-jun and c-fos. Mol Cell Biol 12: 292–301.
  30. 30. Rosenzweig A, Halazonetis TD, Seidman JG, Seidman CE (1991) Proximal regulatory domains of rat atrial natriuretic factor gene. Circulation 84: 1256–1265.
  31. 31. Paradis P, MacLellan WR, Belaguli NS, Schwartz RJ, Schneider MD (1996) Serum response factor mediates AP-1-dependent induction of the skeletal alpha-actin promoter in ventricular myocytes. J Biol Chem 271: 10827–10833.
  32. 32. Behrens A, Sibilia M, David JP, Mohle-Steinlein U, Tronche F, et al. (2002) Impaired postnatal hepatocyte proliferation and liver regeneration in mice lacking c-jun in the liver. Embo J 21: 1782–1790.
  33. 33. Fleischmann A, Hvalby O, Jensen V, Strekalova T, Zacher C, et al. (2003) Impaired long-term memory and NR2A-type NMDA receptor-dependent synaptic plasticity in mice lacking c-Fos in the CNS. J Neurosci 23: 9116–9122.
  34. 34. Bruning JC, Michael MD, Winnay JN, Hayashi T, Horsch D, et al. (1998) A muscle-specific insulin receptor knockout exhibits features of the metabolic syndrome of NIDDM without altering glucose tolerance. Mol Cell 2: 559–569.
  35. 35. Kassiri Z, Oudit GY, Sanchez O, Dawood F, Mohammed FF, et al. (2005) Combination of tumor necrosis factor-alpha ablation and matrix metalloproteinase inhibition prevents heart failure after pressure overload in tissue inhibitor of metalloproteinase-3 knock-out mice. Circ Res 97: 380–390.
  36. 36. Krishnan J, Suter M, Windak R, Krebs T, Felley A, et al. (2009) Activation of a HIF1alpha-PPARgamma axis underlies the integration of glycolytic and lipid anabolic pathways in pathologic cardiac hypertrophy. Cell Metab 9: 512–524.
  37. 37. Eferl R, Ricci R, Kenner L, Zenz R, David JP, et al. (2003) Liver tumor development. c-Jun antagonizes the proapoptotic activity of p53. Cell 112: 181–192.
  38. 38. Crackower MA, Oudit GY, Kozieradzki I, Sarao R, Sun H, et al. (2002) Regulation of myocardial contractility and cell size by distinct PI3K-PTEN signaling pathways. Cell 110: 737–749.
  39. 39. Li YY, Feldman AM, Sun Y, McTiernan CF (1998) Differential expression of tissue inhibitors of metalloproteinases in the failing human heart. Circulation 98: 1728–1734.
  40. 40. Sugden PH (2001) Signalling pathways in cardiac myocyte hypertrophy. Ann Med 33: 611–622.
  41. 41. Rockman HA, Ross RS, Harris AN, Knowlton KU, Steinhelper ME, et al. (1991) Segregation of atrial-specific and inducible expression of an atrial natriuretic factor transgene in an in vivo murine model of cardiac hypertrophy. Proc Natl Acad Sci U S A 88: 8277–8281.
  42. 42. Kang PM, Izumo S (2003) Apoptosis in heart: basic mechanisms and implications in cardiovascular diseases. Trends Mol Med 9: 177–182.
  43. 43. Spinale FG (2007) Myocardial matrix remodeling and the matrix metalloproteinases: influence on cardiac form and function. Physiol Rev 87: 1285–1342.
  44. 44. Seeland U, Haeuseler C, Hinrichs R, Rosenkranz S, Pfitzner T, et al. (2002) Myocardial fibrosis in transforming growth factor-beta(1) (TGF-beta(1)) transgenic mice is associated with inhibition of interstitial collagenase. Eur J Clin Invest 32: 295–303.
  45. 45. Brooks WW, Conrad CH (2000) Myocardial fibrosis in transforming growth factor beta(1)heterozygous mice. J Mol Cell Cardiol 32: 187–195.
  46. 46. Villarreal FJ, Dillmann WH (1992) Cardiac hypertrophy-induced changes in mRNA levels for TGF-beta 1, fibronectin, and collagen. Am J Physiol 262: H1861–1866.
  47. 47. Villarreal FJ, Lee AA, Dillmann WH, Giordano FJ (1996) Adenovirus-mediated overexpression of human transforming growth factor-beta 1 in rat cardiac fibroblasts, myocytes and smooth muscle cells. J Mol Cell Cardiol 28: 735–742.
  48. 48. Lorts A, Schwanekamp JA, Elrod JW, Sargent MA, Molkentin JD (2009) Genetic manipulation of periostin expression in the heart does not affect myocyte content, cell cycle activity, or cardiac repair. Circ Res 104: e1–7.
  49. 49. Duisters RF, Tijsen AJ, Schroen B, Leenders JJ, Lentink V, et al.. (2009) miR-133 and miR-30 regulate connective tissue growth factor: implications for a role of microRNAs in myocardial matrix remodeling. Circ Res 104: 170–178, 176p following 178.
  50. 50. Shanmugam P, Valente AJ, Prabhu SD, Venkatesan B, Yoshida T, et al. (2011) Angiotensin-II type 1 receptor and NOX2 mediate TCF/LEF and CREB dependent WISP1 induction and cardiomyocyte hypertrophy. J Mol Cell Cardiol 50: 928–938.
  51. 51. Katsuragi N, Morishita R, Nakamura N, Ochiai T, Taniyama Y, et al. (2004) Periostin as a novel factor responsible for ventricular dilation. Circulation 110: 1806–1813.
  52. 52. Kuhn B, del Monte F, Hajjar RJ, Chang YS, Lebeche D, et al. (2007) Periostin induces proliferation of differentiated cardiomyocytes and promotes cardiac repair. Nat Med 13: 962–969.
  53. 53. Muthuchamy M, Grupp IL, Grupp G, O'Toole BA, Kier AB, et al. (1995) Molecular and physiological effects of overexpressing striated muscle beta-tropomyosin in the adult murine heart. J Biol Chem 270: 30593–30603.
  54. 54. Otey CA, Rachlin A, Moza M, Arneman D, Carpen O (2005) The palladin/myotilin/myopalladin family of actin-associated scaffolds. Int Rev Cytol 246: 31–58.
  55. 55. Flashman E, Redwood C, Moolman-Smook J, Watkins H (2004) Cardiac myosin binding protein C: its role in physiology and disease. Circ Res 94: 1279–1289.
  56. 56. Ferrari MB, Podugu S, Eskew JD (2006) Assembling the myofibril: coordinating contractile cable construction with calcium. Cell Biochem Biophys 45: 317–337.
  57. 57. Aoki H, Sadoshima J, Izumo S (2000) Myosin light chain kinase mediates sarcomere organization during cardiac hypertrophy in vitro. Nat Med 6: 183–188.
  58. 58. Chien KR, Zhu H, Knowlton KU, Miller-Hance W, van-Bilsen M, et al. (1993) Transcriptional regulation during cardiac growth and development. Annu Rev Physiol 55: 77–95.
  59. 59. Fleischmann A, Hafezi F, Elliott C, Reme CE, Ruther U, et al. (2000) Fra-1 replaces c-Fos-dependent functions in mice. Genes Dev 14: 2695–2700.
  60. 60. Sadoshima J, Montagne O, Wang Q, Yang G, Warden J, et al. (2002) The MEKK1-JNK pathway plays a protective role in pressure overload but does not mediate cardiac hypertrophy. J Clin Invest 110: 271–279.
  61. 61. Shimazaki M, Nakamura K, Kii I, Kashima T, Amizuka N, et al. (2008) Periostin is essential for cardiac healing after acute myocardial infarction. J Exp Med 205: 295–303.
  62. 62. Wisdom R, Johnson RS, Moore C (1999) c-Jun regulates cell cycle progression and apoptosis by distinct mechanisms. EMBO J 18: 188–197.
  63. 63. Eferl R, Sibilia M, Hilberg F, Fuchsbichler A, Kufferath I, et al. (1999) Functions of c-Jun in liver and heart development. J Cell Biol 145: 1049–1061.
  64. 64. Shaulian E, Karin M (2002) AP-1 as a regulator of cell life and death. Nat Cell Biol 4: E131–136.
  65. 65. Fujita T, Ishikawa Y (2011) Apoptosis in heart failure. -The role of the beta-adrenergic receptor-mediated signaling pathway and p53-mediated signaling pathway in the apoptosis of cardiomyocytes. Circ J 75: 1811–1818.
  66. 66. Gravning J, Orn S, Kaasboll OJ, Martinov VN, Manhenke C, et al. (2012) Myocardial connective tissue growth factor (CCN2/CTGF) attenuates left ventricular remodeling after myocardial infarction. PLoS One 7: e52120.
  67. 67. Ahmed MS, Gravning J, Martinov VN, von Lueder TG, Edvardsen T, et al. (2011) Mechanisms of novel cardioprotective functions of CCN2/CTGF in myocardial ischemia-reperfusion injury. Am J Physiol Heart Circ Physiol 300: H1291–1302.
  68. 68. Moe IT, Pham TA, Hagelin EM, Ahmed MS, Attramadal H (2013) CCN2 exerts direct cytoprotective actions in adult cardiac myocytes by activation of the PI3-kinase/Akt/GSK-3beta signaling pathway. J Cell Commun Signal 7: 31–47.
  69. 69. Venkatesan B, Prabhu SD, Venkatachalam K, Mummidi S, Valente AJ, et al. (2010) WNT1-inducible signaling pathway protein-1 activates diverse cell survival pathways and blocks doxorubicin-induced cardiomyocyte death. Cell Signal 22: 809–820.
  70. 70. Su F, Overholtzer M, Besser D, Levine AJ (2002) WISP-1 attenuates p53-mediated apoptosis in response to DNA damage through activation of the Akt kinase. Genes Dev 16: 46–57.
  71. 71. Li B, Wang L, Chi B (2013) Upregulation of periostin prevents P53-mediated apoptosis in SGC-7901 gastric cancer cells. Mol Biol Rep 40: 1677–1683.