While ryanodine receptor 1 (RyR1) critically contributes to skeletal muscle contraction abilities by mediating Ca2+ion oscillation between sarcoplasmatic and myofibrillar compartments, AMP-activated protein kinase (AMPK) senses contraction-induced energetic stress by phosphorylation at Thr172. Phosphorylation of RyR1 at serine2843 (pRyR1Ser2843) results in leaky RyR1 channels and impaired Ca2+homeostasis. Because acute resistance exercise exerts decreased contraction performance in skeletal muscle, preceded by high rates of Ca2+-oscillation and energetic stress, intense myofiber contractions may induce increased RyR1 and AMPK phosphorylation. However, no data are available regarding the time-course and magnitude of early RyR1 and AMPK phosphorylation in human myofibers in response to acute resistance exercise.
Determine the effects and early time-course of resistance exercise on pRyR1Ser2843 and pAMPKThr172 in type I and II myofibers.
7 male subjects (age 23±2 years, height: 185±7 cm, weight: 82±5 kg) performed 3 sets of 8 repetitions of maximum eccentric knee extensions. Muscle biopsies were taken at rest, 15, 30 and 60 min post exercise. pRyR1Ser2843 and pAMPKThr172 levels were determined by western blot and semi-quantitative immunohistochemistry techniques.
While total RyR1 and total AMPK levels remained unchanged, RyR1 was significantly more abundant in type II than type I myofibers. pRyR1Ser2843 increased 15 min and peaked 30 min (p<0.01) post exercise in both myofiber types. Type I fibers showed relatively higher increases in pRyR1Ser2843 levels than type II myofibers and remained elevated up to 60 min post resistance exercise (p<0.05). pAMPKThr172 also increased 15 to 30 min post exercise (p<0.01) in type I and II myofibers and in whole skeletal muscle.
Resistance exercise induces acutely increased pRyR1Ser2843 and concomitantly pAMPKThr172 levels for up to 30 min in resistance exercised myofibers. This provides a time-course by which pRyR1Ser2843 can mechanistically impact Ca2+handling properties and consequently induce reduced myofiber contractility beyond immediate fatiguing mechanisms.
Citation: Gehlert S, Bungartz G, Willkomm L, Korkmaz Y, Pfannkuche K, Schiffer T, et al. (2012) Intense Resistance Exercise Induces Early and Transient Increases in Ryanodine Receptor 1 Phosphorylation in Human Skeletal Muscle. PLoS ONE 7(11): e49326. https://doi.org/10.1371/journal.pone.0049326
Editor: Petras Dzeja, Mayo Clinic, United States of America
Received: June 10, 2012; Accepted: October 10, 2012; Published: November 16, 2012
Copyright: © 2012 Gehlert et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This investigation was funded by the Federal Institute of Sports Science (BISp) IIA1-507 070103/09-10. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Human skeletal muscle tissue represents the vital organ for human locomotion. As such, it exerts a high plasticity to adapt to various modes of exercise . For example, intense contractions of myofibers (as occurs during exercise) initially result in gradually decreased skeletal muscle contraction properties, including acutely reduced myofiber contractility, which occurs already after few seconds of high intense exercise , . More importantly, intense exercise also induces sustained alterations in skeletal muscle contractility that last up to several min post exercise , . This phenomenon is described as the slow recovery curve of myocellular fatigue  in which a sustained increase in relaxation time between periodic contractions of myofibers can be observed . The molecular mechanisms contributing to these phenomena are still a matter of debate . However, calcium (Ca2+) plays a fundamental role in the onset of skeletal muscle fatigue , , ,  because its oscillation in myofibrillar areas links sarcolemma depolarization to muscle contraction, which is also known as excitation-contraction (EC) coupling . The ryanodine receptor 1 (RyR1) channel complex is mainly involved in facilitating the accurate release of Ca2+from sarcoplasmic compartments into myofibrillar areas and triggers the important calcium oscillation that is required for continued myofiber contractions. RyR1 has been observed to be posttranslationally modified at several residues, predominantly by phosphorylation at serine2843 (pRyR1Ser2843) . This modification contributes critically towards skeletal muscle contraction impairment upon exercise as it destabilizes the closed state of RyR1, thereby increasing the ratio of open channels , , which, consequently, facilitate uncontrolled Ca2+release and inaccurate distribution of Ca2+ions in myofiber compartments , . Bellinger and co-workers determined that chronic exercise in a mouse model results in increased phosphorylation of RyR1 on Ser2843 and, consequently, impaired skeletal muscle contractility . Additionally, total RyR1 levels in human skeletal muscle have been found to decrease in response to bed rest and increase due to long term exercise . However, to date, no data are available concerning the acute phosphorylation level of RyR1 in response to exercise. Increased RyR1 phosphorylation is likely to occur in response to acute and severe resistance exercise as this exercise mode requires a high rate of Ca2+-oscillation and induces stress within myofibers. RyR1 phosphorylation might have an impact on Ca2+handling structures, transiently increased Ca2+levels and also on kinases relevant for mediating its own phosphorylation. Thus, an early increase in RyR1 phosphorylation after exercise could potentially provide a subtle cellular indicator for impaired Ca2+handling properties in a sensitive recovery period after exercise without affecting general myofiber contractility. Therefore, we hypothesized that increased phosphorylation of RyR1 at Ser2843 will be observed in an early and transient time-course in response to high intense resistance exercise in human skeletal muscle. ATP-dependent ion channels and myosin ATPase enzymes exert high rates of ATP turnover and, thus, energetic stress  in contracting myofibers, which consequently induces increased phosphorylation of AMP-activated protein kinase (AMPK). Because this emphasizes a contraction-induced effect, we further postulated that exercise-induced phosphorylation of RyR1 is accompanied by elevated pAMPKThr172 levels, indirectly indicating that increased pRyR1Ser2843 results from myofiber contractions.
Type I and type II myofibers show distinct mechanic and metabolic properties and offer different recruitment patterns during exercise. A distinct recruitment of type I and II myofibers in response to exercise , ,  may induce a different load on these myofibers. This may consequently lead to different magnitudes of stress on downstream effectors which mediate the molecular bases for cellular signaling  and EC coupling . Thus, we hypothesized that type I and II myofibers would present with differences in pRyR1Ser2843 and pAMPKThr172 levels in response to exercise, as would individual fibers within each myofiber population due to unequal recruitment of fibers in exercising skeletal muscle.
A model of maximum eccentric leg extensions on human subjects was used to apply high intense muscular workload. Here, we show that pRyR1Ser2843 and pAMPKThr172 levels increase significantly in an early and transient manner in both type I and type II myofibers 15 to 30 min post exercise. These data are highly significant as they describe the fiber type-specific response of RyR1 phosphorylation in response to acute exercise bouts and beyond.
Materials and Methods
7 healthy active, but not exceptionally resistance- or endurance-trained, male volunteers (age: 23±2 years, height: 185±7 cm, and weight: 82±5 kg) participated in the present study. All subjects were informed orally and in writing of the study’s purpose and the possible risks involved before providing written informed consent to participate. The study was approved by the Ethic Committee of the German Sport University Cologne in compliance with the Declaration of Helsinki. Dates and times of exercise and muscle biopsies were documented for each subject. Subjects were assigned an anonymous ID during the study.
Standardization of Diet and Activity before Testing
Subjects were instructed to refrain from vigorous physical activity two days prior to baseline biopsies as well as prior the main stimulus. After fasting overnight, the subjects were advised to drink one standardized energy drink (Fresubin® protein energy drink, Fresenius Kabi Deutschland GmbH, Bad Homburg, Germany; containing 20 g protein, 24.8 g carbohydrate 13.4 g fat, and providing 1260 kJ) two hours prior the training intervention to carry out training in the fed state. Subjects were allowed to drink water ad libitum.
On the day of the main trial, subjects reported to the laboratory at 07:45 AM. Prior to the resistance exercise bouts, a 5 min warm-up with a workload of 1 W*kg–1 on a cycle ergometer was carried out. A combined warm-up and main exercise program was carried out subsequently on an isokinetic leg extension machine. The program was automatically operated by the control unit of the isokinetic device. Range of motion, angle velocity, as well as resting time between exercise sets were equalized for each subject. The first phase featured 3 sets of 4 submaximal (30% of maximum force) concentric and eccentric repetitions and 90 sec resting intervals between the sets. The angular velocity was determined by 65°*sec–1 movement speed in concentric and eccentric phases. After a 3 min resting phase, the main stimulus was applied featuring 3 sets of 8 maximal eccentric repetitions with a 3 min rest between the sets. The angular velocity during the eccentric contraction phase was carried out at 25°*sec–1. The leg was passively returned to the extended knee position over the concentric phase to the starting position with an angular velocity of 75°*sec–1. All subjects were verbally encouraged during the exercise session to perform all 24 contractions with maximum force. The exercise regimen induced approximately 70 sec of maximum eccentric force on skeletal muscle.
After the exercise was completed, subjects walked a short distance (≈ 250 m) to the local outpatient clinic of the German Sport University Cologne. After a local anesthesia was applied to the vastus lateralis at its incision, muscle biopsies were collected from the exercised leg.
To prevent potential injury due to damaged muscle tissue under maximum eccentric contractions, baseline biopsies of the vastus lateralis muscle were taken at rest 5 days prior the exercise intervention. On the day of the experimental trial, biopsies were collected 15 min, 30 min and 60 min post exercise. The 3 biopsies were taken 2 cm distal from each other starting 2 cm distal of the resting biopsy. Muscle biopsies were obtained from the middle region of the vastus lateralis between the spina iliaca anterior superior and the lateral part of the patella. Biopsies were gathered 2.5 cm below the fascia using the percutaneous needle biopsy technique .
Muscle samples were freed from blood and non-muscle material, embedded in Tissue-Tek (Sakura Finetek, Zoeterwoude, Netherlands), frozen in liquid nitrogen-cooled isopentane and stored at −80°C. For immunohistochemical analyses, 7 µm cross sections of all biopsy time points were mounted in triplicates on Polysine® slides (VWR International GmbH, Darmstadt, Germany), aligned carefully for cross-sectional analysis, air-dried and stored at −80°C until further analysis.
Immunohistochemical Staining and Analysis of pRYR1 Ser2843 and pAMPKThr172
Immunohistochemical analysis was conducted as described previously . Cryo-sections were brought to room temperature and subsequently incubated for 10 min at 37°C. Sections were fixed for 5 min in −20°C pre-cooled acetone. Sections were blocked in TBS containing 5% BSA for 1 hour at room temperature. Slides were then incubated overnight at 4°C with monoclonal primary phospho-specific antibodies. Antibodies recognizing phosphorylated RyR1Ser2843, (Abcam, Cambrigde, UK) , , total RyR1 (Abcam, Cambridge, UK), phosphorylated AMPKThr172 (Cell Signaling, Beverly MA, USA), total AMPK (Cell Signaling, Beverly, MA, USA) and A4.840 (Developmental Studies Hybridoma Bank, Iowa City, USA), which is raised against adult human slow myosin heavy chain type 1 (MyHC1), were used. Antibodies were diluted 1∶200 (rabbit pRyR1Ser2843 and total RyR1), 1∶100 (rabbit pAMPKThr172 and total AMPK) or 1∶300 (mouse A4.840) in TBS containing 0.8% BSA. Slides were rinsed 5 times for 5 min each with TBS and then incubated for 1 hour with appropriate polyclonal biotinylated secondary antibodies (DakoCytomation, Glostrup, Denmark) diluted 1∶400 in TBS. Negative controls were processed in the same way as the experimental cross-sections; however, primary antibody incubations were substituted by incubation with 0.8% TBS. Thereafter, slides were incubated for 1 hour with Streptavidin biotinylated Horseradish Peroxidase complex (Amersham Biosciences, Uppsala, Sweden) diluted 1∶400 in TBS. After rinsing, staining was carried out using a 3,3`-diaminobenzidine (DAB) solution (0.09 M phosphate buffer (pH 7.4), 2.2 mM DAB, 7.03 mM ammonium chloride, 0.93 mM nickel sulfate, 10.44 mM ß-D-glucose and 0.000024 mM glucose oxidase). After dehydration, the stained sections were embedded in Entellan (Merck, Darmstadt, Germany) and supplied with a coverslip. Muscle cross sections from all biopsy time points of 1 subject were stained within a single batch using the same antibody dilution and development time to minimize variability in staining efficiency. Duplicate mounted serial sections of each time point were stained on a single slide for MyHC1 with the monoclonal A4.840 and polyclonal pRyR1Ser2843 antibodies as well as for pRyR1Ser2843 and pAMPKThr172. The intensity of myofibrillar staining for pRyR1Ser2843 and pAMPKThr172 was determined separately for type I and type II myofibers. Additionally, myofiber type-specific levels of total RyR1 and total AMPK were determined separately for each time point. pRyR1Ser2843 and pAMPKThr172 localized specifically to type I and type II myofibers as did total RyR1 and total AMPK.
Staining of pRyR1Ser2843 and pAMPKThr172 was additionally carried out in identical myofibers to determine the impact of exercise on both parameters in single myofibers. All slides were examined with a Zeiss Axiophot 200 light microscope coupled to a Sony 3CCD Color Video Camera. The background intensity was equalized for each slide and subject prior to image capturing. Differences in staining intensity between time points were determined as the difference between background intensity and measured sarcoplasmic intensity. Digitally captured images (200x magnification) were analyzed to determine the fiber type. To determine the fiber type-specific phosphorylation pattern in the sarcoplasmic compartment of myofibers, pAMPKThr172- and pRyR1Ser2843-stained cross sections were compared to the consecutive area, showing the corresponding type I and II myofiber distributions. The specific staining intensity was quantified for each myofiber by selection of the sarcoplasmic region of the myofiber and its subsequent assessment by optical densitometry using the software ImageJ® (National Institutes of Health, USA). Intracellular pRyR1Ser2843 and pAMPKThr172 content was set as the mean staining intensity. 70±6 myofibers per biopsy time point and subject were analyzed for fiber type-specific pRyR1Ser2843 and pAMPKThr172 signals.
Tissue was prepared as described under “Immunohistochemical Analysis”. The following primary antibodies were used: mouse α-actinin (Sigma-Aldrich, Steinheim, Germany; dilution 1∶250) and rabbit pRyR1Ser2843 (Abcam, Cambridge, UK; dilution 1∶100). The following secondary fluorescent antibodies were used: goat anti-mouse Alexa488 (Invitrogen, Karlsruhe, Germany; dilution 1∶500) and goat anti-rabbit Alexa555 (Invitrogen, Karlsruhe, Germany; dilution 1∶500). Pictures were taken using a Zeiss confocal laser scanning microscope equipped with a Plan-Neofluar 40x/1.3 Oil DIC objective (LSM 510Meta, Zeiss, Jena, Germany). Alexa488 was exited by an Argon laser and detected using the filter set BP505-530. Alexa555 was exited by a Neon laser and detected using the filter set BP565-615.
20 mg of muscle tissue was homogenized in ice-cold lysis buffer (Cell Signaling, Boston, U.S.A.) using a commercially available micro-dismembrator (Braun, Melsungen, Germany) and stored at –80°C for further analysis. The protein content of each homogenate was determined by the Lowry test kit (BioRad, Munich, Germany). 30 µg of homogenate protein was thawed on ice, suspended in buffer (0.5 M Tris-HCl, 10% glycerol, 2% sodium dodecyl sulphate, 5% 2-mercaptoethanol, and 0.05% bromophenolblue), and heated at 95°C for 5 min. Tissue proteins were separated on a 6% acrylamide self-casted minigel using a gel casting system (PerfectBlue Vertical Double Gel Systems, Twin S, PeqLab, Erlangen, Germany) in Tris-glycine electrophoresis buffer (0.25 M Tris-HCl, 1.92 M glycine, 1% [w/v] SDS). After electrophoretic separation, proteins were transferred to a polyvinylidene difluoride (PVDF) membrane (BioRad, Munich, Germany) by semidry blotting (65 min at 12 V, 155 mA, and 3 W) using a semidry blotting system (PerfectBlue Semidry Electro Blotter, Sedec S, PeqLab, Erlangen, Germany). The membranes were blocked in 5% low-fat milk for 75 min. Afterwards, membranes were washed with Tris-buffered saline containing Tween (150 mM NaCl, 10 mM Tris-HCl, 0.05% Tween 20, pH 7.5). Membranes were incubated overnight at 4°C with rabbit polyclonal total AMPK and phosphorylated AMPKThr172 antibodies (Cell Signaling, Beverly, MA, USA; dilution 1∶1000) total RyR1 and RyR1Ser2843 antibodies (Abcam, Cambridge, UK; dilution 1∶500 total RyR1 and 1∶750 pRyR1 Ser2843). After membrane stripping using commercially available stripping buffer (ThermoScientific, Rockford, U.S.A.), membranes were re-incubated overnight at 4°C with mouse monoclonal anti myosin heavy chain-1 (MyHC1) antibody (A4.951 dilution 1∶2000, DSHB, University of Iowa, U.S.A.). Total RyR1 western blot analysis was performed on separate gels and membranes. Respective secondary antibodies (goat anti-rabbit and goat anti-mouse, dilutions in TBST for both 1∶2000) were purchased from Thermo Scientific (Rockford, U.S.A.) and membranes were incubated for 1 hour at room temperature. Proteins were detected by an enhanced chemo- luminescence assay (ECL Kit, Amersham-Life Science, Buckinghamshire, UK) exposed to X-ray film (Kodak X-OMAT Engineering, Eastman Kodak Co., Rochester, NY). Total RyR1 and MyHC1 served as internal loading controls and pRyR1Ser2843 signals were normalized to total RyR1.
All data are expressed as means ± standard error of means (S.E.M.). A multifactorial ANOVA for repeated measures with the factors ‘time’ and ‘fiber type’ was applied to determine the differences in the phosphorylation pattern of sarcoplasmic RyR1 content over time. In the case of a significant difference between factors, a Bonferroni post-hoc test was applied to locate the differences in fiber type dependent analysis. Tukeys post-hoc analysis was conducted for the western blotting analysis. Statistical significance was set at p<0.05. Linear regressions between variables were assigned using Pearson’s product moment correlation index.
Immunohistochemistry and Localization of RyR1
To demonstrate the pRyR1Ser2843 staining specificity, immunofluorescence and DAB staining was performed, which further verified localization of pRyR1Ser2843 in junctional sarcoplasmic areas. α-actinin (Figure 1A) and pRyR1Ser2843 (Figure 1B) were stained in representative longitudinal cross sections of skeletal muscles. As demonstrated, pRyR1Ser2843 was located in cross striated areas in representative longitudinal skeletal muscle sections of immunofluorescence stained (Figure 1C) and DAB stained (Figure 1E) myofibers. Immunofluorescence staining demonstrates Z-bands (α-actinin) located in the proximal vicinity of junctional sarcoplasmic reticuli (pRyR1Ser2843) surrounding the t-tubuli which are located in the transitional zone of A- and I-bands. The negative control (Figure 1D) demonstrates that the obtained pRyR1Ser2843 signal was specific.
(A) Representative picture of longitudinal arranged myofibers displaying α-actinin staining (Alexa488) and (B) pRyR1Ser2843 staining (Alexa555) (C) Merged picture demonstrates localization of Z-bands (α-actinin, Alexa488) in close vicinity of junctional sarcoplasmic reticuli (pRyR1Ser2843, Alexa555). (D) Myofiber cross-section displaying an unstained negative control without primary antibody (α-actinin and pRyR1Ser2843) incubation. (E) Immunohistochemical DAB staining of pRyR1Ser2843 in longitudinal skeletal muscle sections (63x magnification). Arrows indicate pRyR1Ser2843 localization in cross striated areas.
Determination of Total RyR1 and Total AMPK in Myofibers
Salanova and co-workers  demonstrated that type I myofibers have less total RyR1 than do type II myofibers in human soleus muscle. To determine whether the human vastus lateralis muscle shows a comparable pattern of total RyR1 abundance and whether acute and severe resistance exercise induces changes in total RyR1 levels over the investigated time-course, we studied the levels of total RyR1 by means of immunohistochemistry. As shown in Figure 2D, the abundance of total RyR1 was significantly different between type I and type II myofibers; however, the amount of total RyR1 in the myofiber types did not change over the time-course (Figure 2G). Importantly, type II myofibers were found to have significantly more total RyR1 than type I myofibers (Figure 2G).
Illustration of DAB stained myofiber cross-sections (20x magnification) showing (A) total AMPK, (B) pAMPKThr172 and (C) corresponding MyHC1 staining displaying type I myofibers (black) and type II myofibers (unstained). No fiber type-specific differences in total AMPK were observed; Illustration of DAB stained consecutive myofiber cross-sections showing (D) total RyR1, (E) pRyR1Ser2843 and (F) corresponding MyHC1 staining displaying type I myofibers (black) and type II myofibers (unstained). As displayed in (D, F) total RyR1 density was considerably lower in type I compared to type II myofibers. (G) Assessment of total RyR1 density in type I and II myofibers at baseline, 15 min, 30 min and 60 min post resistance exercise. Type II myofibers displayed significantly higher RyR1 densities than type I myofibers (p<0.01). Total RyR1 did not change over the time-course in type I and II myofibers. *headed bars display significant differences between myofibers types (p<0.01).
It was recently demonstrated  that total AMPK levels do not differ between type I and type II myofibers in human skeletal muscle. Furthermore, the authors did not find any changes in total AMPK levels after exercise . In line with these observations, we did not find any changes in the total amount of AMPK between type I and type II myofibers (Figure 2A), nor did we find any influence of acute resistance exercise on total AMPK levels up to 60 min after exercise (data not shown).
Resistance Exercise-induced Phosphorylation of pRyR1 Ser2843
The differential investigation of pRyR1Ser2843 abundance within type I and type II myofibers was carried out by staining consecutive cross-sections for pRyR1Ser2843 and type I myosin heavy chain (MyHC1). Figure 3A displays pRyR1Ser2843 immunohistochemical staining before exercise and its consecutive MyHC1 stained cross-section showing type I and II myofibers (Figure 3B). Figure 3C shows an increased abundance of pRyR1Ser2843 in stained cross-sections at 30 min post exercise. Figure 3D displays its consecutive cross-section stained for MyHC1. Figure 3E shows the phosphorylation levels of pRyR1Ser2843 in type I and type II myofibers over the time-course from baseline conditions up to 60 min post exercise in relation to total RyR1 levels. At baseline conditions, no fiber type-specific differences in RyR1 phosphorylation levels were detected. As early as 15 min post exercise, significant increases (p<0.01) in pRyR1Ser2843 staining intensity in both fiber types were detected. The RyR1 phosphorylation level in type I and II fibers remained significantly increased (p<0.01) up to 30 min after resistance exercise. pRyR1Ser2843 decreased significantly (p<0.01) 60 min after exercise in comparison to the 15 and 30 min time-points, which showed peak phosphorylation in both myofiber types. pRyR1Ser2843 phosphorylation levels returned to near-baseline levels in type II myofibers, but remained significantly elevated in type I myofibers (p<0.05) at 60 min post resistance exercise.
(A) pRyR1Ser2843-stained myofiber cross-section at baseline (PRE) (20x magnification). (B) Consecutive myofiber cross-section specifically stained for type I MyHC1 (A4.840) assigning type I (dark) and type II (unstained) myofibers. (C) pRyR1Ser2843-stained myofiber cross-section in type I and type II myofibers 30 min post exercise. (D) Consecutive myofiber cross-section of figure 3C displaying type I (dark) and type II (unstained) myofibers (E) Densitometry analysis of pRyR1Ser172 staining in type I and II myofibers cross-sections at baseline as well as 15, 30 and 60 min after resistance exercise. Significantly (p<0.01) increased levels 15 and 30 min post exercise compared to baseline levels in type II (§) and up to 60 min in type I (#) myofibers. (F) Western blotting analysis of pRyR1Ser2843 (n = 7). pRyR1Ser2843 (band size is observed at 270 kDa according to ) was analyzed PRE, 15, 30 and 60 min following exercise in comparison to total RyR1 levels. Myosin heavy chain (MyHC1, 220 kDa) served as an additional internal loading control. (§) pRyR1Ser2843 significantly different towards baseline levels at 15 min (p<0.05) and 30 min (p<0.01) after resistance exercise.
To further confirm the findings that pRyR1Ser2843 levels are significantly increased at 15 and 30 min post exercise, as determined by quantitative immunohistochemistry, western blots were conducted using whole muscle lysates (Figure 3F). The RyR1 complex has a molecular weight of about 565 kDa . However, it was demonstrated that a band around 270 kDa obtained by western blot analysis is specific for skeletal muscle RyR1 , . Total RyR1 (270 kDa) and MyHC1 (220 kDa) served as internal loading controls. Representative examples in Figure 3F show that both total RyR1 and MyHC1 levels remain unchanged within 60 min post resistance exercise. Compared to baseline levels, pRyRSer2843 levels increased considerably at 15 min after resistance exercise (p<0.05), peaking at 30 min post resistance exercise (p<0.01) and returning towards baseline levels at 60 min after exercise.
Resistance Exercise Induced Phosphorylation of pAMPKThr172
All subjects completed 3 sets of 8 repetitions of maximum voluntary eccentric knee extensions. pAMPKThr172, which has been described to show increased activity upon single bouts of resistance exercise , was used as a marker for contraction-induced energetic stress. As shown for pRyR1Ser2843, fiber type-specific pAMPKThr172 levels were determined in consecutive cross-sections of myofibers stained for pAMPKThr172 and MyHC I at baseline (Figure 4A and B) and 30 min post resistance exercise (Figure 4C and D). pAMPKThr172 staining intensities are depicted in relation to total AMPK levels. Fiber type-specific phosphorylation of AMPKThr172 (Figure 4E) showed significantly increased levels 15 min (p<0.01) post exercise, peaking after 30 min (p<0.01) in both myofiber types. By 60 min post exercise, pAMPKThr172 dropped down to baseline levels. Increased pAMPKThr172 levels were confirmed by western blotting in muscle homogenates at both 15 and 30 min post exercise (p<0.05, respectively) (Figure 4F) and confirmed to decrease to baseline levels within 60 min post resistance exercise. These data demonstrate the impact of the applied exercise regime on skeletal muscle cellular stress.
(A) pAMPKThr172-stained myofiber cross-section at baseline (PRE) (20x magnification). (B) Consecutive myofiber cross-section specifically stained for type I MyHC1 (A4.840) assigning type I (dark) and type II (unstained) myofibers. (C) pAMPKThr172-stained myofiber cross-section in type I and type II myofibers 30 min post exercise. (D) Consecutive myofiber cross-section of figure 3 C. (E) Densitometry analysis of pAMPKThr172 staining in type I and II myofibers at baseline as well as 15, 30 and 60 min post resistance exercise. Significantly (p<0.01) increased levels 15 to 30 min post exercise compared to baseline levels in type I (#) and II (§) myofibers. (F) Western blotting analysis (n = 7) of pAMPKThr172 to the respective time points showing significantly increased pAMPKThr172 levels 30 min post exercise (p<0.01) (§).
pRyRSer2843 and pAMPKThr172 Levels in Identical Myofibers
We investigated by immunohistochemical techniques the phosphorylation pattern of pAMPKThr172 (Figure 5A) and pRyR1Ser2843 (Figure 5B) at baseline and 30 min post exercise (Figure 5C and D) in the same myofibers of exercised subjects. The investigation was carried out using multiple consecutive cross sections stained for pAMPKThr172 and pRyR1Ser2843 from biopsies obtained at baseline and 30 min post exercise. Figure 5E depicts the data points obtained from one representative subject showing the combined staining of pAMPKThr172 and pRyR1Ser2843 before and 30 min post resistance exercise. As depicted in Figure 5E, control and exercised myofibers presented a broad range of different intensities of both AMPK and RyR1 phosphorylation within myofibers. It is clear, however, that pRyR1Ser2843 and pAMPKThr172 levels were increased simultaneously in the same myofibers as a consequence of resistance exercise. Hence, the majority of myofibers shifted within 30 min post exercise towards an increased amount of pRyR1Ser2843 (Figure 3E) and also pAMPKThr172 (Figure 4E) phosphorylation compared to baseline levels. Together, these data demonstrate that RyR1 is phosphorylated in the same fibers as AMPK and, therefore, strongly suggest that RyR1 phosphorylation is a direct consequence of resistance exercise.
(A) pAMPKThr172-stained myofiber cross-section at baseline (PRE) (20x magnification). (B) Consecutive myofiber cross-section specifically stained for pRyR1Ser2843 at baseline (C) pAMPKThr172-stained myofiber cross-section 30 min post exercise showing increased staining intensities compared to baseline condition. (D) Consecutive myofiber cross-section of figure 4C showing increased staining intensities compared to baseline. (E) Distribution of combined phosphorylation levels of pAMPKThr172 and pRyR1Ser2843 within a population of single myofibers of one representative subject at baseline and 30 min post exercise. Each data point reflects the values of pAMPKThr172 and pRyR1Ser2843 within a single myofiber to the specified time point. The scatter plot reveals a heterogeneous distribution of combined phosphorylation levels of AMPK and RyR1 within single myofibers at baseline (○). 30 min post exercise the majority of myofibers offered significantly, however gradually increased pAMPKThr172 and pRyR1ASer2843 phosphorylation levels (•).
Ca2+represents an essential ion in skeletal muscle as it primarily mediates the basis of electromechanical coupling in myofibers by its rapid and thorough oscillation between sarcoplasmic and myofibrillar compartments. However, severely contracting skeletal muscle inevitably fatigues in response to an intense workload , which leads to gradually reduced contraction properties of myofibers, lasting from seconds up to several minutes after cessation of exercise. This fatigue reduces the ability to perform repeated exercise bouts within a tight time-course . Several cellular factors contribute to this event, including the regeneration of phosphates , neuronal factors  and Ca2+homeostasis .
The present study investigated acute effects of eccentric resistance exercise on phosphorylation levels of the skeletal muscle Ca2+release channel RyR1. Phosphorylation of RyR1 has been shown to induce “leaky” RyR1 channels , impaired myofibrillar Ca2+handling and, consequently, reduced contraction performance in chronically loaded mouse skeletal muscle. However, the previous data reveal a lack of knowledge regarding the time-course of RyR1 regulation in response to acute high intense exercise and, in particular, concerning whether different myofiber types are affected to different magnitudes. A primary novel finding of this study is that basal RyR1 phosphorylation levels can be rapidly and transiently increased up to 30 min in human myofibers as a response to 70 sec of maximum eccentric contraction and muscular tension.
We hypothesized that the impact of the applied exercise setup would not affect pAMPKThr172 and pRyR1Ser2843 levels to an equal extent in the proportion of type I and II myofibers as skeletal muscle constitutes a heterogeneous tissue in which type I and II myofibers are not consistently recruited during exercise . This fact might affect distinct RyR1 and AMPK phosphorylation levels  within both populations. pRyR1Ser2843 was found to increase significantly in whole skeletal muscle, including both myofiber types. However, relatively higher increases in type I myofibers were observed, which remained elevated up to 60 min post exercise.
To obtain indirect clues for contraction-induced RyR1 phosphorylation, in parallel with the pRyR1Ser2843 studies, we investigated phosphorylation levels of AMPKThr172, which occurs in response to exercise in skeletal muscle . Its phosphorylation is caused by energetic stress due to increased ATP turnover at ATP-dependent ion channels and myosin ATPase enzymes during electromechanical coupling  in myofibers. Here, we determined whether, parallel to elevated pRyR1Ser2843 levels, significant increases in pAMPKThr172 could be seen in type I and II myofibers up to 30 min post resistance. As we indeed did observe parallel increases in phosphorylation, we conclude that the observed raise in pRyR1Ser2843 levels occurred as a response to myofiber contraction. Despite a heterogeneous range of co-regulation of pAMPKThr172 and pRyR1Ser2843 within the investigated myofiber population (Figure 5E), we surmise that, 30 min after exercise, the parallel increase of both parameters within identical myofibers (Figure 5A–D) reflects a contraction-induced event. We speculate that the observed heterogeneity is due to distinct activity levels of motoneurons at rest and during exercise . Indeed, AMPK and RyR1 phosphorylation can be triggered in response to exercise-induced stress , ; but it remains unclear whether they directly relate to each other at the molecular level. However, due to the observed paralleled changes in pAMPKThr172 and pRyR1Ser2843 in the current study, the co-regulation of both molecules, especially those lying in spatial vicinity to each other might be expected. Thus, it will be of future interest to determine whether exercise-induced regulation of AMPK and RyR1 in skeletal muscle myofibers is particularly occurring locally, in mechanically and energetically stressed environment.
Increased AMPK phosphorylation has recently been shown to occur in both myofiber types up to 120 min following endurance exercise . However, the metabolic and mechanical impact of 70 sec of maximum eccentric contractions differs considerably from extended endurance exercise , which might have contributed to the shorter time-course of increased pAMPKThr172 in the present study. Because AMPK phosphorylation reflects a direct response to contraction-induced energetic turnover , this strongly suggests a broad contraction involvement of both type II an especially, type I myofibers in the present study. The observed increase in pRyR1Ser2843 takes place in a time-course corresponding to that of AMPKThr172 phosphorylation and shows a relatively higher increase in type I compared to type II myofibers up to 60 min post exercise. Our results emphasize the overall higher impact of the applied exercise regimen on type I myofibers. However, besides the observed changes in total RyR1 levels in response to unloading or chronic overload , no data are available concerning fiber type-specific responses of RyR1 phosphorylation in response to acute exercise. Our data provide evidence that the observed responses of transiently elevated RyR1 phosphorylation levels within myofibers reflect the impact of strenuous exercise on RyR1 channels within myofibers. Importantly, this can reveal differences in stress-induced regulation of structures involved in Ca2+handling in functionally distinct myofiber types. However, molecular differences concerning RyR1 regulation within human myofibers may exist, which to date are not known. This might include a different density of kinases within type I and II myofibers that contribute to RyR1 phosphorylation, e.g CAMKII and PKA, as well as responsible phosphatases that mediate its de-phosphorylation ; this would affect the time-course of increased RyR1 phosphorylation in myofibers regardless of any load dependent properties of myofiber types. Thereby, it might be speculated and should be considered in future studies that the observed pRyR1Ser2843 elevations are likely be driven by acute activations of CaMKII at Thr286 and more importantly by the formation of the catalytic subunit of protein kinase A (PKAc), as both kinases are activated upon acute exercise stimulations , .
Our data, combined with the described impact of RyR1 phosphorylation on Ca2+handling properties by Bellinger and co-workers , suggest that RyR1 phosphorylation is increased in response to intense resistance exercise, contributing to a sustained reduction in contraction properties up to 30 min after exercise. This time-course corresponds to a slow recovery period after intense myofiber contractions in which a reduction in myofiber contractility and relaxation ability has been observed , . This phenomenon is decidedly one of the most important effects of RyR1 phosphorylation , although its phosphorylation has not been linked to the post exercise recovery period after fatiguing muscle contractions.
This is the first study showing the kinetics of increased pRyR1Ser2843 after resistance exercise in humans. Our data adds important knowledge regarding the time-course of RyR1 phosphorylation and, importantly, to a time-dependent and partly distinct response in subpopulations of type I and type II myofibers. However, as the difference in RyR1 phosphorylation between fiber types was found to be significant only at the 60 min post exercise time-point, further subpopulation exercise-based studies are needed. Replication of these findings is important as knowing that distinct myofibers may differ in their susceptibility to RyR1 phosphorylation in response to exercise. This what can have considerable impact on the behavior of competing athletes.
The current study does not link the impact of RyR1 phosphorylation within myofibers to decreased myofiber contractility, as multiple biopsies made the investigation of contraction abilities impossible to the investigated time points. However, the current results do extend the known mechanism of RyR1 phosphorylation. Until now, RyR1 phosphorylation has been solely investigated under chronic loading at an early and transient time period after exhausting exercise in human skeletal muscle. Combined approaches, such as EMG derivations, strength testing and multiple biopsies, are needed to investigate the extent to which increased RyR1 phosphorylation alters the contraction abilities of myofibers in general and following repeated training bouts within short recovery periods after exercise. Knowing this time-course would crucially affect a broad spectrum of training behaviors. It will be important to determine whether RyR1 modification can be altered by changes in physical activity between single bouts of exercise. Besides affecting myofiber contractility, pRyR1Ser2843-mediated changes in sarcoplasmatic Ca2+levels may also offer an important function in exercise-induced Ca2+signaling, as elevated sarcoplasmic Ca2+levels may trigger enhanced Ca2+binding to its targets, including NFAT, Calcineurin and CaMKIV . These factors influence the modulation of myofiber plasticity, e.g. activity-induced myofiber shifting  or mitochondrial biogenesis , and thus emphasize their importance for exercising skeletal muscle. As each exercise bout induces a transient increase in intracellular Ca2+levels, it can be speculated that RyR1Ser2843 phosphorylation might also contribute indirectly to early Ca2+-induced signaling and, thus, be important for skeletal muscle micro-adaptations.
The present study indicates that 70 sec of maximum eccentric exercise induces transiently increased phosphorylation levels of pRyR12843, up to 30 min post exercise, in human type I and II skeletal myofibers. These results provide a sensitized time period in which pRyR1Ser2843 can exert a sustained impact on impaired calcium handling properties. This may affect skeletal muscle contraction performance of critically preloaded myofibers in sports beyond immediate fatiguing mechanisms. pRyR1Ser2843 may further provide a marker to detect subtle disturbances in skeletal muscle myofiber performance.
The authors are grateful to Kathryn D. Rogers for critically reading the manuscript. The authors thank Katharina Hermanns (Institute of Cardiovascular Research and Sport Medicine, Department of Molecular and Cellular Sport Medicine) for expert technical assistance.
Conceived and designed the experiments: SG FS. Performed the experiments: SG LW TS FS. Analyzed the data: SG KP FS. Contributed reagents/materials/analysis tools: YK. Wrote the paper: SG GB WB FS.
- 1. Berchtold MW, Brinkmeier H, Muntener M (2000) Calcium ion in skeletal muscle: its crucial role for muscle function, plasticity, and disease. Physiol Rev 80: 1215–1265.
- 2. Bigland-Ritchie B, Jones DA, Woods JJ (1979) Excitation frequency and muscle fatigue: electrical responses during human voluntary and stimulated contractions. Exp Neurol 64: 414–427.
- 3. Choi SJ, Widrick JJ (2009) Combined effects of fatigue and eccentric damage on muscle power. J Appl Physiol 107: 1156–1164.
- 4. Bigland-Ritchie B, Johansson R, Lippold OC, Smith S, Woods JJ (1983) Changes in motoneurone firing rates during sustained maximal voluntary contractions. J Physiol 340: 335–346.
- 5. Bigland-Ritchie B, Cafarelli E, Vollestad NK (1986) Fatigue of submaximal static contractions. Acta Physiol Scand Suppl 556: 137–148.
- 6. Edwards RH, Hill DK, Jones DA, Merton PA (1977) Fatigue of long duration in human skeletal muscle after exercise. J Physiol 272: 769–778.
- 7. Westerblad H, Lannergren J, Allen DG (1997) Slowed relaxation in fatigued skeletal muscle fibers of Xenopus and Mouse. Contribution of [Ca2+]i and cross-bridges. J Gen Physiol 109: 385–399.
- 8. Allen DG, Lamb GD, Westerblad H (2008) Skeletal muscle fatigue: cellular mechanisms. Physiol Rev 88: 287–332.
- 9. Plaugher G, Hendricks AH (1991) The inter- and intraexaminer reliability of the Gonstead pelvic marking system. J Manipulative Physiol Ther 14: 503–508.
- 10. Westerblad H, Allen DG (1991) Changes of myoplasmic calcium concentration during fatigue in single mouse muscle fibers. J Gen Physiol 98: 615–635.
- 11. Bruton JD, Lannergren J, Westerblad H (1998) Mechanisms underlying the slow recovery of force after fatigue: importance of intracellular calcium. Acta Physiol Scand 162: 285–293.
- 12. Allen DG, Lamb GD, Westerblad H (2008) Impaired calcium release during fatigue. J Appl Physiol 104: 296–305.
- 13. Bellinger AM, Mongillo M, Marks AR (2008) Stressed out: the skeletal muscle ryanodine receptor as a target of stress. J Clin Invest 118: 445–453.
- 14. Bellinger AM, Reiken S, Dura M, Murphy PW, Deng SX, et al. (2008) Remodeling of ryanodine receptor complex causes “leaky” channels: a molecular mechanism for decreased exercise capacity. Proc Natl Acad Sci U S A 105: 2198–2202.
- 15. Betzenhauser MJ, Marks AR (2010) Ryanodine receptor channelopathies. Pflugers Arch 460: 467–480.
- 16. Salanova M, Schiffl G, Rittweger J, Felsenberg D, Blottner D (2008) Ryanodine receptor type-1 (RyR1) expression and protein S-nitrosylation pattern in human soleus myofibres following bed rest and exercise countermeasure. Histochem Cell Biol 130: 105–118.
- 17. Hardie DG (2011) Sensing of energy and nutrients by AMP-activated protein kinase. Am J Clin Nutr 93: 891S–6.
- 18. Sahlin K, Soderlund K, Tonkonogi M, Hirakoba K (1997) Phosphocreatine content in single fibers of human muscle after sustained submaximal exercise. Am J Physiol 273: C172–C178.
- 19. Beltman JG, de Haan A, Haan H, Gerrits HL, van Mechelen W, et al. (2004) Metabolically assessed muscle fibre recruitment in brief isometric contractions at different intensities. Eur J Appl Physiol 92: 485–492.
- 20. Altenburg TM, Degens H, van Mechelen W, Sargeant AJ, de Haan A (2007) Recruitment of single muscle fibers during submaximal cycling exercise. J Appl Physiol 103: 1752–1756.
- 21. Godin R, Ascah A, Daussin FN (2010) Intensity-dependent activation of intracellular signalling pathways in skeletal muscle: role of fibre type recruitment during exercise. J Physiol 588: 4073–4074.
- 22. Bergstrom J (1975) Percutaneous needle biopsy of skeletal muscle in physiological and clinical research. Scand J Clin Lab Invest 35: 609–616.
- 23. Gehlert S, Theis C, Weber S, Schiffer T, Hellmich M, et al. (2010) Exercise-induced decline in the density of LYVE-1-positive lymphatic vessels in human skeletal muscle. Lymphat Res Biol 8: 165–173.
- 24. Munch G, Bolck B, Sugaru A, Brixius K, Bloch W, et al. (2001) Increased expression of isoform 1 of the sarcoplasmic reticulum Ca(2+)-release channel in failing human heart. Circulation 103: 2739–2744.
- 25. Lee-Young RS, Canny BJ, Myers DE, McConell GK (2009) AMPK activation is fiber type specific in human skeletal muscle: effects of exercise and short-term exercise training. J Appl Physiol 107: 283–289.
- 26. Bellinger AM, Reiken S, Carlson C, Mongillo M, Liu X, et al. (2009) Hypernitrosylated ryanodine receptor calcium release channels are leaky in dystrophic muscle. Nat Med 15: 325–330.
- 27. Dreyer HC, Fujita S, Cadenas JG, Chinkes DL, Volpi E, et al. (2006) Resistance exercise increases AMPK activity and reduces 4E-BP1 phosphorylation and protein synthesis in human skeletal muscle. J Physiol 576: 613–624.
- 28. Girard O, Mendez-Villanueva A, Bishop D (2011) Repeated-sprint ability - part I: factors contributing to fatigue. Sports Med 41: 673–694.
- 29. Baker JS, McCormick MC, Robergs RA (2010) Interaction among Skeletal Muscle Metabolic Energy Systems during Intense Exercise. J Nutr Metab 2010: 905612.
- 30. Bigland-Ritchie B, Woods JJ (1984) Changes in muscle contractile properties and neural control during human muscular fatigue. Muscle Nerve 7: 691–699.
- 31. Atherton PJ, Babraj J, Smith K, Singh J, Rennie MJ, et al. (2005) Selective activation of AMPK-PGC-1alpha or PKB-TSC2-mTOR signaling can explain specific adaptive responses to endurance or resistance training-like electrical muscle stimulation. FASEB J 19: 786–788.
- 32. Rose AJ, Kiens B, Richter EA (2006) Ca2+-calmodulin-dependent protein kinase expression and signalling in skeletal muscle during exercise. J Physiol 574: 889–903.
- 33. Chasiotis D (1983) The regulation of glycogen phosphorylase and glycogen breakdown in human skeletal muscle. Acta Physiol Scand Suppl 518: 1–68.
- 34. Chin ER (2004) The role of calcium and calcium/calmodulin-dependent kinases in skeletal muscle plasticity and mitochondrial biogenesis. Proc Nutr Soc 63: 279–286.
- 35. Serrano AL, Murgia M, Pallafacchina G, Calabria E, Coniglio P, et al. (2001) Calcineurin controls nerve activity-dependent specification of slow skeletal muscle fibers but not muscle growth. Proc Natl Acad Sci U S A 98: 13108–13113.
- 36. Wu H, Kanatous SB, Thurmond FA, Gallardo T, Isotani E, et al. (2002) Regulation of mitochondrial biogenesis in skeletal muscle by CaMK. Science 296: 349–352.