Abstract
In recent decades, the scientific community has seen an increased interest in rigor and reproducibility. In 2017, concerns about methodological thoroughness and reporting practices were implicated as significant barriers to reproducibility within the preclinical cardiovascular literature, particularly in studies using animal research. The Langendorff, whole heart technique has proven to be an invaluable research tool, being modified in a myriad of ways to probe questions across the spectrum of physiological and pathophysiological functions of the heart. As a result, significant variability in the application of the Langendorff technique exists. This literature review quantifies the different methods employed in the implementation of the Langendorff technique and provides brief examples of how individual parametric differences can impact the outcomes and interpretation of studies. From 2017 to 2020, significant variability of animal models, anesthesia, cannulation time, perfusate composition, pH, and temperature demonstrate that the technique has diversified to meet new challenges and answer different scientific questions. The review also reveals which individual methods are most frequently reported, even if there is no explicit agreement upon which parameters should be reported. The analysis of methods related to the Langendorff technique suggests a framework for considering methodological approach when interpreting seemingly contradictory results, rather than concluding that results are irreproducible.
Keywords: electrophysiology, Langendorff, methods reporting, reproducibility
INTRODUCTION
In recent decades, the scientific community has seen an increased interest in rigor and reproducibility, as is evident by an increase in the number of studies investigating the perceived lack of scientific reproducibility (1). A precipitating event leading to the renewed interest in reproducibility can be traced back to the United States Food and Drug Administration’s withdrawal of 10 prescription drugs from the market between 1997 and 2000. These steps were taken after the drugs’ adverse effects in females became apparent, effects which were not detected in preclinical research nor clinical trials as a result of the male bias present in those studies (GAO-01–754) (2).In response to the historical male bias in scientific studies, the National Institutes of Health (NIH) Revitalization Act, PL 103-43 directed the NIH to establish guidelines for the inclusion of females in clinical research in 1993. In June 2015, the NIH further released notice NOT-OD-15–102, requiring consideration of sex as a biological variable in preclinical research funded by the agency.
Also contributing to the interest in scientific reproducibility, Bayer HealthCare and Amgen published reports in which they were only able to reproduce results from less than 30% of selected high-impact preclinical studies (3, 4). This added fuel to a “reproducibility crisis” narrative in both the scientific and public spheres. Since the release of these reports, there has been an increase in the number of popular editorials, commentaries, and books targeted to lay audiences to raise awareness (and sometimes stoke fear/outrage) among the general public regarding the impact of irreproducibility in federally funded biomedical research (5–7).
In 2017, our field was brought into the fold when “poor methodological rigor and [lack of] transparent reporting practices” were implicated as significant impediments to reproducibility within the preclinical cardiovascular literature (8). In this review, we summarize the state of methods reporting for the 5 years following the publication of NIH NOT-OD-15–102 as it relates specifically to the Langendorff technique, given its continued widespread use in preclinical cardiac research and our laboratory’s continued use of the technique for basic science investigations.
First performed in 1866 by Carl Ludwig and Elias Cyon, and modified into modern form in 1898 by Oskar Langendorff, the retrograde perfusion of the ex vivo heart has been instrumental in advancing our knowledge of cardiac physiology (9–13). In the past century, the Langendorff technique, including the perfusion systems and fluids paired with it, has been adapted for use in a wide variety of preclinical animal models (10, 14, 15). In this article, the evolution of experimental design(s) associated with the Langendorff technique and the potential impact of these variations to alter experimental outcomes are detailed and discussed. Although the review is highly focused on one particular technique that is also narrowly confined to only a few fields of scientific inquiry, the case study is illustrative of the lack of or evolution of unstated methods reporting consensus. The review also offers a handful of peer-reviewed example studies for why a particular variable may be worth reporting. Finally, a few thoughts are offered on how methods reporting could be improved by deliberate conversation.
METHODS
A systematic review of the scientific literature was performed on July 29, 2021. The search was conducted in PubMed Central (http://www.ncbi.nlm.nih.gov/pmc) using the search terms: (Isolated[All Fields] AND (“heart”[MeSH Terms] OR “heart”[All Fields])) AND (Retrograde[All Fields] AND (“perfusion”[MeSH Terms] OR “perfusion”[All Fields]))) OR Langendorff[All Fields] AND (“open access”[filter] AND (“2016/01/01”[PubDate]: “2020/12/31”[PubDate]). In other words, this expression searches for manuscripts that contain the following keywords: Isolated Heart and Retrograde Perfusion, Isolated Heart and Perfusion, Isolated Heart and Langendorff, Heart and Retrograde Perfusion, Heart and Perfusion, and Heart and Langendorff. The query identified 2,597 manuscripts.
Characteristics of Studies Included
This review only includes experimental studies that use the Langendorff technique for primary data collection. Exclusion criteria were as follows: manuscripts that were not primary research articles (i.e., editorials, reviews, case studies, etc.), manuscripts that only used Langendorff perfusion for the purpose of cell isolation, and manuscripts that used only working heart preparations. Following exclusions on the aforementioned principles, 443 manuscripts (n) were included in the analysis.
Data collection instrument.
The outcomes of the PubMed Central search were collected in a standardized data collection record that contained the following fields: PMCID, Journal Name, Animal Species, Animal Sex, Animal Age, Animal Weight, Organ Weight, Anesthesia Use (yes/no), Heparin Use (yes/no), Cannulation Time, Experimental Temperature, Perfusate Name, Perfusate pH, Perfusate Recirculation, Perfusate Composition Provided (yes/no), [NaCl], [NaHCO3], [NaH2PO4], [NaOH], [NaSO4], [Na2EDTA], [Na-Hexanoate], [KCl], [KH2PO4], [KHCO3], [MgSO4], [MgCl2], [d-glucose], [CaCl2], [H2PO4], [HEPES], [Pyruvate], [Na-Pyruvate], [EDTA], [Acetate], [Octanoic Acid], [Oleate], [Insulin], [Bovine Serum Albumin], [2,3-butanedione monoxime], [Blebbistatin], [Lactate], [Taurine].
The database of results has been uploaded to figshare.com and can be accessed with the unique Digital Object Identifier (DOI: https://doi.org/10.6084/m9.figshare.20137562).
RESULTS
Animal Model
An important consideration in preclinical research is the choice of experimental model. For research involving animal studies, factors to consider include utility as a research model, level of clinical translatability, cost, and maintenance. The choice of model extends beyond species to include the decision of genetic strain, sex, age, and weight.
Species.
Of the 443 manuscripts meeting inclusion criteria for this review, the majority of studies used rodent models for studying cardiac function with the Langendorff technique: 125 mouse, 252 rat, 38 rabbit, 15 guinea pig, 4 canine, 11 pig, 1 chicken, 1 hamster, 1 sheep, and 1 trout (Tables 1 and 2). Six manuscripts reported data from multiple animal species, which have all been independently quantified in the aforementioned list. Although larger mammalian species may serve as closer homologs to humans in certain regard, they often lack the utility found in smaller species such as rodents. This point is illustrated by the insight into genomic regulation of phenotype provided by the use of transgenic mouse models, despite the fact that murine models have substantial differences in cardiac ultrastructure, ion exchange, and protein expression relative to humans (16–19). For instance, calcium handling differs greatly across species; small rodents have an increased dependence on the sarco/endoplasmic reticulum Ca2+-ATPase for relaxation, as opposed to the cardiac sodium-calcium exchanger (NCX) (20–23). There are also appreciable differences in potassium channel expression and potassium current densities that result in heterogeneous repolarization patterns and action potential morphologies (24, 25). Specifically, in mouse and rat, the large transient outward potassium (K+) current (Ito) is predominantly responsible for rapid membrane repolarization, whereas in human, rabbit, canine, and guinea pig, the delayed rectifier K+-currents, IKs and IKr, are primarily responsible for membrane repolarization (24–26). Guinea pigs and pigs on the other hand do not functionally express Ito, which has been implicated as a major cause of early repolarization in diseases such as the Brugada syndrome (27–29). Thus, species differences can be important when studying intracellular calcium handling or repolarization. Given the preponderance of rodent studies in the field, the remainder of the review will mainly provide exemplars of how rodent-specific physiology is affected by choice of experimental technique.
Table 1.
Description of animal sex reporting broken down by animal species
| Animal Sex | Chicken | Dog | Guinea Pig | Hamster | Mouse | Pig | Rabbit | Rat | Sheep | Trout | Totals | % of Total |
|---|---|---|---|---|---|---|---|---|---|---|---|---|
| Male | 0 | 2 | 8 | 1 | 59 | 0 | 13 | 201 | 0 | 0 | 284 | 63.3 |
| Female | 0 | 0 | 4 | 0 | 4 | 0 | 4 | 11 | 0 | 0 | 23 | 5.1 |
| Both | 0 | 0 | 3 | 0 | 22 | 1 | 12 | 14 | 0 | 0 | 52 | 11.6 |
| Not provided | 1 | 2 | 0 | 0 | 40 | 10 | 9 | 26 | 1 | 1 | 90 | 20.0 |
| Totals | 1 | 4 | 15 | 1 | 125 | 11 | 38 | 252 | 1 | 1 | 449 | 100.0 |
Table 2.
Description of animal age and weight reporting broken down by animal species
| Chicken | Dog | Guinea Pig | Hamster | Mouse | Pig | Rabbit | Rat | Sheep | Trout | Totals | % | |
|---|---|---|---|---|---|---|---|---|---|---|---|---|
| Age | 0 | 3 | 10 | 1 | 5 | 8 | 28 | 126 | 1 | 1 | 183 | 40.8 |
| Weight | 0 | 0 | 2 | 0 | 74 | 0 | 1 | 37 | 0 | 0 | 114 | 25.4 |
| Both | 0 | 1 | 1 | 0 | 12 | 0 | 4 | 70 | 0 | 0 | 88 | 19.6 |
| Not provided | 1 | 0 | 2 | 0 | 34 | 3 | 5 | 19 | 0 | 0 | 64 | 14.2 |
| Totals | 1 | 4 | 15 | 1 | 125 | 11 | 38 | 252 | 1 | 1 | 449 | 100.0 |
Genetic strain.
The genetic strain of animals was not always readily apparent in the manuscripts analyzed. In many cases, the strain was determined by following several citations to the original studies describing species strain background. In these cases, it was not always clear whether or not the transgenic mouse had been maintained on the original background or bred into a new strain.
Within a given species, differences in experimental outcomes have been linked to variation among genetic strains (30, 31). For instance, Maudsley nonreactive rats display a faster decline in norepinephrine levels in their heart than reactive strains, hinting at a strain-specific determinant to norepinephrine metabolism, which is important given the frequent use of isoproterenol, the isopropylamine analog of epinephrine, in Langendorff preparations (32). Jelinek et al. (31) further demonstrated that genetic background is the principal determinant of ventricular arrhythmia susceptibility following ß-adrenergic stimulation in mice. Furthermore, Obergassel et al. (33) used Langendorff-perfused mouse hearts to elegantly demonstrate that genetic strain has a strong role in atrial electrophysiological parameters including action potential duration, interatrial activation times, and atrial effective refractory periods.
These variances in outcomes extend to environmental factors surrounding how the species are housed and cared for leading up to experiments. For example, the development of myocardial lesions in response to a high-fat diet is mouse strain-specific, suggesting that studies within the same species may not be directly comparable without consideration of genetic strain (34). This becomes particularly important with varying ages and diets of the study animals.
Sex.
In the manuscripts reviewed, 63.3% (n = 284) included only male animals in their studies, 5.1% (n = 23) included only females, 11.6% (n = 52) included both males and females, whereas 20.0% (n = 90) did not report the sex of the animals used (Table 1).
Sex as a biological variable is well known to affect cardiac function in both physiological and pathophysiological states. Recently, the American Journal of Physiology - Heart and Circulatory Physiology editorial staff published an article outlining the importance of and reinforcing the journal’s commitment to, the inclusion of sex as a biological variable (35). Numerous recent reports provide further evidence for the importance of sex-specific signaling leading to differences in electrophysiological, mechanical, and metabolic function of the heart (36–41). For example, different levels of endogenous estrogen receptor signaling are known to lead to sex-based differences in genomic expression of the α subunit of the L-type Ca2+ channel and NCX1, expression and activity of the Ryanodine receptor (RyR2), ejection fraction and strength of contraction, and rate of repolarization (QT interval) (42–51). Although intrinsic neurohumoral modification of cardiac function is intentionally reduced by organ isolation in the Langendorff technique, it is unlikely that the acute removal of sex hormone signaling will completely revert structural and functional changes consequent of a lifetime of differences in endogenous sex-hormone signaling. Other sex-dependent differences without a clear underlying etiology include age-related changes. For instance, left ventricular (LV) systolic function, as measured by global longitudinal strain, is significantly higher in old versus young male mice but relatively preserved in females (52). Similarly, although both male and female mice have changes in aortic structure with age, only the males have concomitant changes in aortic function (52). Taken together, these studies suggest that care should be taken in considering the role of sex in studies using the Langendorff technique, particularly when used to analyze the effects of Ca2+ regulation, sex hormone signaling, and cardiac ultrastructural remodeling. Of note, there is a reason for growing optimism as a recent manuscript by Woitowich et al. (53) showed a significant increase in sex-specific reporting in general biology studies between 2009 and 2019.
Age.
In the manuscripts reviewed, 40.8% (n = 183) quantitatively reported animal age at the time of the experiment (Table 2). However, the majority of studies qualitatively reported using “adult” or “mature” animals. A recent survey among scientists found that “adult” was loosely defined as anywhere between 6 and 20 wk in laboratory rodents (54). These manuscripts were classified as “data not specified” for the animal age field because of the ambiguity associated with the qualitative descriptor. One factor likely contributing to the underreporting of animal age may be linked to age tracking by commercial vendors. For example, when our group requests the vendor to provide date of births for guinea pigs, the dates for all animals are identical in each shipment, which is possible, but unlikely when repeated weekly, and year after year.
The effect of age on cardiac structure and function has been examined extensively (55–60). From birth to adolescence, there are numerous and substantial changes to the heart. Structurally, cardiomyocytes increase in volume (hypertrophy), gaining their distinct rectangular shape, and proteins such as connexin43 and the voltage-gated sodium channel (Nav1.5) redistribute from a uniform sarcolemmal distribution at birth to a polarized distribution clustering at intercalated disks by the time of sexual maturity (55–57). Functionally, neonatal hearts demonstrate increased heart rate, faster atrioventricular conduction, shortened action potential duration, and decreased ventricular refractoriness relative to their adult counterparts in Langendorff-perfused Sprague–Dawley rats (61). With advancing age, there is an increase in fibroblast infiltration, reduction in vascular integrity, and loss of metabolic flexibility (62–64). These changes result in lower diastolic and mean arterial pressures, reduced isovolumetric relaxation time/diastolic time intervals, and elevated left ventricular end-diastolic and end-systolic volumes (52). Advanced age is a known risk factor for cardiac disease (59), and as the geriatric population of the world continues to grow, there is an increased need to refine our understanding of age on cardiac function (65–67).
While it is unlikely that age discrepancies of a few days to a week will substantially alter functional outcomes in adult animals, even nuanced differences in age could have a dramatic impact during early life (56, 57). For instance, between birth to 10 wk postnatal, there are rapid and significant changes in the orientation of transmembrane proteins on the cardiomyocyte, the innervation of the myocardium, and the metabolic biochemistry of the heart (55–57, 68, 69). In the rat, there is a 6.2-fold increase in LV weight and a 69% increase in septum secundum length and width within the first 11-days postnatal, and myocyte cell volume increases up to 25-fold in the first 2 months of life (70–72). In humans and rodents alike, the innervation of the heart is relatively immature at birth and continues developing during childhood and early adolescence (68, 73–75). Regarding energy metabolism, there is a switch from preferential carbohydrate dependence to fatty acid oxidation within the first 30-days postnatal in rodents; in humans, this switch occurs before birth (76–78). There are also significant increases in creatinine and phosphocreatine concentrations within the first month of life in dogs, rabbits, guinea pigs, mice, and rats (78, 79). Furthermore, geriatric aging is known to underlie substantial changes in cardiac structure and function. For instance, there is an increase in fibrotic infiltration, a decrease in vascular integrity, and dehiscence of the intercalated disk that occurs with geriatric aging (62, 63, 80). In the context of the Langendorff technique, Waldeyer et al. (81) demonstrated significant changes in action potential morphology and epicardial conduction velocity associated with aging in wild-type Langendorff perfused mouse hearts.
Weight.
Animal weight was quantified and reported in 25.4% (n = 114) of manuscripts reviewed. Table 2 shows reporting trends for the most frequently used animal models. Laboratory animal weight is a highly variable parameter, and one study noted that it is not uncommon for animals to arrive with weights 10% lower than noted by the vendor at the time of shipment (82). This weight difference may be explained by scale differences and/or weight loss during shipment. In particular with retired breeder guinea pigs, a geriatric model, animal weight can vary by upward of 5% daily depending on eating and hydration habits, defecation and urination differences, and whether fluids have been administered.
Changes in weight, particularly for prey species, are an indicator of emotional and physical stress (83). This becomes important when studying cardiac function, as both acute and chronic stress impact cardiovascular dynamics. For instance, the neurocardiac axis provides a framework for how acute emotional stress, as may occur with animal transportation, is linked with acute cardiovascular events. Sympathetic hyperactivation induces cytokine release and a proinflammatory state, leading to endothelial activation and potentially thrombosis in predisposed animals (84). Alternatively, chronic stress has been shown to impair baroreflex, chemoreflex, and heart rate variability, potentially hindering the study of coronary pressure and intrinsic heart rate (85).
Aside from obesity studies, there is no suggestion that small fluctuations in laboratory animal body weight, not associated with stress, will significantly alter experimental outcomes. However, body weight may give insight into organ weight, more specifically heart weight. This is of importance as higher cardiac/total body weight ratios have been linked with increasing likelihood of cardiac lesions and worse cardiovascular outcomes (86). This phenomenon was reviewed in a recent manuscript by Patel et al. (87), summarizing the effects of epicardial adipose tissue on cardiac function. As such, many studies continue to report organ weight (including heart weight) to body weight ratios, and therefore a general knowledge of animal weight ranges would be beneficial for cross-study comparisons (88, 89). In this regard, 27.3% (n = 121) of manuscripts specifically reported heart weights (31 manuscripts reported heart weight in grams only, whereas the other 90 reported heart weight-to-body weight or heart weight-to-tibia length ratios). It is also worth noting that “control” laboratory rodents are metabolically morbid compared with their undomesticated counterparts, presenting with a higher incidence of obesity, sedentary lifestyle, and insulin resistance (90).
In total, 19.6% (n = 88) of manuscripts reported both age and weight of the animal at the time of the experiment (Table 2). Often either age or weight is documented, but infrequently both, when characterizing laboratory animals. Although there are barriers to age tracking in laboratory animals, particularly those purchased from commercial vendors, a better understanding of specific age ranges would help inform the applicability of the research outcomes.
Anesthetic Agent
Over the past several decades, numerous studies have shown that sedatives and anesthetics commonly used in animal research produce a wide range of off-target effects with significant impacts on cardiovascular function (91–96). Below, we briefly comment on some of the known cardiac effects of pentobarbital, ketamine, and isoflurane—the three most commonly reported anesthetics in the manuscripts reviewed (Table 3).
Table 3.
Description of commonly administered anesthetics broken down by animal species distribution
| Chicken | Dog | Guinea Pig | Hamster | Mouse | Pig | Rabbit | Rat | Sheep | Trout | Totals | % | |
|---|---|---|---|---|---|---|---|---|---|---|---|---|
| Ketamine | 0 | 0 | 0 | 0 | 11 | 4 | 18 | 38 | 0 | 0 | 71 | 15.8 |
| Pentobarbital | 0 | 2 | 8 | 1 | 42 | 0 | 11 | 89 | 0 | 0 | 153 | 34.1 |
| Isoflurane | 0 | 1 | 5 | 0 | 18 | 0 | 3 | 22 | 0 | 0 | 49 | 10.9 |
| Thiopental | 0 | 0 | 0 | 0 | 0 | 0 | 1 | 17 | 0 | 0 | 18 | 4.0 |
| Tribromoethanol | 0 | 0 | 0 | 0 | 8 | 0 | 0 | 0 | 0 | 0 | 8 | 1.8 |
| Chloral hydrate | 0 | 0 | 0 | 0 | 2 | 0 | 0 | 11 | 0 | 0 | 13 | 2.9 |
| Cervical dislocation/Decapitation | 1 | 0 | 1 | 0 | 10 | 0 | 1 | 8 | 0 | 1 | 22 | 4.9 |
| Other | 0 | 0 | 0 | 0 | 3 | 1 | 0 | 16 | 0 | 0 | 20 | 4.4 |
| Not specified | 0 | 1 | 1 | 0 | 31 | 6 | 4 | 51 | 1 | 0 | 95 | 21.2 |
| Totals | 1 | 4 | 15 | 1 | 125 | 11 | 38 | 252 | 1 | 1 | 449 | 100.00 |
Pentobarbital.
Of the manuscripts reviewed, 34.0% (n = 153) used pentobarbital as their primary anesthetic agent. Pentobarbital is a short-acting barbiturate that agonizes GABAA receptors, in turn, hyperpolarizing neurons within the central nervous system leading to dose-dependent sedation and depression of the sensory cortex (91). Several studies have explored the effects of pentobarbital on cardiac function in ex vivo heart preparations (92, 93). Segal et al. (92) demonstrated that in male Sabra rats, use of pentobarbital as the primary anesthetic, before cardioectomy, decreased the sensitivity of electrical and mechanical function to changes in extracellular calcium concentration (range = 0.5–2.5 mM) and thyroid hormone exposure (1 µM 3,5,3'-triiodothyronine for 0–40 min incubation). Jiang et al. (93) showed that pentobarbital (50 mg/kg) significantly decreased heart rate, left ventricular systolic pressure (LVSP), and the maximum rate of rise in left ventricular pressure (+dP/dt) in isolated Sprague–Dawley rat hearts when compared with nonanesthetized control rat hearts. The authors suggest that their results are due to a disruption of physiological calcium handling by pentobarbital. Taken together, these reports indicate that the use of pentobarbital may complicate comparisons of calcium handling and mechanical function between studies using other anesthetics.
Ketamine.
Ketamine was the primary anesthetic agent used in 15.8% (n = 71) of manuscripts in our analysis (Table 3). Ketamine is a noncompetitive N-methyl-D-aspartate (NMDA) receptor antagonist. NMDA inhibition in the central nervous system results in depressed sensation in the sensory association area of the cortex, the limbic system, and the thalamus (94, 95). Neuronal inhibition in these areas of the central nervous system results in an inability to receive and process sensory information, such as pain (94, 95). In addition, ketamine results in an analgesic effect via inhibition of nitric oxide (NO) synthase (96). An important off-target consequence of NO inhibition, relevant to the Langendorff technique, is that NO is involved in intrinsic vasoregulation (97). Similar to pentobarbital, Jiang et al. (93) reported that ketamine (100 mg/kg) significantly decreases heart rate, LVSP, and +dP/dt in isolated Sprague–Dawley rat hearts when compared with nonanesthetized control rat hearts. Furthermore, Sloan et al. (98) showed that ketamine protects against ischemia-reperfusion injury in a dose-dependent manner. Together, these reports suggest that the use of ketamine as an anesthetic agent may complicate broad interpretation of experiments in which intrinsic vasoregulation is important, or in studies investigating ischemia-reperfusion injury.
Isoflurane.
Of the manuscripts reviewed, 10.9% (n = 49) used isoflurane as their primary anesthetic agent (Table 3). Isoflurane, first discovered in 1965, is a methyl ethyl ether that is widely used for anesthetic purposes in clinical and preclinical studies alike (99). Unlike the aforementioned anesthetics, isoflurane is a volatile gas that is inhaled rather than injected, often in an induction chamber, or using forced ventilation with oxygen. Although the precise mechanism of action with isoflurane remains unknown, the compound produces a generalized, reversible depression of the central nervous system (100). Recent studies have demonstrated that isoflurane pharmacologically preconditions the mitochondria against ischemia-reperfusion injury by priming mitochondrial KATP channels via protein kinase-C signaling pathways, resulting in a blunted ischemia-reperfusion injury (101). Isoflurane has also been shown to attenuate reactive oxygen species produced by mitochondrial complex I and complex II substrates (102). Together, these reports suggest that isoflurane may uniquely affect mitochondrial energetics relative to injected anesthetics, particularly in the context of ischemia-reperfusion injury.
The changes in cardiac physiology accompanying the use of pentobarbital, ketamine, and isoflurane demonstrate that the choice of anesthetic could impact data interpretation and study conclusions. Of concern, 21.2% (n = 95) of manuscripts reviewed did not include details on anesthesia in their methods—creating a potential source for ambiguity in the interpretation and assimilation with related literature.
Heparin
Of the manuscripts reviewed, 53.3% (n = 236) reported the injection of heparin before euthanasia; reported doses ranged from 1 U/kg to 5,000 U/kg. Furthermore, 2.0% (n = 9) of manuscripts specifically stated they did not use heparin before euthanasia, and the remaining 44.7% (n = 198) manuscripts did not specifically state whether heparin was or was not administered. Numerous studies have demonstrated the effect of heparin on cardiovascular function in laboratory animals. Specifically, heparin has been suggested to increase breakdown of vascular endothelial glycocalyx in rat models of ex vivo lung perfusion and to augment the vasopressor effect of protamine in conscious dogs (103, 104). In neither instance were the groups studying the direct effect of heparin on the heart, but their combined results suggest that heparin may alter vascular endothelial function, perhaps leading to differences in coronary artery function in Langendorff-perfused hearts. Though, more detailed studies are needed to positively determine the effect, if any, heparin administration has on ex vivo cardiac function.
Cannulation Time
Of the manuscripts reviewed, only 2.5% (n = 11) quantified the time elapsed from excision to cannulation of the isolated heart, with times ranging from <30 s up to 4 min. Most manuscripts addressed cannulation time with a qualitative statement to the effect of, “the heart was quickly excised and mounted on a Langendorff apparatus.” To date, to our knowledge, no studies have directly examined the relationship between the duration of precannulation ischemia time (i.e., time from cardioectomy to cannulation and restoration of perfusion) and subsequent cardiac function.
An evaluation of the ischemia preconditioning literature may offer insights into how precannulation ischemia can influence cardiac function in hearts studied with the Langendorff technique. First described in 1986, ischemic preconditioning is an endogenous protective mechanism in which early periods of transient ischemia condition the heart to better withstand a subsequent ischemic insult and thereby provide protection against the threat of prolonged ischemia (105). The effect has been confirmed in all species studied, but the precise mechanism(s) by which preconditioning confers cardioprotection is an active area of research. What is known though is that the degree of cardioprotection is directly related to the duration of ischemic preconditioning (106).
In studies using the Langendorff technique, the time to cannulation is effectively an ischemic preconditioning period. Unintended consequences of precannulation ischemic conditioning are not limited to confounding results in ischemia or ischemia-reperfusion studies. For instance, one known consequence of preconditioning is increased activation of nitric oxide (NO) synthase and subsequent NO generation, which is known to have a vasodilatory effect within the heart (97, 107). The role of NO in vasospasm, as it relates to angina and ischemia, is also an area of significant research that might be impacted by precannulation ischemia (108). Furthermore, NO can modulate voltage-gated sodium channel conductance in cardiomyocytes by cyclic GMP and cyclic AMP pathways, highlighting a third direct role of NO on cardiac electrophysiology (109). As such, NO levels can impact the outcome of hemodynamic (110, 111) and electrophysiological (112, 113) studies performed using the Langendorff technique.
Recent guidelines by Bøtker et al. (14) recommend a cannulation time of <3 min for all hearts mounted with the Langendorff technique. Establishing an upper cannulation time limit is a complex task as extrapolating the necessary ischemic duration to induce preconditioning is difficult to ascertain from previous manuscripts given the wide range of reported times, with estimates spanning from 20 s to 15 min (114, 115). Given the functional effects of different anesthetics (see subsection “Anesthetic Agent”) and the sex-dependent differences in response to ischemia (116–118), it is foreseeable that establishing an upper limit to cannulation time will require multiple considerations and approaches. Increasing the accuracy of reporting cannulation times may therefore provide metadata that can inform future research in this area.
Circadian Considerations
Although the time of surgery relative to the circadian cycle of animals was not noted in the manuscripts evaluated here, it may become a parameter of interest for a few reasons. First, the circadian cycles of activity are not consistent between species (119). For instance, humans are diurnal, guinea pigs are crepuscular, with activity mostly at dawn and dusk with rest periods in between and mice, rats, and hamsters for example are nocturnal (120). Performing experiments during the daytime, particularly if the animal facilities’ light/dark cycles are tied to the environmental day/night cycle, may yield results in these rodents that are more pertinent during human periods of inactivity (aka sleep), as has been well described in the oncology literature (121). Second, circadian mechanisms have been shown to govern cardiovascular function and arrhythmia susceptibility in mammals (122, 123). At the cellular level, outward potassium channels have been shown to display circadian variation, likely through their interaction with the KV channel-interacting protein 2 (KChIP2) (122). As interest in chronobiology increases, with the goal of optimizing therapies or identifying the circadian rhythms that increase the risk of death, knowing when an experiment was performed is an important consideration for improving rigor and reproducibility.
Perfusate
Composition.
In the manuscripts reviewed, 66.1% (n = 293) reportedly used a Krebs–Henseleit (KH) or “modified KH” solution, and 18.5% (n = 82) used a “Tyrode” or “modified Tyrode” solution (Fig. 1). The remaining manuscripts used a Krebs–Ringer solution (n = 10), blood supplemented perfusate solution or blood (n = 5), Ringer-Locke solution (n = 1), generically named “buffer/perfusate solution” (n = 23), or provided no details for their solution composition (n = 29). In this review, modified versions of KH or Tyrode are combined for analysis of KH solution or Tyrode solution composition, respectively. Of the 293 manuscripts using the KH nomenclature, 59 (20%) did not provide details of the solution composition. Of the remaining 234 KH solutions, there were 183 (75%) distinct perfusate compositions. Despite these composition variances, all are referenced by the same name. Similarly, of the 82 manuscripts using the Tyrode nomenclature, 12 (15%) did not describe the solution composition. In the remaining 70 manuscripts, there were 61 (87%) distinct perfusate compositions referenced by the same name. To demonstrate the variability existing within and between KH and Tyrode solutions, the distribution of sodium, potassium, calcium, magnesium, glucose, bicarbonate, and HEPES concentrations for all reported KH and Tyrode solutions are plotted in Fig. 2. These particular components were graphed because they are commonly included in all solutions. The graphs demonstrate substantial variation between KH and Tyrode solutions, but also within KH and Tyrode solutions.
Figure 1.
Breakdown of perfusates used by naming convention.
Figure 2.

Violin plots of components commonly included in KH and Tyrode solutions. These components were selected for display based on their nearly ubiquitous appearance in perfusates reviewed. It is worth noting, that 59 manuscripts using “KH” and 12 manuscripts using “Tyrode” provided no details on perfusate composition and thus are not included in these violin plots. KH, Krebs–Henseleit.
Although the Langendorff technique has been adapted to answer a variety of experimental questions since its inception, the basic principles behind the technique have not changed in the past 125 years. However, the perfusion fluids paired with the Langendorff technique have evolved substantially. Despite the multitude of perfusate compositions existing in the current literature, naming conventions are such that nearly all perfusates are named a KH, Tyrode, or a modified solution. This is notable considering that neither the KH solution nor Tyrode solution were conceived for maintenance of ex vivo cardiac function.
For example, Maurice Vejux Tyrode, a pharmacologist at Harvard Medical School, published his research investigating the mode of action of purgative salts on the isolated rabbit intestine in 1910 (124). Tyrode’s solution was born out of necessity when he found that the perfusates previously described by Ringer, Locke, Hedon, and Adler all failed to viably sustain the perfused intestine (124). The KH solution, first published in 1932, was developed by Hans Krebs and his medical student Kurt Henseleit as a synthetic medium intended to approximate the composition of blood plasma to facilitate the study of urea formation in liver slices (125, 126). Since their inception, both solutions have been modified component by component to suit a myriad of experimental needs without a concurrent change in nomenclature to reflect these modifications (127).
An appreciation that altering perfusate ionic composition affects cardiac function dates back to the early 1880s when Ringer reported the essential nature of calcium in creating cardiac contractions (128–134). Since Julius Bernstein’s introduction of the “Membrane Theory of Electrical Potentials” in 1902, a substantial amount of work has been devoted to understanding how deviations in physiochemical gradients alter bioelectric events (135). During the 20th century, work by numerous biophysicists, physiologists, and physicians established our understanding of electrophysiology of excitable tissues, mechanical properties of contractile tissues, and metabolic function in living cells; in each case demonstrating the ability for changes in ionic gradients to influence cellular function (125, 126, 136–142). In recent years, studies investigating the effect of ionic control of cardiac function demonstrate that relatively modest changes in perfusate potassium, sodium, and calcium ionic concentrations have a profound effect on cardiac function under both physiological and pathophysiological conditions (143–151).
Although the traditional naming conventions lend themselves to preserving the names of scientists that have contributed seminal findings, the convention limits communication of the actual fluid compositions used in ex vivo isolated heart preparations. To eliminate ambiguity from methods reporting, the scientific community could shift to defining their solutions by components and concentrations as opposed to historical naming conventions alone.
pH.
In the manuscripts reviewed, 55.6% (n = 246) of studies specifically included information regarding the final pH of their solution, though <5% of manuscripts specified how the solution pH was equilibrated (e.g., titration of HCl, NaOH, or CO2). The latter is noteworthy considering that equilibration will change the total ion concentration of several solution components, potentially altering cardiac function (see Composition).
As early as 1880, the effect of pH on cardiac function was recognized when Walter H. Gaskell demonstrated that decreasing extracellular pH had a negative inotropic effect on isolated frog hearts (152). In the subsequent 139 years, many studies have determined the mechanisms by which acidosis, both intracellular and extracellular, modifies cardiac function (153–159). For instance, decreased pH has a significantly negative inotropic effect on excitation-contraction coupling pathways (160). Acidosis results in reduced transmembrane calcium current, calcium release from the sarcoplasmic reticulum, sensitivity of the contractile myofilaments to calcium, calcium uptake by SERCA2a, O2 consumption, and in turn, decreased metabolism and levels of high-energy transfer molecules such as phosphocreatine (155, 158). Acidosis is also known to decrease heart rate, increase the PR interval, and prolong the AV node refractory period (156, 161, 162). Conversely, alkalosis is associated with decreased T-wave amplitude and decreased pacing threshold (163). Increasing pH has also been identified as mediating interaction between the α1-adrenergic receptors and insulin receptor family in cardiomyocytes (164). In addition to the absolute value of pH, the choice of the buffer will also affect Langendorff perfused hearts. Specifically, exclusion of bicarbonate in HEPES-buffered solutions changes kinetics of the Na+-HCO3− symporter, which has a direct role, via HCO3− transport across the membrane, and an indirect role, via changing local sodium gradients and thus influencing the Na+-H+ transporter, in regulating intracellular pH in the heart (165–169). Furthermore, tuning pH is often achieved by adding NaOH; this additional sodium may affect Na+/K+-ATPase pumps, Na+ gradient, and other Na+-dependent ion channels within cardiomyocytes (170). Because of the multitude of transporters and ion channels that are dependent on not only the absolute hydrogen concentration but also the components that come together to achieve a certain pH, precisely documenting these during perfusion may allow a greater understanding of cardiomyocyte function and offer insights into heterogeneous outcomes.
Temperature.
In the literature reviewed, 75.2% (n = 333) of studies reported perfusing hearts at physiological temperature (37°C ± 2°C), 2.9% (n = 13) at below physiological temperature (ranging from 4°C to 35°C), and 21.9% (n = 97) did not specify the temperature at which the heart was maintained. Although the majority of studies were performed at, or near, physiological temperatures, the details surrounding temperature control were often absent. Of the manuscripts analyzed, 27.1% (n = 120) stated that excised hearts were rinsed in “ice cold” perfusate, one manuscript stated that the heart was rinsed in perfusate maintained at 37°C, and in the remaining manuscripts it was difficult to ascertain whether or not freshly excised hearts were rinsed in ice-cold perfusate, room temperature perfusate, or physiological temperature perfusate before cannulation, or no perfusate at all. It was also often unclear whether epicardial temperature was maintained consistent with coronary temperature by way of a heated humidity chamber or superfused in a heated bath or left free hanging at room temperature. Finally, 18 manuscripts specifically stated they recirculated perfusate, 20 manuscripts specifically stated they did not recirculate perfusate, and in the remaining 405 manuscripts it was unclear whether or not perfusates were perfused in a single pass system, where perfusate passes through the heart and is siphoned off as effluent waste, or a closed system where the effluent is collected and recirculated again through the heart. Recirculation is often used for studies involving expensive reagents, but care should be exercised to ensure that the technique does not substantively create conditions of physiologically relevant metabolite waste accumulation and pH imbalance. One way to address confounding variables introduced by recirculation could be the inclusion of open and recirculated vehicle control studies, if feasible.
At hypo- and hyperthermic temperatures, there are substantial changes in channel kinetics, ion flow, pH, and molecular processes (171–174). Both elastic and viscous components of cardiac muscle mechanics, the latter more so, increase with temperature (175) and may impact studies of hemodynamics with the Langendorff technique. Membrane potential, conduction velocity, and action potential magnitude are proportional to temperature, whereas action potential duration is inversely related to temperature (176, 177). One example of a temperature:variable relationship that is not bidirectional is from Vostarek et al., who observed a significant decrease in the amplitude of calcium transients with increasing temperatures from 37°C to 40°C but found them unchanged when decreasing temperatures from 37°C to 34°C (178). Of note, hyperthermic temperatures produce a significant increase in the rate of calcium release from the sarcoplasmic reticulum (179). While controlling endocardial, epicardial, and coronary temperature simultaneously and uniformly is a complex task, including temperature settings in methods reporting is recommended.
The Citation Trail and Paywalls
While relying on citations to fully describe methods is an efficient way to keep the total word count below publication limits, it can lead to ambiguity, confusion, and/or inaccuracy. This is particularly the case when a text states “methods as previously reported” with modifications or deviations that are not clearly enumerated. Reliance on “methods as previously reported” is particularly troublesome when the citing and cited manuscripts include fundamental differences in approach, such as the utilization of different animal models. For instance, one manuscript using male Wistar rats states, “Ischemia/reperfusion was studied ex vivo according to the Langendorff model, with minor modifications (citation).” The paper cited referred to a manuscript in which Langendorff-heart perfusion was performed in a rabbit model. Generalizations such as these create ambiguity regarding anesthesia dosing, coronary flow rate or pressure, isovolumetric balloon size, etc., as it is unlikely that such parameters will remain constant when switching from a rabbit model to a rat model or vice versa.
A second limitation of relying on citations for methods reporting is the matter of access. With the recognition of the need for increased transparency and data sharing to improve reproducibility in science, open access journals are gaining in popularity. As we limited our review to open access manuscripts indexed in PubMed Central, it is worth noting that finding “methods as previously described” occasionally required looking outside of the open access literature. Citing previous methods in manuscripts that are not publicly available undermines the spirit of open access. To mitigate this, numerous journals are now making manuscripts available after some period of time, but this does not address the often acute need to understand a recently published manuscript. Hopefully, this review demonstrates that nuanced methodological details may be important in interpreting the results of a study and are a critical component of a rigorous and impactful scientific manuscript. One suggestion could be the creation of open access methodological reporting repositories that are maintained and updated by the authors/laboratory. Alternatively, just as abstracts are open access and indexed by PubMed, journals could consider making methods open access for studies that use frequently used methods.
Strategies for Improving Transparency in Experimental Design
In the past decade, numerous manuscripts have provided guidance for improving rigor and reproducibility in multiple facets of preclinical cardiology (35, 180–183). While each of the aforementioned guidelines dives into a specific realm of preclinical cardiology, the narrative arc can grossly be distilled into the need for more transparent and standardized reporting practices; which should not be confounded with the need for strict standardization in experimental design that would have the potential to limit creativity and scientific exploration.
This manuscript adds to this narrative by detailing the wide range of methods associated with the Langendorff technique and advocating for more thorough methods reporting. While these assertions are based solely on the authors’ interpretation of the current state of the field, we suggest the inclusion of “methods tables” in manuscripts when using the Langendorff technique for primary data collection, with the hope that inclusion of “methods tables” can be adopted by journals and archived in an open access repository to inform future study design. Such a methods table could be established by a consensus report generated by a group of interested scientists, and include information on animal species, sex, age (when reliably attainable through vendors or bred in-house), and weight at a minimum. Furthermore, a “surgical considerations” table could be included that outlines the use and dosage of heparin (or lack thereof), the surgical anesthetic administered, any provided analgesic, the use of chilled/room temperature/or warm buffer for washing the excised heart, and total time to cannulation. Finally, a table containing information on perfusate composition and experimental agent(s) (drugs, peptides, etc.) could also be provided. One advantage of standardizing methods reporting in tables would be to reduce the creative lengths some go to avoid “self-plagiarism” in the methods. While well-intentioned, the continuous rewriting of methods can introduce copy errors. On the other hand, facilitating methods reporting with a table could also increase the likelihood that a critical change introduced into the experiment might not be noted if the writer is not forced to critically evaluate the methods section for each manuscript.
Tables could also establish a minimum information reporting practice for general Langendorff design, but there will always be a need for additional methods reporting for specific applications of the Langendorff technique such as optical mapping, left ventricular pressure recordings, ischemia-reperfusion protocols, etc., all of which may not be conducive to a tabular design. In these instances, we might suggest adding detailed experimental protocols to the supplemental materials that provide the reader with enough detail to not only understand the experiment but also replicate the experimental design precisely if so desired.
In all cases, if we share a joint goal of improving rigor and reproducibility, journals and reviewers alike should be cognizant of methods reporting during the manuscript review process and ensure inclusion of sufficient detail for each study. We appreciate that tables take up more physical space on the page relative to inline text and that the adoption of tables by journals may not be currently realistic. Instead, the aforementioned “open access methods” may be a first reasonable step to ensuring methods are freely available to all.
Limitations of This Review
Our data provide only a recent snapshot of the Langendorff literature from 2017 to 2020, whereas a nondate constrained search of (Isolated[All Fields] AND (“heart”[MeSH Terms] OR “heart”[All Fields])) AND (Retrograde[All Fields] AND (“perfusion”[MeSH Terms] OR “perfusion”[All Fields]))) OR Langendorff[All Fields]) in PubMed and PubMed Central returns nearly 15,000 results spanning more than one century. As such, it must be noted that while our results can provide a glimpse into the recent past, they cannot describe the evolution of methods reporting as it relates to the Langendorff technique.
Conclusions
Over one and a half centuries have passed since Ludwig and Cyon first published the technique of retrograde perfusion in ex vivo hearts. In the meantime, researchers have extensively used, and continue to use, the Langendorff technique for investigating the electrical, mechanical, and metabolic function of the heart. The Langendorff technique has been modified in a multitude of ways to probe questions across the spectrum of physiological and pathophysiological functions of the heart. As such, it would be inauspicious to review, in detail, all aspects of methods used for data collection in Langendorff prepared hearts. Instead, we described a subset of the experimental design that is conserved and most commonly documented in methods sections across Langendorff studies.
Numerous common areas of biological and experimental variation were detailed for consideration related to the Langendorff whole heart preparation, including animal models, anesthesia, cannulation time, perfusate composition, pH, and temperature. For each methodological variable, reporting practices were heterogeneous. Variations in these parameters may have an important impact on experimental outcomes in Langendorff-perfused hearts and serve as a potential explanation for why some studies are seemingly irreproducible. An alternative view, however, is that heterogeneous scientific outcomes are a desirable scientific product that can yield important insights into health and disease if methodological reporting is enhanced. In this regard, several attempts have been made at establishing guidelines for the design and reporting of cardiac electrophysiology studies (183, 184). Though, as the data above demonstrate, unreported variance remains a contemporary issue. As such, we must continue community discussions on methods reporting and work with journals to determine how to best approach methods reporting.
GRANTS
This study was supported by the National Institutes of Health Grants F31-HL147438 (to D.R.K.), R01-HL141855, R01-HL138003, and R01-HL102298 (to S.P.).
DISCLOSURES
No conflicts of interest, financial or otherwise, are declared by the authors.
AUTHOR CONTRIBUTIONS
D.R.K., K.M.H., and S.P. conceived and designed research; D.R.K., K.M.H., G.S.H., and S.P. performed experiments; D.R.K., K.M.H., G.S.H., and S.P. analyzed data; D.R.K., K.M.H., G.S.H., and S.P. interpreted results of experiments; D.R.K., K.M.H., and S.P. prepared figures; D.R.K., K.M.H., and S.P. drafted manuscript; D.R.K., K.M.H., G.S.H., and S.P. edited and revised manuscript; D.R.K., K.M.H., G.S.H., and S.P. approved final version of manuscript.
REFERENCES
- 1. Goodman SN, Fanelli D, Ioannidis JPA. What does research reproducibility mean? Sci Transl Med 8: 341ps12, 2016. doi: 10.1126/scitranslmed.aaf5027. [DOI] [PubMed] [Google Scholar]
- 2. Parekh A, Fadiran EO, Uhl K, Throckmorton DC. Adverse effects in women: implications for drug development and regulatory policies. Expert Rev Clin Pharmacol 4: 453–466, 2011. doi: 10.1586/ecp.11.29. [DOI] [PubMed] [Google Scholar]
- 3. Prinz F, Schlange T, Asadullah K. Believe it or not: how much can we rely on published data on potential drug targets? Nat Rev Drug Discov 10: 712–713, 2011. doi: 10.1038/nrd3439-c1. [DOI] [PubMed] [Google Scholar]
- 4. Begley CG, Ellis LM. Drug development: raise standards for preclinical cancer research. Nature 483: 531–533, 2012. doi: 10.1038/483531a. [DOI] [PubMed] [Google Scholar]
- 5. Freedman LP. On rigor and replication. Science 356: 34–34, 2017. doi: 10.1126/science.aam8039. [DOI] [PubMed] [Google Scholar]
- 6. Harris R. Rigor Mortis (1st ed.). New York: Basic Books, 2017. [Google Scholar]
- 7. Fanelli D. Opinion: is science really facing a reproducibility crisis, and do we need it to? Proc Natl Acad Sci USA 115: 2628–2631, 2018. doi: 10.1073/pnas.1708272114. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 8. Ramirez FD, Motazedian P, Jung RG, Di Santo P, MacDonald ZD, Moreland R, Simard T, Clancy AA, Russo JJ, Welch VA, Wells GA, Hibbert B. Methodological rigor in preclinical cardiovascular studies. Circ Res 120: 1916–1926, 2017. doi: 10.1161/CIRCRESAHA.117.310628. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 9. Langendorff O. Untersuchungen am überlebenden Säugethierherzen. Pflüger Arch 61: 291–332, 1895. doi: 10.1007/BF01812150. [DOI] [Google Scholar]
- 10. Skrzypiec-Spring M, Grotthus B, Szelag A, Schulz R. Isolated heart perfusion according to Langendorff-Still viable in the new millennium. J Pharmacol Toxicol Methods 55: 113–126, 2007. doi: 10.1016/j.vascn.2006.05.006. [DOI] [PubMed] [Google Scholar]
- 11. Broadley KJ. The Langendorff heart preparation-Reappraisal of its role as a research and teaching model for coronary vasoactive drugs. J Pharmacol Methods 2: 143–156, 1979. doi: 10.1016/0160-5402(79)90038-X. [DOI] [Google Scholar]
- 12. Porter WT. A new method for the study of the isolated mammalian heart. Am J Physiol- 1: 511–518, 1898. doi: 10.1152/ajplegacy.1898.1.4.511. [DOI] [Google Scholar]
- 13. Zimmer HG. The isolated perfused heart and its pioneers. News Physiol Sci 13: 203–210, 1998. doi: 10.1152/physiologyonline.1998.13.4.203. [DOI] [PubMed] [Google Scholar]
- 14. Bøtker HE, Hausenloy D, Andreadou I, Antonucci S, Boengler K, Davidson SM, Deshwal S, Devaux Y, Di Lisa F, Di Sante M, Efentakis P, Femminò S, García-Dorado D, Giricz Z, Ibanez B, Iliodromitis E, Kaludercic N, Kleinbongard P, Neuhäuser M, Ovize M, Pagliaro P, Rahbek-Schmidt M, Ruiz-Meana M, Schlüter K-D, Schulz R, Skyschally A, Wilder C, Yellon DM, Ferdinandy P, Heusch G. Practical guidelines for rigor and reproducibility in preclinical and clinical studies on cardioprotection. Basic Res Cardiol 113: 39, 2018. doi: 10.1007/s00395-018-0696-8. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 15. Entz M 2nd, King DR, Poelzing S. Design and validation of a tissue bath 3D printed with PLA for optically mapping suspended whole heart preparations. Am J Physiol Heart Circ Physiol 313: H1190–H1198, 2017. doi: 10.1152/ajpheart.00150.2017. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 16. Rosati B, Dong M, Cheng L, Liou S-R, Yan Q, Park JY, Shiang E, Sanguinetti M, Wang H-S, McKinnon D. Evolution of ventricular myocyte electrophysiology. Physiol Genomics 35: 262–272, 2008. doi: 10.1152/physiolgenomics.00159.2007. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 17. O'Hara T, Rudy Y. Quantitative comparison of cardiac ventricular myocyte electrophysiology and response to drugs in human and nonhuman species. Am J Physiol-Heart Circ Physiol 302: H1023–H1030, 2012. doi: 10.1152/ajpheart.00785.2011. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 18. Guo D, Zhou J, Zhao X, Gupta P, Kowey PR, Martin J, Wu Y, Liu T, Yan GX. L-type calcium current recovery versus ventricular repolarization: preserved membrane-stabilizing mechanism for different QT intervals across species. Heart Rhythm 5: 271–279, 2008. doi: 10.1016/j.hrthm.2007.09.025. [DOI] [PubMed] [Google Scholar]
- 19. Trautwein W, McDonald TF. Current-voltage relations in ventricular muscle preparations from different species. Pflugers Arch 374: 79–89, 1978. doi: 10.1007/BF00585700. [DOI] [PubMed] [Google Scholar]
- 20. Sham JS, Hatem SN, Morad M. Species differences in the activity of the Na(+)-Ca2+ exchanger in mammalian cardiac myocytes. J Physiol 488: 623–631, 1995. doi: 10.1113/jphysiol.1995.sp020995. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 21. Bridge JHB, Smolley JR, Spitzer KW. The relationship between charge movements associated with ICa and INa-Ca in cardiac myocytes. Science 248: 376–378, 1990. doi: 10.1126/science.2158147. [DOI] [PubMed] [Google Scholar]
- 22. Weber CR, Piacentino V, Ginsburg KS, Houser SR, Bers DM. Na+-Ca2+ exchange current and submembrane [Ca2+] during the cardiac action potential. Circ Res 90: 182–189, 2002. doi: 10.1161/hh0202.103940. [DOI] [PubMed] [Google Scholar]
- 23. Weber CR, Piacentino V, Houser SR, Bers DM. Dynamic regulation of sodium/calcium exchange function in human heart failure. Circulation 108: 2224–2229, 2003. doi: 10.1161/01.CIR.0000095274.72486.94. [DOI] [PubMed] [Google Scholar]
- 24. Huang CLH. Murine electrophysiological models of cardiac arrhythmogenesis. Physiol Rev 97: 283–409, 2017. doi: 10.1152/physrev.00007.2016. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 25. Bartos DC, Grandi E, Ripplinger CM. Ion channels in the heart. Compr Physiol 5: 1423–1464, 2015. doi: 10.1002/cphy.c140069. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 26. Gussak I, Chaitman BR, Kopecky SL, Nerbonne JM. Rapid venticular repolarization in rodents: electrocardiographic manifestations, molecular mechanisms, and clinical insights. J Electrocardiol 33: 159–170, 2000. doi: 10.1016/s0022-0736(00)80072-2. [DOI] [PubMed] [Google Scholar]
- 27. Francis J, Antzelevitch C. Atrial fibrillation and Brugada syndrome. J Am Coll Cardiol 51: 1149–1153, 2008. doi: 10.1016/j.jacc.2007.10.062. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 28. Calloe K, Cordeiro JM, Di Diego JM, Hansen RS, Grunnet M, Olesen SP, Antzelevitch C. A transient outward potassium current activator recapitulates the electrocardiographic manifestations of Brugada syndrome. Cardiovasc Res 81: 686–694, 2009. doi: 10.1093/cvr/cvn339. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 29. Gussak I, Antzelevitch C, Bjerregaard P, Towbin JA, Chaitman BR. The Brugada syndrome: clinical, electrophysiologic and genetic aspects. J Am Coll Cardiol 33: 5–15, 1999. doi: 10.1016/s0735-1097(98)00528-2. [DOI] [PubMed] [Google Scholar]
- 30. Rougier J-S, Essers MC, Gillet L, Guichard S, Sonntag S, Shmerling D, Abriel H. A distinct pool of Nav1.5 channels at the lateral membrane of murine ventricular cardiomyocytes. Front Physiol 10: 834, 2019. doi: 10.3389/fphys.2019.00834. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 31. Jelinek M, Wallach C, Ehmke H, Schwoerer AP. Genetic background dominates the susceptibility to ventricular arrhythmias in a murine model of β-adrenergic stimulation. Sci Rep 8: 2312, 2018. doi: 10.1038/s41598-018-20792-5. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 32. Slater J, Blizard DA, Pohorecky LA. Central and peripheral norepinephrine metabolism in rat strains selectively bred for differences in response to stress. Pharmacol Biochem Behav 6: 511–520, 1977. doi: 10.1016/0091-3057(77)90110-1. [DOI] [PubMed] [Google Scholar]
- 33. Obergassel J, O'Reilly M, Sommerfeld LC, Kabir SN, O'Shea C, Syeda F, Eckardt L, Kirchhof P, Fabritz L. Effects of genetic background, sex, and age on murine atrial electrophysiology. Europace 23: 958–969, 2021. doi: 10.1093/europace/euaa369. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 34. Charlton KM, Corner AH, Davey K, Kramer JK, Mahadevan S, Sauer FD. Cardiac lesions in rats fed rapeseed oils. Can J Comp Med 39: 261–269, 1975. [PMC free article] [PubMed] [Google Scholar]
- 35. Lindsey ML, LeBlanc AJ, Ripplinger CM, Carter JR, Kirk JA, Hansell Keehan K, Brunt KR, Kleinbongard P, Kassiri Z. Reinforcing rigor and reproducibility expectations for use of sex and gender in cardiovascular research. Am J Physiol Heart Circ Physiol 321: H819–H824, 2021. doi: 10.1152/ajpheart.00418.2021. [DOI] [PubMed] [Google Scholar]
- 36. Czubryt MP, Espira L, Lamoureux L, Abrenica B. The role of sex in cardiac function and disease. Can J Physiol Pharmacol 84: 93–109, 2006. doi: 10.1139/y05-151. [DOI] [PubMed] [Google Scholar]
- 37. Prabhavathi K, Selvi KT, Poornima KN, Sarvanan A. Role of biological sex in normal cardiac function and in its disease outcome – a review. J Clin Diagn Res 8: BE01–BE04, 2014. doi: 10.7860/JCDR/2014/9635.4771. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 38. Hula N, Vu J, Quon A, Kirschenman R, Spaans F, Liu R, Cooke C-LM, Davidge ST. Sex-specific effects of prenatal hypoxia on the cardiac endothelin system in adult offspring. Am J Physiol Heart Circ Physiol 322: H442–H450, 2022. doi: 10.1152/ajpheart.00636.2021. [DOI] [PubMed] [Google Scholar]
- 39. Börzsei D, Priksz D, Szabó R, Bombicz M, Karácsonyi Z, Puskás LG, Fehér LZ, Radák Z, Kupai K, Berkó AM, Varga C, Juhász B, Pósa A. Exercise-mitigated sex-based differences in aging: from genetic alterations to heart performance. Am J Physiol Heart Circ Physiol 320: H854–H866, 2021. doi: 10.1152/ajpheart.00643.2020. [DOI] [PubMed] [Google Scholar]
- 40. Veenema R, Casin KM, Sinha P, Kabir R, Mackowski N, Taube N, Bedja D, Chen R, Rule A, Kohr MJ. Inorganic arsenic exposure induces sex-disparate effects and exacerbates ischemia-reperfusion injury in the female heart. Am J Physiol Heart Circ Physiol 316: H1053–H1064, 2019. doi: 10.1152/ajpheart.00364.2018. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 41. Kabir R, Sinha P, Mishra S, Ebenebe OV, Taube N, Oeing CU, Keceli G, Chen R, Paolocci N, Rule A, Kohr MJ. Inorganic arsenic induces sex-dependent pathological hypertrophy in the heart. Am J Physiol Heart Circ Physiol 320: H1321–H1336, 2021. doi: 10.1152/ajpheart.00435.2020. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 42. Parks RJ, Howlett SE. Sex differences in mechanisms of cardiac excitation-contraction coupling. Pflugers Arch 465: 747–763, 2013. doi: 10.1007/s00424-013-1233-0. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 43. Parks RJ, Ray G, Bienvenu LA, Rose RA, Howlett SE. Sex differences in SR Ca(2+) release in murine ventricular myocytes are regulated by the cAMP/PKA pathway. J Mol Cell Cardiol 75: 162–173, 2014. doi: 10.1016/j.yjmcc.2014.07.006. [DOI] [PubMed] [Google Scholar]
- 44. Papp R, Bett GCL, Lis A, Rasmusson RL, Baczkó I, Varró A, Salama G. Genomic upregulation of cardiac Cav1.2α and NCX1 by estrogen in women. Biol Sex Differ 8: 26, 2017. doi: 10.1186/s13293-017-0148-4. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 45. Mahmoodzadeh S, Dworatzek E. The role of 17β-estradiol and estrogen receptors in regulation of Ca2+ channels and mitochondrial function in cardio myocytes. Front Endocrinol (Lausanne) 10: 310, 2019. doi: 10.3389/fendo.2019.00310. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 46. Schmaltz HN, Southern DA, Maxwell CJ, Knudtson ML, Ghali WA; APPROACH Investigators. Patient sex does not modify ejection fraction as a predictor of death in heart failure: Insights from the APPROACH cohort. J Gen Intern Med 23: 1940–1946, 2008. doi: 10.1007/s11606-008-0804-9. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 47. Leblanc N, Chartier D, Gosselin H, Rouleau JL. Age and gender differences in excitation-contraction coupling of the rat ventricle. J Physiol 511: 533–548, 1998. doi: 10.1111/j.1469-7793.1998.533bh.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 48. Ayaz O, Howlett SE. Testosterone modulates cardiac contraction and calcium homeostasis: cellular and molecular mechanisms. Biol Sex Differ 6: 9, 2015. doi: 10.1186/s13293-015-0027-9. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 49. Salama G, Bett GCL. Sex differences in the mechanisms underlying long QT syndrome. Am J Physiol Heart Circ Physiol 307: H640–H648, 2014. doi: 10.1152/ajpheart.00864.2013. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 50. Locati EH, Zareba W, Moss AJ, Schwartz PJ, Vincent GM, Lehmann MH, Towbin JA, Priori SG, Napolitano C, Robinson JL, Andrews M, Timothy K, Hall WJ. Age- and sex-related differences in clinical manifestations in patients with congenital long-QT syndrome: findings from the International LQTS Registry. Circulation 97: 2237–2244, 1998. doi: 10.1161/01.cir.97.22.2237. [DOI] [PubMed] [Google Scholar]
- 51. Lehmann MH, Timothy KW, Frankovich D, Fromm BS, Keating M, Locati EH, Taggart RT, PhD, Towbin JA, Moss AJ, Schwartz PJ, Vincent GM. Age-gender influence on the rate-corrected QT interval and the QT-heart rate relation in families with genotypically characterized long QT syndrome. J Am Coll Cardiol 29: 93–99, 1997. doi: 10.1016/S0735-1097(96)00454-8. [DOI] [PubMed] [Google Scholar]
- 52. Zhang TY, Zhao BJ, Wang T, Wang J. Effect of aging and sex on cardiovascular structure and function in wildtype mice assessed with echocardiography. Sci Rep 11: 22800, 2021. doi: 10.1038/s41598-021-02196-0. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 53. Woitowich NC, Beery A, Woodruff T. A 10-year follow-up study of sex inclusion in the biological sciences. eLife 9:e56344, 2020. doi: 10.7554/eLife.56344. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 54. Jackson SJ, Andrews N, Ball D, Bellantuono I, Gray J, Hachoumi L, Holmes A, Latcham J, Petrie A, Potter P, Rice A, Ritchie A, Stewart M, Strepka C, Yeoman M, Chapman K. Does age matter? The impact of rodent age on study outcomes. Lab Anim 51: 160–169, 2017. doi: 10.1177/0023677216653984. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 55. Peters NS, Severs NJ, Rothery SM, Lincoln C, Yacoub MH, Green CR. Spatiotemporal relation between gap junctions and fascia adherens junctions during postnatal development of human ventricular myocardium. Circulation 90: 713–725, 1994. doi: 10.1161/01.cir.90.2.713. [DOI] [PubMed] [Google Scholar]
- 56. Vreeker A, van Stuijvenberg L, Hund TJ, Mohler PJ, Nikkels PGJ, van Veen TAB. Assembly of the cardiac intercalated disk during pre- and postnatal development of the human heart. PLoS One 9: e94722, 2014. doi: 10.1371/journal.pone.0094722. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 57. Angst BD, Khan LUR, Severs NJ, Whitely K, Rothery S, Thompson RP, Magee AI, Gourdie RG. Dissociated spatial patterning of gap junctions and cell adhesion junctions during postnatal differentiation of ventricular myocardium. Circ Res 80: 88–94, 1997. doi: 10.1161/01.res.80.1.88. [DOI] [PubMed] [Google Scholar]
- 58. Fleg JL, Strait J. Age-associated changes in cardiovascular structure and function: a fertile milieu for future disease. Heart Fail Rev 17: 545–554, 2012. doi: 10.1007/s10741-011-9270-2. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 59. Strait JB, Lakatta EG. Aging-associated cardiovascular changes and their relationship to heart failure. Heart Fail Clin 8: 143–164, 2012. doi: 10.1016/j.hfc.2011.08.011. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 60. Jakovljevic DG, Papakonstantinou L, Blamire AM. Effect of physical activity on age-related changes in cardiac function and performance in women. Circ Cardiovasc Imaging 8: e002086, 2014. doi: 10.1161/CIRCIMAGING.114.002086. [DOI] [PubMed] [Google Scholar]
- 61. Swift LM, Burke M, Guerrelli D, Reilly M, Ramadan M, McCullough D, Prudencio T, Mulvany C, Chaluvadi A, Jaimes R, Posnack NG. Age-dependent changes in electrophysiology and calcium handling: implications for pediatric cardiac research. Am J Physiol Heart Circ Physiol 318: H354–H365, 2020. doi: 10.1152/ajpheart.00521.2019. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 62. Xu X, Wang B, Ren C, Hu J, Greenberg DA, Chen T, Xie L, Jin K. Age-related impairment of vascular structure and functions. Aging Dis 8: 590–610, 2017. doi: 10.14336/AD.2017.0430. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 63. Trial J, Cieslik KA. Changes in cardiac resident fibroblast physiology and phenotype in aging. Am J Physiol Heart Circ Physiol 315: H745–H755, 2018. doi: 10.1152/ajpheart.00237.2018. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 64. Lesnefsky EJ, Chen Q, Hoppel CL. Mitochondrial metabolism in aging heart. Circ Res 118: 1593–1611, 2016. doi: 10.1161/CIRCRESAHA.116.307505. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 65. Salihu HM, Bonnema SM, Alio AP. Obesity: what is an elderly population growing into? Maturitas 63: 7–12, 2009. doi: 10.1016/j.maturitas.2009.02.010. [DOI] [PubMed] [Google Scholar]
- 66. Lunenfeld B, Stratton P. The clinical consequences of an ageing world and preventive strategies. Best Pract Res Clin Obstet Gynaecol 27: 643–659, 2013. doi: 10.1016/j.bpobgyn.2013.02.005. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 67. Christensen K, Doblhammer G, Rau R, Vaupel JW. Ageing populations: the challenges ahead. Lancet 374: 1196–1208, 2009. doi: 10.1016/S0140-6736(09)61460-4. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 68. Hew KW, Keller KA. Postnatal anatomical and functional development of the heart: a species comparison. Birth Defects Res B Dev Reprod Toxicol 68: 309–320, 2003. doi: 10.1002/bdrb.10034. [DOI] [PubMed] [Google Scholar]
- 69. Maillet M, Van Berlo JH, Molkentin JD. Molecular basis of physiological heart growth: fundamental concepts and new players. Nat Rev Mol Cell Biol 14: 38–48, 2013. doi: 10.1038/nrm3495. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 70. Mattfeldt T, Mall G. Growth of capillaries and myocardial cells in the normal rat heart. J Mol Cell Cardiol 19: 1237–1246, 1987. doi: 10.1016/s0022-2828(87)80533-3. [DOI] [PubMed] [Google Scholar]
- 71. Wulfsohn D, Nyengaard JR, Tang Y. Postnatal growth of cardiomyocytes in the left ventricle of the rat. Anat Rec A Discov Mol Cell Evol Biol 277: 236–247, 2004. doi: 10.1002/ar.a.20009. [DOI] [PubMed] [Google Scholar]
- 72. Vliegen HW, van der Laarse A, Huysman JA, Wijnvoord EC, Mentar M, Cornelisse CJ, Eulderink F. Morphometric quantification of myocyte dimensions validated in normal growing rat hearts and applied to hypertrophic human hearts. Cardiovasc Res 21: 352–357, 1987. doi: 10.1093/cvr/21.5.352. [DOI] [PubMed] [Google Scholar]
- 73. Kimura K, Ieda M, Fukuda K. Development, maturation, and transdifferentiation of cardiac sympathetic nerves. Circ Res 110: 325–336, 2012. doi: 10.1161/CIRCRESAHA.111.257253. [DOI] [PubMed] [Google Scholar]
- 74. Végh A, Duim S, Smits A, Poelmann R, ten Harkel A, DeRuiter M, Goumans M, Jongbloed M. Part and parcel of the cardiac autonomic nerve system: unravelling its cellular building blocks during development. J Cardiovasc Dev Dis 3: 28, 2016. doi: 10.3390/jcdd3030028. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 75. Horackova M, Byczko Z, Slavikova J. Postnatal development of the rat intrinsic cardiac nervous system: a confocal laser scanning microscopy study in whole-mount atria. Tissue and Cell 32: 377–388, 2000. doi: 10.1054/tice.2000.0126. [DOI] [PubMed] [Google Scholar]
- 76. Piquereau J, Novotova M, Fortin D, Garnier A, Ventura-Clapier R, Veksler V, Joubert F. Postnatal development of mouse heart: formation of energetic microdomains. Journal of Physiology 588: 2443–2454, 2010. doi: 10.1113/jphysiol.2010.189670. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 77. Piquereau J, Ventura-Clapier R. Maturation of cardiac energy metabolism during perinatal development. Front Physiol 9: 959, 2018. doi: 10.3389/fphys.2018.00959. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 78. Hall N, DeLuca M. Developmental changes in creatine phosphokinase isoenzymes in neonatal mouse hearts. Biochem Biophys Res Commun 66: 988–994, 1975. doi: 10.1016/0006-291X(75)90737-8. [DOI] [PubMed] [Google Scholar]
- 79. Baldwin KM, Cooke DA, Cheadle WG. Enzyme alterations in neonatal heart muscle during development. J Mol Cell Cardiol 9: 651–660, 1977. doi: 10.1016/S0022-2828(77)80360-X. [DOI] [PubMed] [Google Scholar]
- 80. Bonda TA, Szynaka B, Sokołowska M, Dziemidowicz M, Winnicka MM, Chyczewski L, Kamiński KA. Remodeling of the intercalated disc related to aging in the mouse heart. J Cardiol 68: 261–268, 2016. doi: 10.1016/j.jjcc.2015.10.001. [DOI] [PubMed] [Google Scholar]
- 81. Waldeyer C, Fabritz L, Fortmueller L, Gerss J, Damke D, Blana A, Laakmann S, Kreienkamp N, Volkery D, Breithardt G, Kirchhof P. Regional, age-dependent, and genotype-dependent differences in ventricular action potential duration and activation time in 410 Langendorff-perfused mouse hearts. Basic Res Cardiol 104: 523–533, 2009. doi: 10.1007/s00395-009-0019-1. [DOI] [PubMed] [Google Scholar]
- 82. Bain CB, Settlage JM, Blair GA, Poelzing S. No relationship between perceived health anomalies and perceived experimental success in retired breeder male Hartley albino guinea pigs (Preprint). bioRxiv 2020. doi: 10.1101/2020.03.06.979336. [DOI]
- 83. Harris RBS, Mitchell TD, Simpson J, Redmann SM, Youngblood BD, Ryan DH. Weight loss in rats exposed to repeated acute restraint stress is independent of energy or leptin status. Am J Physiol Regul Integr Comp Physiol 282: R77–R88, 2002. doi: 10.1152/ajpregu.2002.282.1.R77. [DOI] [PubMed] [Google Scholar]
- 84. Sandrini L, Ieraci A, Amadio P, Zarà M, Barbieri SS. Impact of acute and chronic stress on thrombosis in healthy individuals and cardiovascular disease patients. Int J Mol Sci 21: 7818, 2020. doi: 10.3390/ijms21217818. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 85. Firmino EMS, Kuntze LB, Lagatta DC, Dias DPM, Resstel LBM. Effect of chronic stress on cardiovascular and ventilatory responses activated by both chemoreflex and baroreflex in rats. J Exp Biol 222: jeb204883, 2019. doi: 10.1242/jeb.204883. [DOI] [PubMed] [Google Scholar]
- 86. Sutko JL, Kenyon JL, Reeves JP. Effects of amrinone and milrinone on calcium influx into the myocardium. Circulation 73: III52–III58, 1986. [PubMed] [Google Scholar]
- 87. Patel KHK, Hwang T, Se Liebers C, Ng FS. Epicardial adipose tissue as a mediator of cardiac arrhythmias. Am J Physiol Heart Circ Physiol 322: H129–H144, 2022. doi: 10.1152/ajpheart.00565.2021. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 88. Ahangarpour A, Zeidooni L, Samimi A, Alboghobeish S, Khorsandi LS, Moradi M. Chronic exposure to arsenic and high fat diet additively induced cardiotoxicity in male mice. Res Pharm Sci 13: 47–56, 2018. doi: 10.4103/1735-5362.220967. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 89. Pan A, Tan Y, Wang Z, Xu G. STAT4 silencing underlies a novel inhibitory role of microRNA-141-3p in inflammation response of mice with experimental autoimmune myocarditis. Am J Physiol Heart Circ Physiol 317: H531–H540, 2019. doi: 10.1152/ajpheart.00048.2019. [DOI] [PubMed] [Google Scholar]
- 90. Martin B, Ji S, Maudsley S, Mattson MP. “Control” laboratory rodents are metabolically morbid: why it matters. Proc Natl Acad Sci USA 107: 6127–6133, 2010. doi: 10.1073/pnas.0912955107. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 91. Lester PA, Moore RM, Shuster KA, Myers DD. Anesthesia and Analgesia. In: The Laboratory Rabbit, Guinea Pig, Hamster, and Other Rodents, edited by Suckow MA, Stevens KA, Wilson RP.. London, Elsevier, 2012, p. 33–56. [Google Scholar]
- 92. Segal J, Schwalb H, Shmorak V, Uretzky G. Effect of anesthesia on cardiac function and response in the perfused rat heart. J Mol Cell Cardiol 22: 1317–1324, 1990. doi: 10.1016/0022-2828(90)90067-c. [DOI] [PubMed] [Google Scholar]
- 93. Jiang X, Gao L, Zhang Y, Wang G, Liu Y, Yan C, Sun H. A comparison of the effects of ketamine, chloral hydrate and pentobarbital sodium anesthesia on isolated rat hearts and cardiomyocytes. J Cardiovasc Med (Hagerstown) 12: 732–735, 2011. doi: 10.2459/JCM.0b013e32834a6697. [DOI] [PubMed] [Google Scholar]
- 94. Aroni F, Iacovidou N, Dontas I, Pourzitaki C, Xanthos T. Pharmacological aspects and potential new clinical applications of ketamine: reevaluation of an old drug. J Clin Pharmacol 49: 957–964, 2009. doi: 10.1177/0091270009337941. [DOI] [PubMed] [Google Scholar]
- 95. Kohrs R, Durieux ME. Ketamine: teaching an old drug new tricks. Anesth Analg 87: 1186–1193, 1998. doi: 10.1097/00000539-199811000-00039. [DOI] [PubMed] [Google Scholar]
- 96. Visser E, Schug SA. The role of ketamine in pain management. Biomed Pharmacother 60: 341–348, 2006. doi: 10.1016/j.biopha.2006.06.021. [DOI] [PubMed] [Google Scholar]
- 97. Sanders DB, Kelley T, Larson D. The role of nitric oxide synthase/nitric oxide in vascular smooth muscle control. Perfusion 15: 97–104, 2000. doi: 10.1177/026765910001500203. [DOI] [PubMed] [Google Scholar]
- 98. Sloan RC, Rosenbaum M, O'Rourke D, Oppelt K, Frasier CR, Waston CA, Allan AG, Brown DA. High doses of ketamine-xylazine anesthesia reduce cardiac ischemia-reperfusion injury in guinea pigs. J Am Assoc Lab Anim Sci 50: 349–354, 2011. [PMC free article] [PubMed] [Google Scholar]
- 99. Eger EI 2nd. Isoflurane: a review. Anesthesiology 55: 559–576, 1981. doi: 10.1097/00000542-198111000-00014. [DOI] [PubMed] [Google Scholar]
- 100. Papich MG (editor). Isoflurane. In: Saunders Handbook of Veterinary Drugs. Elsevier, 2016, p. 411–412. [Google Scholar]
- 101. Zaugg M, Lucchinetti E, Spahn DR, Pasch T, Schaub MC. Volatile anesthetics mimic cardiac preconditioning by priming the activation of mitochondrial K(ATP) channels via multiple signaling pathways. Anesthesiology 97: 4–14, 2002. doi: 10.1097/00000542-200207000-00003. [DOI] [PubMed] [Google Scholar]
- 102. Wang J, Sun J, Qiao S, Li H, Che T, Wang C, An J. Effects of isoflurane on complex II-associated mitochondrial respiration and reactive oxygen species production: roles of nitric oxide and mitochondrial KATP channels. Mol Med Rep 20: 4383–4390, 2019. doi: 10.3892/mmr.2019.10658. [DOI] [PubMed] [Google Scholar]
- 103. Noda K, Philips BJ, Ren X, Sanchez PG. Impact of heparin on endothelial glycocalyx in lung grafts during ex vivo lung perfusion. J Heart Lung Transpl 40: S344–S345, 2021. doi: 10.1016/j.healun.2021.01.972. [DOI] [Google Scholar]
- 104. Oguchi T, Doursout MF, Kashimoto S, Liang YY, Hartley CJ, Chelly JE. Role of heparin and nitric oxide in the cardiac and regional hemodynamic properties of protamine in conscious chronically instrumented dogs. Anesthesiology 94: 1016–1025, 2001. doi: 10.1097/00000542-200106000-00016. [DOI] [PubMed] [Google Scholar]
- 105. Murry CE, Jennings RB, Reimer KA. Preconditioning with ischemia: a delay of lethal cell injury in ischemic myocardium. Circulation 74: 1124–1136, 1986. doi: 10.1161/01.CIR.74.5.1124. [DOI] [PubMed] [Google Scholar]
- 106. Iliodromitis EK, Lazou A, Kremastinos DT. Ischemic preconditioning: protection against myocardial necrosis and apoptosis. Vasc Health Risk Manag 3: 629–637, 2007. [PMC free article] [PubMed] [Google Scholar]
- 107. Weerateerangkul P, Chattipakorn S, Chattipakorn N. Roles of the nitric oxide signaling pathway in cardiac ischemic preconditioning against myocardial ischemia-reperfusion injury. Med Sci Monit 17: RA44–RA52, 2011. doi: 10.12659/MSM.881385. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 108. Shibutani S, Osanai T, Ashitate T, Sagara S, Izumiyama K, Yamamoto Y, Hanada K, Echizen T, Tomita H, Fujita T, Miwa T, Matsubara H, Homma Y, Okumura K. Coronary vasospasm induced in transgenic mouse with increased phospholipase C-δ1 activity. Circulation 125: 1027–1036, 2012. doi: 10.1161/CIRCULATIONAHA.111.064303. [DOI] [PubMed] [Google Scholar]
- 109. Amezcua JL, Palmer RM, de Souza BM, Moncada S. Nitric oxide synthesized from l-arginine regulates vascular tone in the coronary circulation of the rabbit. Br J Pharmacol 97: 1119–1124, 1989. doi: 10.1111/j.1476-5381.1989.tb12569.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 110. Koretsune Y, Corretti MC, Kusuoka H, Marban E. Mechanism of early ischemic contractile failure. Inexcitability, metabolite accumulation, or vascular collapse? Circ Res 68: 255–262, 1991. doi: 10.1161/01.RES.68.1.255. [DOI] [PubMed] [Google Scholar]
- 111. Kitakaze M, Marban E. Cellular mechanism of the modulation of contractile function by coronary perfusion pressure in ferret hearts. J Physiol 414: 455–472, 1989. doi: 10.1113/jphysiol.1989.sp017698. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 112. Chang KC, Sasano T, Wang YC, Huang SKS. Nitric oxide synthase 1 adaptor protein, an emerging new genetic marker for QT prolongation and sudden cardiac death. Acta Cardiol Sin 29: 217–225, 2013. [PMC free article] [PubMed] [Google Scholar]
- 113. Wang L. Role of nitric oxide in regulating cardiac electrophysiology. Exp Clin Cardiol 6: 167–171, 2001. [PMC free article] [PubMed] [Google Scholar]
- 114. Wijns W, Serruys PW, Slager CJ, Grimm J, Krayenbuehl HP, Hugenholtz PG, Hess OM. Effect of coronary occlusion during percutaneous transluminal angioplasty in humans on left ventricular chamber stiffness and regional diastolic pressure-radius relations. J Am Coll Cardiol 7: 455–463, 1986. doi: 10.1016/s0735-1097(86)80453-3. [DOI] [PubMed] [Google Scholar]
- 115. Myers ML, Bolli R, Lekich RF, Hartley CJ, Roberts R. Enhancement of recovery of myocardial function by oxygen free-radical scavengers after reversible regional ischemia. Circulation 72: 915–921, 1985. doi: 10.1161/01.cir.72.4.915. [DOI] [PubMed] [Google Scholar]
- 116. Xue Q, Zhang L. Prenatal hypoxia causes a sex-dependent increase in heart susceptibility to ischemia and reperfusion injury in adult male offspring: role of protein kinase C epsilon. J Pharmacol Exp Ther 330: 624–632, 2009. doi: 10.1124/jpet.109.153239. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 117. Kher A, Wang M, Tsai BM, Pitcher JM, Greenbaum ES, Nagy RD, Patel KM, Wairiuko GM, Markel TA, Meldrum DR. Sex differences in the myocardial inflammatory response to acute injury. Shock 23: 1–10, 2005. doi: 10.1097/01.shk.0000148055.12387.15. [DOI] [PubMed] [Google Scholar]
- 118. Piro M, Della Bona R, Abbate A, Biasucci LM, Crea F. Sex-related differences in myocardial remodeling. J Am Coll Cardiol 55: 1057–1065, 2010. doi: 10.1016/j.jacc.2009.09.065. [DOI] [PubMed] [Google Scholar]
- 119. Rivkees SA. The development of circadian rhythms: from animals to humans. Sleep Med Clin 2: 331–341, 2007. doi: 10.1016/j.jsmc.2007.05.010. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 120. Harkness JE, Murray KA, Wagner JE. Biology and diseases of guinea pigs. In: Laboratory Animal Medicine, edited by Anderson LC, Otto G, Pritchett-Corning KR, Whary MT.. London, Elsevier, 2002, p. 203–246. [Google Scholar]
- 121. Gery S, Koeffler HP. Circadian rhythms and cancer. Cell Cycle 9: 1097–1103, 2010. doi: 10.4161/cc.9.6.11046. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 122. Jeyaraj D, Haldar SM, Wan X, McCauley MD, Ripperger JA, Hu K, Lu Y, Eapen BL, Sharma N, Ficker E, Cutler MJ, Gulick J, Sanbe A, Robbins J, Demolombe S, Kondratov RV, Shea SA, Albrecht U, Wehrens XHT, Rosenbaum DS, Jain MK. Circadian rhythms govern cardiac repolarization and arrhythmogenesis. Nature 483: 96–99, 2012. doi: 10.1038/nature10852. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 123. Schroder EA, Ono M, Johnson SR, Rozmus ER, Burgess DE, Esser KA, Delisle BP. The role of the cardiomyocyte circadian clocks in ion channel regulation and cardiac electrophysiology. J Physiol 600: 2037–2048, 2022. doi: 10.1113/JP282402. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 124. Tyrode MV. The mode of action of some purgative slats. Archives internationales de pharmacodynamie et de therapie 20: 205–223, 1910. [Google Scholar]
- 125. Kornberg H, Williamson DH. Hans Adolf Krebs, 25 August 1900– 22 November 1981. Biogr Mem Fellows R Soc 30: 351–385, 1984. doi: 10.1098/rsbm.1984.0013. [DOI] [PubMed] [Google Scholar]
- 126. Krebs HA, Henseleit K. Untersuchungen uber die Harnstoffbildung im Tierkörper. Hoppe-Seyler´s Zeitschrift für physiologische Chemie 210: 33–66, 1932. doi: 10.1515/bchm2.1932.210.1-2.33. [DOI] [Google Scholar]
- 127. Leetham C. Action of certain drugs on isolated strips of ventricle. J Physiol 46: 151–158, 1913. doi: 10.1113/jphysiol.1913.sp001583. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 128. Miller DJ. Sydney Ringer; physiological saline, calcium and the contraction of the heart. J Physiol 555: 585–587, 2004. doi: 10.1113/jphysiol.2004.060731. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 129. Fye WB. Sydney Ringer, calcium, and cardiac function. Circulation 69: 849–853, 1984. doi: 10.1161/01.CIR.69.4.849. [DOI] [PubMed] [Google Scholar]
- 130. Ringer S. An investigation regarding the action of rubidium and Cæsium salts compared with the action of potassium salts on the ventricle of the frog’s. J Physiol 4: 370–386, 1884. doi: 10.1113/jphysiol.1884.sp000139. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 131. Ringer S. A third contribution regarding the influence of the inorganic constituents of the blood on the ventricular contraction. J Physiol 4: 222–225, 1883. doi: 10.1113/jphysiol.1883.sp000127. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 132. Ringer S. A further contribution regarding the influence of the different constituents of the blood on the contraction of the heart. J Physiol 4: 29–42, 1883. doi: 10.1113/jphysiol.1883.sp000120. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 133. Ringer S. Concerning the influence exerted by each of the constituents of the blood on the contraction of the ventricle. J Physiol 3: 380–393, 1882. doi: 10.1113/jphysiol.1882.sp000111. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 134. Ringer S. Regarding the action of hydrate of soda, hydrate of ammonia, and hydrate of potash on the ventricle of the frog’s heart. J Physiol 3: 195–202, 1882. doi: 10.1113/jphysiol.1882.sp000095. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 135. Seyfarth EA. Julius Bernstein (1839-1917): pioneer neurobiologist and biophysicist. Biol Cybern 94: 2–8, 2006. doi: 10.1007/s00422-005-0031-y. [DOI] [PubMed] [Google Scholar]
- 136. Hodgkinson A. Plasma electrolyte concentrations in women and the effects of oestrogen administration. Maturitas 4: 247–256, 1982. doi: 10.1016/0378-5122(82)90055-X. [DOI] [PubMed] [Google Scholar]
- 137. Hodgkin AL, Huxley AF, Katz B. Measurement of current‐voltage relations in the membrane of the giant axon of Loligo. J Physiol 116: 424–448, 1952. doi: 10.1113/jphysiol.1952.sp004716. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 138. Hodgkin AL, Huxley AF. A quantitative description of membrane current and its application to conduction and excitation in nerve. J Physiol 117: 500–544, 1952. doi: 10.1113/jphysiol.1952.sp004764. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 139. Schwiening CJ. A brief historical perspective: Hodgkin and Huxley. J Physiol 590: 2571–2575, 2012. doi: 10.1113/jphysiol.2012.230458. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 140. Weidmann S. Electrical constants of trabecular muscle from mammalian heart. J Physiol 210: 1041–1054, 1970. doi: 10.1113/jphysiol.1970.sp009256. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 141. Weidmann S. The electrical constants of Purkinje fibres. J Physiol 118: 348–360, 1952. doi: 10.1113/jphysiol.1952.sp004799. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 142. Weidmann S, Hodgkin AL. The diffusion of radiopotassium across intercalated disks of mammalian cardiac muscle. J Physiol 187: 323–342, 1966. doi: 10.1113/jphysiol.1966.sp008092. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 143. Hoeker GS, James CC, Barrett SH, Smyth JW, Poelzing S. Combined effects of gap junctional and ephaptic coupling therapies on conduction and arrhythmogenesis during ischemia/reperfusion. Biophys J 114: 623a, 2018. doi: 10.1016/j.bpj.2017.11.3368. [DOI] [Google Scholar]
- 144. George SA, Hoeker G, Calhoun PJ, Entz M, Raisch TB, King DR, Khan M, Baker C, Gourdie RG, Smyth JW, Nielsen MS, Poelzing S. Modulating cardiac conduction during metabolic ischemia with perfusate sodium and calcium in guinea pig hearts. Am J Physiol Heart Circ Physiol 316: H849–H861, 2019. doi: 10.1152/ajpheart.00083.2018. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 145. Entz M, George SA, Zeitz MJ, Raisch T, Smyth JW, Poelzing S. Heart rate and extracellular sodium and potassium modulation of gap junction mediated conduction in Guinea pigs. Front Physiol 7: 16–10, 2016. doi: 10.3389/fphys.2016.00016. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 146. George SA, Sciuto KJ, Lin J, Gourdie RG, Poelzing S. Extracellular sodium and potassium levels modulate cardiac conduction in mice heterozygous null for the Connexin43 gene. Pflugers Arch 467: 2287–2297, 2015. doi: 10.1007/s00424-015-1698-0. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 147. George SA, Poelzing S. Cardiac conduction in isolated hearts of genetically modified mice – Connexin43 and salts. Prog Biophys Mol Biol 120: 189–198, 2016. doi: 10.1016/j.pbiomolbio.2015.11.004. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 148. Hoeker GS, James CC, Tegge AN, Gourdie RG, Smyth JW, Poelzing S. Attenuating loss of cardiac conduction during no-flow ischemia through changes in perfusate sodium and calcium. Am J Physiol Heart Circ Physiol 319: H396–H409, 2020. doi: 10.1152/ajpheart.00112.2020. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 149. King DR, Padget RL, Perry J, Hoeker G, Smyth JW, Brown DA, Poelzing S. Elevated perfusate [Na+] increases contractile dysfunction during ischemia and reperfusion. Sci Rep 10: 17289, 2020. doi: 10.1038/s41598-020-74069-x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 150. Wu X, Hoeker GS, Blair GA, King DR, Gourdie RG, Weinberg SH, Poelzing S. Hypernatremia and intercalated disc edema synergistically exacerbate long-QT syndrome type 3 phenotype. Am J Physiol Heart Circ Physiol 321: H1042–H1055, 2021. doi: 10.1152/ajpheart.00366.2021. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 151. King DR, Entz M, Blair GA, Crandell I, Hanlon AL, Lin J, Hoeker GS, Poelzing S. The conduction velocity-potassium relationship in the heart is modulated by sodium and calcium. Pflugers Archiv 473: 557–571, 2021. doi: 10.1007/s00424-021-02537-y. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 152. Gaskell WH. On the tonicity of the heart and blood vessels. J Physiol 3: 48–92, 1880. doi: 10.1113/jphysiol.1880.sp000083. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 153. Poole-Wilson PA. Acidosis and contractility of heart muscle. Ciba Found Symp 87: 58–76, 1982. doi: 10.1002/9780470720691.ch4. [DOI] [PubMed] [Google Scholar]
- 154. Noori S, Wu TW, Seri I. PH effects on cardiac function and systemic vascular resistance in preterm infants. J Pediatr 162: 958–963.e1, 2013. doi: 10.1016/j.jpeds.2012.10.021. [DOI] [PubMed] [Google Scholar]
- 155. Kagiyama Y, Hill JL, Gettes LS. Interaction of acidosis and increased extracellular potassium on action potential characteristics and conduction in guinea pig ventricular muscle. Circ Res 51: 614–623, 1982. doi: 10.1161/01.RES.51.5.614. [DOI] [PubMed] [Google Scholar]
- 156. Mitchell JH, Wildenthal K, Johnson RL, Pauline J. The effects of acid-base disturbances on cardiovascular and pulmonary function. Kidney Int 1: 375–389, 1972. doi: 10.1038/ki.1972.48. [DOI] [PubMed] [Google Scholar]
- 157. Aberra A, Komukai K, Howarth FC, Orchard CH. The effect of acidosis on the ECG of the rat heart. Exp Physiol 86: 27–31, 2001. doi: 10.1113/eph8602051. [DOI] [PubMed] [Google Scholar]
- 158. Orchard CH, Kentish JC. Effects of changes of pH on the contractile function of cardiac muscle. Am J Physiol Cell Physiol 258: C967–C981, 1990. doi: 10.1152/ajpcell.1990.258.6.C967. [DOI] [PubMed] [Google Scholar]
- 159. Nisbet AM, Burton FL, Walker NL, Craig MA, Cheng H, Hancox JC, Orchard CH, Smith GL. Acidosis slows electrical conduction through the atrio-ventricular node. Front Physiol 5: 233, 2014. doi: 10.3389/fphys.2014.00233. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 160. Orchard CH, Cingolani HE. Acidosis and arrhythmias in cardiac muscle. Cardiovasc Res 28: 1312–1319, 1994. doi: 10.1093/cvr/28.9.1312. [DOI] [PubMed] [Google Scholar]
- 161. Shapiro JI. Functional and metabolic responses of isolated hearts to acidosis: effects of sodium bicarbonate and Carbicarb. Am J Physiol Heart Circ Physiol 258: H1835–H1839, 1990. doi: 10.1152/ajpheart.1990.258.6.H1835. [DOI] [PubMed] [Google Scholar]
- 162. Cheng H, Smith GL, Orchard CH, Hancox JC. Acidosis inhibits spontaneous activity and membrane currents in myocytes isolated from the rabbit atrioventricular node. J Mol Cell Cardiol 46: 75–85, 2009. doi: 10.1016/j.yjmcc.2008.09.709. [DOI] [PubMed] [Google Scholar]
- 163. Hughes JC, Tyers GF, Torman HA. Effects of acid-base imbalance on myocardial pacing thresholds. J Thorac Cardiovasc Surg 69: 743–746, 1975. doi: 10.1016/S0022-5223(19)41509-2. [DOI] [PubMed] [Google Scholar]
- 164. Meijles DN, Fuller SJ, Cull JJ, Alharbi HO, Cooper STE, Sugden PH, Clerk A. The insulin receptor family and protein kinase B (Akt) are activated in the heart by alkaline pH and α1-adrenergic receptors. Biochem J 478: 2059–2079, 2021. doi: 10.1042/BCJ20210144. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 165. Lagadic-Gossmann D, Buckler KJ, Vaughan-Jones RD. Role of bicarbonate in pH recovery from intracellular acidosis in the guinea-pig ventricular myocyte. J Physiol 458: 361–384, 1992. doi: 10.1113/jphysiol.1992.sp019422. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 166. Terzic A, Pucéat M, Clément-Chomienne O, Vassort G. Phenylephrine and ATP enhance an amiloride insensitive bicarbonate-dependent alkalinizing mechanism in rat single cardiomyocytes. Naunyn Schmiedebergs Arch Pharmacol 346: 597–600, 1992. doi: 10.1007/BF00169019. [DOI] [PubMed] [Google Scholar]
- 167. Khandoudi N, Albadine J, Robert P, Krief S, Berrebi-Bertrand I, Martin X, Bevensee MO, Boron WF, Bril A. Inhibition of the cardiac electrogenic sodium bicarbonate cotransporter reduces ischemic injury. Cardiovasc Res 52: 387–396, 2001. doi: 10.1016/S0008-6363(01)00430-8. [DOI] [PubMed] [Google Scholar]
- 168. Aalkjaer C, Boedtkjer E, Choi I, Lee S. Cation-coupled bicarbonate transporters. Compr Physiol 4: 1605–1637, 2014. doi: 10.1002/cphy.c130005. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 169. Bauza G, Le Moyec L, Eugène M. pH regulation during ischaemia-reperfusion of isolated rat hearts, and metabolic effects of 2,3-butanedione monoxime. J Mol Cell Cardiol 27: 1703–1713, 1995. doi: 10.1016/S0022-2828(95)90821-8. [DOI] [PubMed] [Google Scholar]
- 170. Bers DM, Barry WH, Despa S. Intracellular Na+ regulation in cardiac myocytes. Cardiovasc Res 57: 897–912, 2003. doi: 10.1016/s0008-6363(02)00656-9. [DOI] [PubMed] [Google Scholar]
- 171. Wilson TE, Crandall CG. Effect of thermal stress on cardiac function. Exerc Sport Sci Rev 39: 12–17, 2011. doi: 10.1097/JES.0b013e318201eed6. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 172. Ranjan R, Logette E, Marani M, Herzog M, Tâche V, Scantamburlo E, Buchillier V, Markram H. A kinetic map of the homomeric voltage-gated potassium channel (Kv) family. Front Cell Neurosci 13: 358, 2019. doi: 10.3389/fncel.2019.00358. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 173. Reeves RB. Temperature-induced changes in blood acid-base status: pH and PCO2 in a binary buffer. J Appl Physiol 40: 752–761, 1976. doi: 10.1152/jappl.1976.40.5.752. [DOI] [PubMed] [Google Scholar]
- 174. Delory GE, King EJ. A sodium carbonate-bicarbonate buffer for alkaline phosphatases. Biochem J 39: 245, 1945. [PubMed] [Google Scholar]
- 175. Templeton GH, Wildenthal K, Willerson JT, Reardon WC. Influence of temperature on the mechanical properties of cardiac muscle. Circ Res 34: 624–634, 1974. doi: 10.1161/01.res.34.5.624. [DOI] [PubMed] [Google Scholar]
- 176. Shah U, Bien H, Entcheva E. Cardiac arrhythmogenesis and temperature. Conf Proc IEEE Eng Med Biol Soc 2006: 841–844, 2006. doi: 10.1109/IEMBS.2006.260090. [DOI] [PubMed] [Google Scholar]
- 177. Jacobs HK, South FE. Effects of temperature on cardiac transmembrane potentials in hibernation. Am J Physiol 230: 403–409, 1976. doi: 10.1152/ajplegacy.1976.230.2.403. [DOI] [PubMed] [Google Scholar]
- 178. Vostarek F, Svatunkova J, Sedmera D. Acute temperature effects on function of the chick embryonic heart. Acta Physiol (Oxf) 217: 276–286, 2016. doi: 10.1111/apha.12691. [DOI] [PubMed] [Google Scholar]
- 179. Kim DH, Sreter FA, Ohnishi ST, Ryan JF, Roberts J, Allen PD, Meszaros LG, Antoniu B, Ikemoto N. Kinetic studies of Ca2+ release from sarcoplasmic reticulum of normal and malignant hyperthermia susceptible pig muscles. Biochim Biophys Acta 775: 320–327, 1984. doi: 10.1016/0005-2736(84)90187-1. [DOI] [PubMed] [Google Scholar]
- 180. Lindsey ML, Bolli R, Canty JM, Du X-J, Frangogiannis NG, Frantz S, Gourdie RG, Holmes JW, Jones SP, Kloner RA, Lefer DJ, Liao R, Murphy E, Ping P, Przyklenk K, Recchia FA, Schwartz Longacre L, Ripplinger CM, Van Eyk JE, Heusch G. Guidelines for experimental models of myocardial ischemia and infarction. Am J Physiol Heart Circ Physiol 314: H812–H838, 2018. doi: 10.1152/ajpheart.00335.2017. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 181. Lindsey ML, de Castro Brás LE, DeLeon-Pennell KY, Frangogiannis NG, Halade GV, O'Meara CC, Spinale FG, Kassiri Z, Kirk JA, Kleinbongard P, Ripplinger CM, Brunt KR. Reperfused vs. nonreperfused myocardial infarction: when to use which model. Am J Physiol Heart Circ Physiol 321: H208–H213, 2021. doi: 10.1152/ajpheart.00234.2021. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 182. Lindsey ML, Kassiri Z, Virag JAI, de Castro Brás LE, Scherrer-Crosbie M. Guidelines for measuring cardiac physiology in mice. Am J Physiol Heart Circ Physiol 314: H733–H752, 2018. doi: 10.1152/ajpheart.00339.2017. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 183. Quinn TA, Granite S, Allessie MA, Antzelevitch C, Bollensdorff C, Bub G, et al. . Minimum information about a cardiac electrophysiology experiment (MICEE): standardised reporting for model reproducibility, interoperability, and data sharing. Prog Biophys Mol Biol 107: 4–10, 2011. doi: 10.1016/j.pbiomolbio.2011.07.001. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 184. Odening KE, Gomez A-M, Dobrev D, Fabritz L, Heinzel FR, Mangoni ME, Molina CE, Sacconi L, Smith G, Stengl M, Thomas D, Zaza A, Remme CA, Heijman J. ESC working group on cardiac cellular electrophysiology position paper: relevance, opportunities, and limitations of experimental models for cardiac electrophysiology research. Europace 23: 1795–1814, 2021. doi: 10.1093/europace/euab142. [DOI] [PMC free article] [PubMed] [Google Scholar]

