Impaired relaxation despite upregulated calcium-handling protein atrial myocardium from type 2 diabetic patients with preserved ejection fraction
© Lamberts et al.; licensee BioMed Central Ltd. 2014
Received: 27 January 2014
Accepted: 26 March 2014
Published: 5 April 2014
Diastolic dysfunction is a key factor in the development and pathology of cardiac dysfunction in diabetes, however the exact underlying mechanism remains unknown, especially in humans. We aimed to measure contraction, relaxation, expression of calcium-handling proteins and fibrosis in myocardium of diabetic patients with preserved systolic function.
Right atrial appendages from patients with type 2 diabetes mellitus (DM, n = 20) and non-diabetic patients (non-DM, n = 36), all with preserved ejection fraction and undergoing coronary artery bypass grafting (CABG), were collected. From appendages, small cardiac muscles, trabeculae, were isolated to measure basal and β-adrenergic stimulated myocardial function. Expression levels of calcium-handling proteins, sarcoplasmic reticulum Ca2+ ATPase (SERCA2a) and phospholamban (PLB), and of β1-adrenoreceptors were determined in tissue samples by Western blot. Collagen deposition was determined by picro-sirius red staining.
In trabeculae from diabetic samples, contractile function was preserved, but relaxation was prolonged (Tau: 74 ± 13 ms vs. 93 ± 16 ms, non-DM vs. DM, p = 0.03). The expression of SERCA2a was increased in diabetic myocardial tissue (0.75 ± 0.09 vs. 1.23 ± 0.15, non-DM vs. DM, p = 0.007), whereas its endogenous inhibitor PLB was reduced (2.21 ± 0.45 vs. 0.42 ± 0.11, non-DM vs. DM, p = 0.01). Collagen deposition was increased in diabetic samples. Moreover, trabeculae from diabetic patients were unresponsive to β-adrenergic stimulation, despite no change in β1-adrenoreceptor expression levels.
Human type 2 diabetic atrial myocardium showed increased fibrosis without systolic dysfunction but with impaired relaxation, especially during β-adrenergic challenge. Interestingly, changes in calcium-handling protein expression suggests accelerated active calcium re-uptake, thus improved relaxation, indicating a compensatory calcium-handling mechanism in diabetes in an attempt to maintain diastolic function at rest despite impaired relaxation in the diabetic fibrotic atrial myocardium. Our study addresses important aspects of the underlying mechanisms of diabetes-associated diastolic dysfunction, which is crucial to developing new therapeutic treatments.
KeywordsDiastolic dysfunction Human myocardium Type 2 diabetes Relaxation Contraction Adrenergic regulation Calcium signaling Myocardial fibrosis
Impaired cardiac function during diastole is one of the early manifestations of cardiac dysfunction in type 2 diabetes, and it makes type 2 diabetic patients prone to developing clinical features of heart failure, with both preserved and reduced ejection fraction (EF)[2, 3]. Diastolic function deteriorates progressively over time, but the exact mechanisms underlying this clinically important increased stiffness and/or impaired relaxation, especially in diabetes, remain unclear. In contrast to systolic dysfunction, treatments for diastolic dysfunction are limited, which is likely due to this lack of knowledge regarding the pathophysiology of diastolic dysfunction.
The diastolic properties of the heart are determined by factors influencing both the passive compliance and the active processes of myocardial relaxation. Thus far, studies using animals with type 1 diabetes and diabetic patients with reduced EF have found increased collagen deposition, which stiffens the extracellular myocardial matrix. More recently, the slow/incomplete removal of Ca2+ from the cytosol during the diastolic period, predominantly governed by the activity of the important sarcoplasmic reticulum Ca2+ ATPase (SERCA2a) under direct control of its endogenous inhibitor phospholamban (PLB), has been shown to contribute to the impaired myocardial relaxation in early diastolic dysfunction. However, the underlying changes in these important calcium-handling proteins are yet to be examined in human diabetic myocardium with preserved EF. Moreover, as impaired diastolic function limits cardiac performance during exercise and leads to an intolerance to tachycardia, it is also crucial to determine how relaxation is challenged by β-adrenergic stimulation, one of the most important extrinsic physiological stimulus of the myocardium.
Therefore we aimed to assess the impact of diabetes on the diastolic function of the atrial myocardium from patients with preserved EF and determine alterations in the calcium-handling proteins specifically linked to myocardial relaxation. To this end we combined active force and relaxation measurements in isolated right atrial cardiac muscles from non-diabetic and diabetic patients with preserved EF and coronary artery disease (CAD), undergoing coronary artery bypass graft (CABG) surgery. Expression levels of calcium-handling proteins and β1-adrenoreceptors were determined via protein analysis and atrial myocardial fibrosis by measuring collagen deposition.
Our study shows for the first time that in human atrial myocardium from diabetic patients with preserved EF and CAD, the force generation is preserved, whereas the relaxation is impaired, and the right atrial cardiac muscles were unresponsive to β-adrenergic stimulation. The impairment in relaxation is associated with an unexpected increase in SERCA2a/PLB protein ratio in the diabetic myocardium suggesting accelerated relaxation. This may indicate a compensatory mechanism in an attempt to maintain diastolic function at rest in the fibrotic diabetic atrial myocardium.
The study was approved by the local Human Ethics Committee (Approval number: LRS12-01-001) and informed consent was obtained. Human right atrial appendages (RAAs) were acquired from patients with type 2 diabetes mellitus (DM, n = 20) and non-diabetic patients (non-DM, n = 36) with CAD who underwent CABG surgery. Non-diabetic patients were classified as having a fasting plasma glucose ≤ 6 mmol/L or an HbA1c score ≤ 6.5% (48 mmol/mol). DM patients were selected based on their clinical diagnosis of type 2 diabetes with duration of more than 1 year. CAD was of such severity as to meet the indications for CABG, which in the majority of cases was triple vessel or high-grade double vessel disease (number of grafts per patient 3.7 ± 0.2 vs. 3.5 ± 0.3, non-DM vs. DM, p = 0.68). Patients requiring emergency CABG, patients with on-going myocardial ischemia prior to CABG and those undergoing concomitant cardiac surgical procedures in addition to CABG were excluded.
All patients had a clinically indicated pre-operative transthoracic echocardiogram, using a Vivid S6, 7, or E9 ultrasound system (GE Vingmed Ultrasound, Horten, Norway). Images were obtained by professional echosonographers, and reviewed offline by a European Association of Cardiovascular Imaging accredited cardiologist. Left ventricular (LV) and left atrial (LA) chamber volumes were derived from a biplane method of discs using the apical 4-chamber and 2-chamber views. Cardiac output measurements were calculated applying the heart rate recorded during the apical 4-chamber view. Ejection fraction (EF) was graded according to the European Association of Echocardiography/American Society of Echocardiography recommendations as preserved (> 50%). LV mass was calculated according Devereux et al., whereas LV volume/mass ratio was calculated at end-systole (LVESV/LV mass).
Tissue acquisition and preservation
In all patients, RAAs were removed under normothermic conditions before cross clamping for cardiopulmonary bypass. Immediately after removal, all specimens were placed in a sealed vial containing a modified, low Ca2+ (0.5 mM) Krebs-Henseleit buffer ((mM): 118.5 NaCl, 4.5 KCl, 1.4 CaCl2, 0.3 NaH2PO4, 1.0 MgCl26H2O, 25 NaHCO3 and 11 glucose) with 6.25 mM 2,3-butanedione monoxime (BDM) previously well oxygenated with carbogen (95%O2–5%CO2). Within 5–10 minutes after removal, the appendages were either dissected into several pieces, flash-frozen and stored at 80°C or fixed in 4% (v/v) formaldehyde solution and stored at -20°C. In a subset of the study, half of the RAA tissue was used immediately to conduct the functional force measurements.
Functional force measurements
From myocardial samples, tiny cardiac muscles (trabeculae) were freshly dissected, transferred to an experimental bath and attached between a force transducer and a micromanipulator. The basal and length dependency of force development were measured in the isolated trabeculae, as previously described. The muscles were constantly superfused with a modified oxygenated Krebs–Henseleit solution, as indicated above but without BDM and at 1.4 mM Ca2+, kept at 40°C and continuously stimulated at 60 bpm (1 Hz). After mounting, the preparations were stimulated for 1 h to allow equilibration. To impose similar stretch levels the muscles in both groups were stretched to the length (Lmax) at which isometric developed force was maximal. After determination of basal force developed (Fdev), length dependency was tested by changing muscle length from 80% to 100% Lmax with 5% incrementing steps. Hereafter the response to β-adrenoceptor stimulation on force development was tested with incrementing doses of dobutamine (10-7 to 10-5 M) given at 6 minutes interval.
Tissue lysate preparation and protein analysis
Total myocardial sample lysates were prepared by manual grinding and followed by suspension in 1.5-fold (w/v) sodium dodecyl sulphate (SDS) lysis buffer (3% (w/v) SDS, 50 mM Tris–HCl (pH 7.5) and protease inhibitor mix composed of 1 mM benzamidine, 2 μg/mL leupeptin, 2 μg/mL pepstatin A, 2 μg/mL aprotinin and 0.5 mM phenylmethylsulfonyl fluoride). The homogenate was incubated on ice for 1 hour, at room temperature for 45 minutes and then centrifuged at 21,000 g for 30 minutes at 4°C where after supernatant was collected. Protein concentrations were determined using the DC protein determination kit (BioRAD) according to manufacturer’s protocol and samples volumes were adjusted for loading. Unless otherwise noted samples were further solubilized in 2× Laemmli sample buffer (65.8 mM Tris–HCl, pH 6.8, 2.1% SDS, 26.3% (w/v) glycerol, 0.01% bromophenol blue) containing 5% β-mercaptoethanol (v/v). Ryanodine receptor (RyR2), SERCA2a, PLB and β1-adrenoreceptor were detected from 75, 60, 50 or 25 μg of lysate, respectively, and glyceraldehyde 3-phosphate dehydrogenase (GAPDH) or β-actin was also identified in each loading condition. Following transfer onto nitrocellulose the membranes were blocked for 1 hour with phosphate buffered saline (PBS, pH 7.4), containing 0.5% Tween 20 and 5% (w/v) skimmed milk. For β1-adrenoceptor and β-actin proteins were transferred onto Polyvinylidene fluoride (PVDF) membranes, blocked for 1 hour with Tris buffered saline (TBS, pH 7.4). The blots were probed with specific antibodies against RyR2, SERCA2a, PLB, GAPDH (Badrilla Ltd), β1-adrenoreceptor (Novus Biologicals) or β-actin (Sapphire Bioscience Pty.Ltd) with corresponding peroxidase conjugated secondary antibodies (Sapphire Bioscience Pty.Ltd). All proteins were detected using an enhanced chemiluminescence kit. Protein band densities were normalized to GAPDH or β-actin as an internal control and are expressed as protein to GAPDH or β-actin ratio. For β1–adrenoceptor (AR) blots, β-actin was used as an internal control because GADP was to close to the β1-AR bands to be separated accurately. Although some studies suggested an impact of diabetes on the gene expression of GAPDH, others and ours did not observe any changes in protein expression of GAPDH or of β-actin (both p > 0.05) between non-DM and DM samples.
Formalin fixed, optical cutting temperature embedded myocardial samples tissue sections of 8 μm thickness were washed with distilled water and PBS, and subsequently exposed to a picro-sirius red solution (0.001% (w/v) sirius red in saturated aqueous picric acid) for 1 hour. Tissue sections were then washed in acidified H2O (0.5% (v/v) acetic acid in H2O) for 10 minutes. Slices were dehydrogenated in an ascending ethanol sequence (85%, 95% and 100% (v/v) in H2O) and washed in xylene. Finally, slices were embedded in a distrene-plasticiser-xylene mounting medium. Images obtained by light microscopy were digitized and analyzed using ImageJ v1.46 software to quantify the percentage of collagen content (fibrosis), as previously described. Briefly, the number of red pixels above a set threshold (similar for all images) was calculated from the total pixel area of interest. The area of cardiomyocytes and collagen, excluding the lumen (i.e. empty spaces), determined the total area of interest. The mean percentage of collagen deposition from 21 randomly selected images was calculated to represent the level of collagen of one RAA.
Differences among groups were compared either using a t-test, chi-square or a two-way ANOVA followed by a Bonferroni post-hoc test as indicated in the legends of the tables and Figures. A p-value of < 0.05 was considered statistically significant. Data are expressed as mean ± SEM.
Non-DM (n = 36)
DM (n = 20)
67 ± 1
68 ± 2
28.2 ± 0.9
33.8 ± 1.6
Blood glucose (mmol/L)
5.9 ± 0.3
10.0 ± 1.0
HbA1c (%) (mmol/mol)
5.8 ± 0.3 (40 ± 1)
7.5 ± 1.2 (58 ± 4)
Diabetes duration (years)
11.6 ± 2.7
Systolic BP (mmHg)
129 ± 3
133 ± 4
Diastolic BP (mmHg)
73 ± 2
70 ± 2
Heart rate (bpm)
64 ± 1
69 ± 2
104 ± 3
95 ± 5
43 ± 2
39 ± 4
61 ± 2
56 ± 3
Cardiac Output (L/min)
3.8 ± 0.1
4.0 ± 0.1
Ejection Fraction (%)
60 ± 1
60 ± 2
1.14 ± 0.04
1.26 ± 0.06
1.05 ± 0.03
1.15 ± 0.06
4.76 ± 0.09
4.72 ± 0.15
3.04 ± 0.10
3.04 ± 0.14
LV mass (g)
193 ± 11
217 ± 18
LV volume/mass (ml/g)
0.22 ± 0.03
0.19 ± 0.03
0.68 ± 0.03
0.79 ± 0.05
0.69 ± 0.03
0.80 ± 0.05
1.05 ± 0.08
0.99 ± 0.08
0.069 ± 0.003
0.067 ± 0.004
10.5 ± 0.8
12.6 ± 1.1
226 ± 7
259 ± 13
4.0 ± 0.1
4.1 ± 0.2
ACE inhibitors/AT blockers
Calcium Channel blocker
Human atrial myocardial function
Basal characteristics and functional parameters of human cardiac muscle
Non-DM (n = 8)
DM (n = 6)
0.046 ± 0.036
0.051 ± 0.043
1.73 ± 0.58
1.34 ± 0.15
23.7 ± 3.6
23.1 ± 1.1
298 ± 37
277 ± 21
145 ± 16
139 ± 7
-204 ± 20
-130 ± 16
166 ± 9
209 ± 6
74 ± 4
93 ± 7
Calcium-handling proteins expression levels
Human atrial myocardial functional response to β-adrenergic stimulation
Our findings show that in human right atrial myocardium from type 2 diabetic patients, with CAD and preserved EF, the contractile state is preserved, whereas relaxation is impaired, despite an increase in SERCA2a:PLB expression ratio. This is associated with an increased level of atrial myocardial fibrosis. The increase in SERCA2a:PLB ratio may suggest a compensatory mechanism in an attempt to maintain diastolic function at rest despite impaired relaxation in the fibrotic diabetic atrial myocardium. We also show for the first time that human right atrial cardiac muscles from patients with type 2 diabetes and preserved EF are unresponsive to β-adrenergic stimulation without a change in expression level of the β1-adrenoreceptors, suggesting impaired downstream β-adrenergic modulation. Our study provides novel information on the underlying pathology of diastolic dysfunction in the diabetic myocardium, strengthening the knowledge base for the development of therapeutics, which are currently very limited for diastolic dysfunction[5, 22].
Impaired relaxation in human right atrial diabetic myocardium at rest
Our in vivo echocardiography data and our ex vivo cardiac muscle data confirmed both preserved contractile function with no development of structural cardiac hypertrophy in diabetic patients with preserved EF. Echocardiography of the left ventricle also revealed a slower early filling time (prolonged deceleration time) and higher filling pressures during early filling (increased E/e’) with a tendency to slower early and late filling velocities (E and A, respectively), which in the isolated right atrial muscles were accompanied by prolongations of early and late relaxation (decreased -dF/dtmin and prolonged Tau). Together these data indicate reduced diastolic function due to impaired relaxation and increased myocardial stiffness of the heart in the diabetic population with preserved EF. This is consistent with previous echocardiography findings in type 1 and type 2 diabetic patients[2, 23] and with functional myocardial studies in type 1 and type 2 diabetic animal models, however the myocardial diastolic dysfunction observed in animal models was always accompanied by systolic dysfunction. On the contrary, Reuter et al. have reported no difference in the rate of relaxation or the contractile function of right atrial cardiac muscles from type 2 diabetic patients undergoing CABG. However, the contractile and relaxation measurements reported in that study were much lower in magnitude when compared to values reported in other studies using human right atrial cardiac muscles[27, 28] and our study (Table 2). This may be related to tissue degradation in their samples due to prolonged loading with a fluorescence indicator, while our experimental measurements were obtained within 90 minutes after dissection.
The heart has the ability to increase its cardiac efficiency via intrinsic means, such as volume. Several studies reported that the Frank-Starling mechanism is maintained in patients with reduced EF[28, 30]. More recently, patients with preserved EF showed a preserved static (intrinsic to the heart) Frank-Starling mechanism, whereas the beat-to-beat dynamic (including the heart-arterial interaction) Frank-Starling mechanism was impaired in these patients. By increasing the length of our isolated cardiac muscles we mimicked the myocardial stretch and recorded a similar increase in force development in both our non-DM and DM groups. This indicates a preserved Frank-Starling mechanism in diabetic patients with preserved EF, and supports the concept that arterial stiffening might be more important for the observed impaired dynamic Frank-Starling mechanism during preserved EF than myocardial stiffening.
Impaired relaxation during physiological challenge
Although contractile function at rest was not altered by diabetes, the relaxation of the right atrial diabetic muscles was impaired over the entire range of myocardial stretch, and both the inotropic and lusitropic responses to β-adrenergic stimulation were completely absent in cardiac muscles from DM patients. A reduced but still responsive myocardium to β-adrenergic stimulation has been observed in many diabetic animal models[33, 34] and has been related to reduced expression levels of β1-adrenoreceptors. Surprisingly, cardiac muscles from our cohort of diabetic patients failed to respond to the β-adrenergic stimulation, even at very high (10-5 M) concentrations, which would indicate a lack of contractile reserve even in these patients with normal resting contractile function. In addition, our new data emphasizes that caution should be taken with translating animal data directly to the human situation. It would be easy to attribute this to the use of β-adrenoceptor blocking agents, however almost all patients, both the diabetic and the non-diabetic, were on β-blocker treatment (Table 1). Secondly, although the hemodynamic responses to dobutamine are reduced in diabetic patients they normally still do respond. Consequently the non-responsiveness to β-adrenergic stimulation in the isolated right atrial cardiac muscles in our study should reside within the myocardium. Thirdly, although a reduced expression of β1-adrenoreceptors has been reported in myocardial tissue from diabetic patients undergoing CABG in the absence of β-blockers, to the best of our knowledge expression of β1-adrenoreceptors has never been reported in human myocardial tissue from diabetic patients with preserved EF. Interestingly, we did not observe a statistically significant reduction in β1-adrenoreceptors expression levels (Figure 3F) in the cardiac tissue from our diabetic cohort. Therefore, we suggest that the reduced β-adrenergic inotropic and lusitropic responses in the diabetic myocardium from patients with preserved EF are related to alterations in downstream β-adrenergic signaling pathways. Phosphorylation of PLB is an important downstream target of β-adrenergic signaling and we observed a markedly reduced PLB protein expression in the diabetic myocardium. Indirectly this implies there is less PLB to be phosphorylated and therefore this could be the reason for the reduced β-adrenergic inotropic and lusitropic responses in the diabetic myocardium from patients with preserved EF. Alternatively, Daniels et al. suggested that reduced β-adrenergic responsiveness in diabetes is related to metabolic changes leading to impaired energy conversion, which becomes apparent during physiological challenge. Additionally, it was recently shown that although exercise limitations were similar between patients with reduced and preserved EF, significant differences occurred in their exercise-induced changes in systolic and diastolic properties, again reflecting their different underlying pathologies.
Underlying mechanism of impaired relaxation
The underlying mechanism of the impaired relaxation may be related to impaired Ca2+ cycling within the cardiomyocytes. In human diabetic myocardium from patients with reduced EF a decreased level of RyR2 mRNA was observed. In contrast, the human atrial myocardium from diabetic patients with preserved EF in our study showed no change in expression of the SR Ca2+ release channel RyR2, which is consistent with the preserved contractile function observed. Interestingly, in human non-diabetic and type 2 diabetic patients with preserved EF, it was reported that both SERCA2a and PLB expression were similar, and recently mRNA of SERCA was also shown to not be different between diabetic and non-diabetic spontaneously hypertensive rats, which is in contrast to our study showing an increased SERCA2a protein expression and a decrease in PLB protein expression. However, an altered mRNA level does not always equate to altered protein expression. Moreover, our observed changes in SERCA2a and PLB expression lead to an increase in the SERCA2a:PLB ratio in myocardial tissue of DM patients. From our data, which suggest accelerated SR Ca2+ uptake, it is tempting to speculate that the changes in protein density reflect a compensatory mechanism to attempt to normalize the impaired relaxation at rest. This is supported by the findings of Selby et al. who suggested that in myocardial muscles obtained from non-diabetic patients with preserved EF, the impaired relaxation is accompanied by a disproportionate increase in SR Ca2+ content due to an increase in SR Ca2+ uptake. Notably, they found that increased SR Ca2+ content did not translate into a stronger contraction. In addition, our results are supported by studies using rodent diabetic models that have reported an up-regulation of SERCA2a, a down-regulation of PLB and an improved contractile function following insulin treatment[19, 41]. These authors showed that expression of SERCA2a mRNA in cardiomyocytes is under control of insulin, associated with changes in SR-Ca2+ uptake and phosphorylation of Akt, and inhibited by phosphoinositide 3 (PI3)-kinase inhibitor wortmanin. This indicates that the underlying cellular mechanism for upregulation of SERCA2a could be mediated by the PI3-kinase-Akt-SERCA2a signaling cascade, suggesting that subtle changes in Ca2+ regulation, which promote diastolic dysfunction prior to overt systolic dysfunction, may be common to early stages of type 2 diabetes involving insulin resistance[19, 42]. Moreover, it was shown recently that elevated oxidative stress may induce oxidative modifications of SERCA2a that could contribute to abnormal function in high-sucrose fed rats mimicking the metabolic syndrome heart.
In the present study, DM patients had an increase in hyperglycemic markers (glucose and HbA1c), despite all being on hyperglycemic control medication (metformin and insulin), and therefore changes in the expression of calcium-handling proteins might still be due to altered glycemic control. These changes in Ca2+ regulation may over time increase the energy demands of the diabetic myocardium and have important ramifications for future diabetic myocardium remodeling, potentially further impairing relaxation and eventually leading to myocardial dysfunction. Therefore, the increased SERCA2A:PLB expression ratio may be compensatory and beneficial for relaxation at resting conditions, but once the myocardium is challenged, there is little reserve for an increase in Ca2+ cycling leading to the lack of response to β-adrenergic stimulation observed in our study. Alternatively, in rodent models, experimental diabetes changed the phosphorylation of the sarcomeric protein troponin I[44, 45] and also markedly shifted the myosin heavy chain (MHC) from the fast (V1) to the slow (V3) isoform[46, 47], although the later might be less important in humans as most MHC already is predominantly in the slow isoform. However, these studies indicate that myocardial relaxation can also be affected by alterations in regulatory myofilament proteins of the cardiac actomyosin system of which upon the effects of diabetes in humans are unknown.
A well-known underlying cause of diastolic dysfunction is increased myocardial fibrosis. The extracellular matrix remodeling plays an important role in cardiac fibrosis and the amount of extracellular collagen is caused by an imbalance between synthesis and degradation of collagen[49, 50] and formation of advanced glycation end-products. Cardiac fibrosis leads to increased myocardial stiffness, eventually resulting in both systolic and diastolic dysfunction. Increased fibrosis is commonly observed in diabetic animal models (see review), whereas reports in human cardiac tissue are conflicting[8, 49]. In our study, the elevated collagen deposition in the right atrium of diabetic patients is indicative of increased fibrosis. Alternatively, increased diastolic myocardial stiffness could result from an increased cardiomyocyte stiffness, which relates to the elasticity of the giant cytoskeletal protein titin and is determined by its isoform expression and/or posttranslational modification[53, 54]. Changes in isoform expression of titin have been observed in type 1 diabetic animal models[47, 55, 56]. Recently in a metabolic animal model hyperphosphorylation of titin contributed importantly to underlying diastolic dysfunction. However the specific role of titin regulating diastolic (dys) function, especially in type 2 diabetes in humans, is still not clear.
Due to the use and access to human tissue, there are a number of limitations to our study. CAD is known to be a co-morbidity and a specific causal factor for the transition from diastolic to systolic failure. As all our patients had CAD for inclusion into the study, our data were not compared to healthy human myocardium, so it is unclear if our findings would translate to patients with DM but without CAD. Non-transplanted donor heart tissue is the closest available “non-diseased’ human myocardial tissue, and our force values obtained in right atrial cardiac muscles from non-DM patients with CAD and preserved EF were similar to data from LV myocardial tissue of non-transplanted donor hearts, although caution should still be taken that the function of the “non-diseased” hearts might still be affected by the cause of death (such as accident trauma), the use of cardioplegic solutions and the variable elapsed time between removal of the heart and the dissection of cardiac muscles. Nevertheless, diabetic patients with CAD are an extensive cohort and are known to have double the risk of progressing to HF compared to non-diabetic CAD patients, and therefore our findings provide important novel and relevant knowledge to a clinically large and important patient group.
Another limitation is that differences in the ultrastructure and Ca2+ dynamics between the atria and ventricular myocardium exists , which need to be carefully considered when translating right atrial findings to the left ventricular myocardium or the whole heart. For instance it has been shown that atrial tissue expresses relatively more SERCA2a and less PLB compared to ventricular tissue. On the other hand, cardiac muscles obtained from right atrial appendages have been extensively used to study the function of human myocardium[9, 26–28].
In patients with CAD and preserved EF, the existence of type 2 diabetes resulted in impaired relaxation and increased fibrosis of the right atrium, with preserved myocardial contractile function. Our novel finding of increased expression of SERCA2a:PLB ratio suggests a compensatory mechanism to enhance relaxation and maintain the diastolic function at rest of the fibrotic diabetic atrial myocardium. We also demonstrate for the first time that human right atrial cardiac muscles from type 2 diabetic patients with preserved EF are unresponsive to β-adrenergic stimulation despite no change in expression of the β1-adrenoreceptor expression levels, suggesting impaired downstream β-adrenergic modulation and lack of contractile reserve. Our study provides novel knowledge on the underlying pathology of diastolic dysfunction in the diabetic myocardium.
Late ventricular filling velocity
Body mass index
Coronary artery bypass graft
Coronary artery disease
Cross sectional area
Minimum rate of relaxation
Maximum rate of contraction
Early ventricular deceleration time
Type 2 diabetes mellitus
Early ventricular myocardium relaxation velocity
Early ventricular filling velocity
Glyceraldehyde 3-phosphate dehydrogenase
Interventricular septal diameter diastole
Left atrial 2-dimensional diameter
Muscle length at which isometric developed force was maximal
Left ventricular end diastolic volume
Left ventricular end systolic volume
Left ventricular internal diameter diastole
Left ventricular internal diameter systole
Left ventricular posterior wall thickness end-diastole
Myosin heavy chain
Phosphate buffered saline
Right atrial appendages
50% relaxation time
Ryanodine receptor 2
Sodium dodecyl sulphate
Sarcoplasmic reticulum Ca2+ ATPase
Time constant of relaxation
Tris buffered saline
Time to peak force.
The authors thank the operating theatre staff of Dunedin Hospital, without whose help this study would not have been possible. This study was kindly supported by research grants from National Heart Foundation Taylor Charitable Trust (#1491), Otago Medical Research Foundation’s Laurenson Award (#LA 306) and Healthcare Otago Charitable Trust (#09335). SC was supported by a Tony Hocken Scholarship from the Department of Medicine - University of Otago.
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