SciELO - Scientific Electronic Library Online

vol.39 issue3Increased expression of SNARE proteins and synaptotagmin IV in islets from pregnant rats and in vitro prolactin-treated neonatal islets author indexsubject indexarticles search
Home Pagealphabetic serial listing  

Services on Demand




Related links


Biological Research

Print version ISSN 0716-9760

Biol. Res. vol.39 no.3 Santiago  2006 

Biol Res 39: 567-581, 2006



Modulation by caffeine of calcium-release microdomains in frog skeletal muscle fibers



Department of Physiology, David Geffen School of Medicine, University of California at Los Angeles (UCLA), Los Angeles, CA, USA.

Dirección para Correspondencia


The effects of caffeine on the process of excitation-contraction coupling in amphibian skeletal muscle fibers were investigated using the confocal spot detection technique. This method permits to carefully discriminate between caffeine effects on the primary sources of Ca2+ release at the Z-lines where the triads are located and secondary actions on other potential Ca Release sources. Our results demonstrate that 0.5 mM caffeine potentiates and prolongs localized action-potential evoked Ca2+ transients recorded at the level of the Z-lines, but that 1mM only prolongs them. The effects at both doses are reversible. At the level of the M-line, localized Ca2+ transients displayed more variability in the presence of 1 mM caffeine than in control conditions. At this dose of caffeine, extra-junctional sources of Ca2+ release also were observed occasionally.

Key terms: excitation-contraction coupling, caffeine, confocal spot detection, calcium transients, frog skeletal muscle, calcium microdomains.


Although Eduardo (Guayo) Rojas was the mentor of only one of the authors of this paper (JLV), his reverence for experimental biophysics has been a legacy passed from generation to generation. Thus, it seems fitting that both authors dedicate this article containing unpublished data to Guayo as a modest token of our appreciation for his love for the inherent beauty of the "unexpected."

But before getting into the scientific section of the work, the authors would like to include in this publication a summary of an introduction to a talk presented October 29, 2002 by JLV in La Serena, Chile, on the occasion of a symposium honoring Eduardo's valuable scientific contributions:

"A few days ago, I was interviewed by a group of high-school students who were preparing a video documentary about the Laboratorio de Fisiologia y Biofisica de Montemar, where I had the privilege to work in my Ph.D. thesis. Among the very insightful questions from the students, one of them asked me: What was the impact that the experience at Montemar had on your life as a scientist and as a person? After a prolonged period of reflection (this was not an easy question to answer), I could only come up with only one spontaneous answer: it made my life! Indeed, it made my life, and I would like to share with you the most important reasons why it did so:

First and foremost, it allowed me to meet and to become really close (perhaps too close, almost like siblings) to two people whom I admire deeply, Guayo and Illani. Our life together during those early years in Montemar went far beyond that of the formal, sometimes cold, student-teacher relationship that I had seen in the University before. On the contrary, my life as a graduate student was one of constant argumentation (mostly about scientific matters) with my advisor. Guayo's leadership forced me to really think about issues and to understand that science is to be lived!

The second reason why Montemar made my life is because at an early stage in my career, I lost the fear of the big problems and the big names in science. My Montemar experience, strongly reinforced by Eduardo's irreverence, taught me that only the big problems in science are worth our efforts and that big names are only guys who were there before us. Indeed, Guayo allowed me to corroborate these principles on many occasions. For example, one weekend only three months after my arrival in Montemar, he went to Santiago and left me in charge of hosting none other than Kenneth S. Cole, Robert (Bob) Taylor, Richard D. Keynes, and his wife, Ann. Needless to say, I still have nightmares about my performance in that occasion, but I indeed recognize that it was a crash course in irreverence.

The third reason why the Montemar experience made my life is relevant to this talk [and the paper below]: I came in touch with a scientific problem that has obsessed me since then, the role of the membrane potential on the Ca2+ regulation in muscle".


A critical step in the excitation-contraction (EC) coupling process in skeletal muscle is the release of Ca2+ ions, stored at a high concentration in the lumen of the terminal cisternae (TC) of the sarcoplasmic reticulum (SR), in response to electrical depolarization of the transverse tubular system (Peachey, 1965). The structures supporting this Ca2+ release phase of EC coupling are proposed to be regions of the SR adjacent to the transverse tubule (T-tubule), known as T-SR junctions, where Ca2+ release channels (ryanodine receptor channels, RyR) and voltage sensors (dihydropyridine receptors, DHPRs) are presumed to be linked through protein-protein interactions (Rios and Pizarro, 1991). In frog skeletal muscle fibers, the T-SR junctions are remarkably well aligned with the Z-lines delimiting every sarcomere (Peachey, 1965; Kim and Vergara, 1998). Consequently, it is expected that, in this preparation, action potentials (APs) generate early increases in the Ca2+ concentration ([Ca2+]) at regions of the sarcomere close to the Z-line and smaller and more delayed changes at more remote regions (M-lines).

The localization of the sites of Ca2+ release at the Z-lines was first demonstrated experimentally by Escobar et al. (1994) using a spot detection method and fluorescent Ca2+ indicators. These authors also observed that, in amphibian muscle fibers, the AP-elicited [Ca2+] increase at the M-line was not delayed significantly relative to that at the Z-line (Z-M delay) and proposed that a broad band of the SR may participate in the release process (Escobar et al., 1994). This suggestion was confirmed in experiments that incorporated technical refinements to the spot detection method (DiFranco et al., 2002) and with quantitative modeling of the diffusion-reaction process involved in the Ca2+ redistribution within the sarcomere (Novo et al., 2003). The underlying mechanisms by which Ca2+ ions released from one region of the SR may lead to activation of the release of additional Ca2+ from neighboring regions are not fully understood, but they can, for example, involve the positive feedback process known as Ca-induced Ca2+-release (CICR, Endo et al., 1970; Fabiato and Fabiato, 1975). Since it has been well documented that caffeine is a strong modulator of CICR in several preparations, it seemed appropriate that its effects are studied in the context of localized detection of Ca2+ transients.

Caffeine is an important potentiator of twitch tension in skeletal muscle that operates at concentrations in the millimolar range (Gutmann and Sandow, 1965; Sandow, 1970). The unveiling of the many factors that contribute to this action of the drug has been a topic of intense research and debate in the field of muscle excitation-contraction (EC) coupling during the past 30 years (for a review see Herrmann-Frank et al., 1999). From this literature, it has become apparent that caffeine effects in vivo may be related to the drug's ability to activate ryanodine receptor (RyR) channels in the sarcoplasmic reticulum (SR) of skeletal muscle fibers. However, there is a great discrepancy in the doses of caffeine required for the direct activation of the RyR in vitro (and probably in vivo), which is in the tens of millimolar range (Rousseau et al., 1988; Sitsapesan and Williams, 1990), compared with the more physiological potentiation of Ca2+ release in amphibian muscle fibers, which occurs in the sub-millimolar (up to 1 mM) range (Delay et al., 1986). Without plunging into controversial topics, we want to concentrate our attention on the latter situation (frog fibers, low caffeine doses), in which the following tenets seem to apply: a) there is no substantial effects on the surface membrane or T-tubule electrical properties (Delay et al., 1986); b) there is no detectable increase in the resting free-Ca2+ level in single muscle fibers, as estimated from measurements with Ca2+ electrodes and Ca2+ indicators (Lopez et al., 1983; Delay et al., 1986); c) there is no effect of the force-generating ability of the contractile filaments (Wendt and Stephenson, 1983); d) caffeine potentiation effects on Ca2+ release are mostly reversible upon removal of the drug; and e) there is measurable shift in the voltage dependence of Ca2+ release towards negative potentials (Delay et al., 1986; Shirokova and Rios, 1996). Altogether, these results suggest that low levels of caffeine modulate EC coupling in amphibian skeletal muscle by secondarily enhancing the ability of the SR to release Ca2+, probably by increasing probability of opening of RyR channels (Rousseau et al., 1988), but without affecting the transduction mechanism at the T-SR junction. The purpose of this paper is to investigate the effects of low caffeine concentrations on the spatiotemporal properties of Ca2+ release domains during the physiological activation of the EC coupling process in order to further elucidate this drug's mechanisms of in vivo potentiation.

Preliminary results on the effects of caffeine have been presented elsewhere (Vergara et al., 2001a).


The general methodology and technical improvements of the confocal spot detection system utilized for the experiments presented below have been described extensively elsewhere (Vergara et al., 2001b; DiFranco et al., 2002). We provide here a brief account of the major features of the confocal technique inasmuch as they are required to understand the experimental data.

Muscle fiber preparation and electrophysiological methods

Briefly, segments of cut single fibers from the dorsal head of the semitendinosus muscle from Rana catesbeiana were mounted in an inverted double Vaseline-gap chamber. The fibers were stretched to 3.7-4.5 μm to prevent contraction. Two Vaseline seals isolated three segments of the fiber. The lateral segments were permeabilized with saponin (100 μg/ml; 1-3 min) to allow for free exchange between the lateral pool's solution and the intracellular milieu of the central segment of the fiber. The central pool was perfused continuously with normal Ringer's solution, with or without caffeine, whereas the lateral pools contained internal solution (see below). APs were elicited by supra- threshold current pulses delivered to the muscle fiber through one lateral pool and recorded with a custom-made electronic circuit (DiFranco et al., 1999). The membrane potential of the central segment of the fiber was measured as the potential of the central pool minus the potential of the lateral pool opposite to that used for current injection. APs were filtered at 10 kHz, with an 8-pole Bessel filter (Frequency Devices, Haverhill, MA, USA) and digitized at 25-50 kHz using a PCI-MIO-16XE-10 data acquisition board (National Instruments, Austin, TX, USA).


Ringer's solution: 114 mM NaCl; 2.5 mM KCl; 10 mM MOPS-Na; 1.8 mM CaCl2, 10 mM dextrose. Isotonic high K: 110 mM K2SO4, 10 mM MOPS. Internal solution: 110 mM Aspartate-K; 20 mM MOPS-K; 1 mM MgCl2, 5 mM Na2phosphocreatine, 5 mM K2-ATP, 0.5 or 1 mM EGTA, 0.1 mg/ml Creatine-phosphokinase. The osmolality and pH of the solutions were adjusted to 250 mOsm/kg and 7.0, respectively. Unless otherwise noted, the experiments were performed at 18°C.

Optical setup and stage-scanning system

The optical system was based on an inverted epifluorescence microscope (Model IM, Zeiss, Oberkochen, Germany). In addition to the standard bright-field configuration, it could operate as a stage scanning confocal or standard fluorescence microscope. In confocal mode, the 488 nm line of an Argon laser (Model 95, Lexel, Freemont, CA, USA) was focused onto a 5 µm pinhole (PH-5, Newport Corporation, Irvine, CA, USA). The pinhole image was projected using a 5x objective through the illumination port of the microscope. A 505DRLP dichroic mirror (Omega Optical, Brattleboro, VT, USA) directed the excitation light to a 100x high NA oil immersion objective (Plan Fluor 100, 1.3 NA, Nikon, Japan) that focused it to a 0.8 mm spot on the preparation. The fluorescence image of the illumination spot was collected with the same lens, passed through a 515 nm long-pass emission filter (Omega Optical), and centered on a 50 mm pinhole (04PIP013, Melles Griot, Rochester, NY, USA) used to mask the square active area (200 μm per side) of a PIN photodiode (HR008, United Detector Technology, Hawthorne, CA, USA), which served as the light detector. The photocurrent was amplified using an integrating patch-clamp unit (Axopatch 200B, Axon Instruments, Foster City, CA, USA) and filtered at 2-5 kHz using an 8-pole Bessel filter (Frequency Devices). The optical signal and the AP were acquired simultaneously using the acquisition board described above. A shutter (22510A1S5, Vincent and Associates, Rochester, NY, USA) was used to control the illumination time of the sample.

The experimental chamber and the electronic headstage were mounted on a custom-made microscope stage. Two open-loop motorized drives (860A-2, Newport) were used for coarse movement of the stage in the x- or y-direction (orthogonal to the optical axis of the microscope). In addition, a high-resolution nanotranslator (Model TSE-150, Burleigh Instruments, Inc., Fishers, NY, USA), driven by an inchworm motor with a closed-loop integral linear encoder, permitted positioning of the stage along the x- axis with 50 nm resolution. A 6000ULN controller (Burleigh Instruments) was used to drive the inchworm motor under computer control using custom-written software in G-language (Labview, National Instruments). This software also was used to control a stepper motor (Z-Axis1, Prairie Technologies, Waunakee, WI, USA), driving the focusing mechanism of the microscope (z-axis) with 500 nm resolution. In stage-scanning confocal mode, the specimen was moved in the x direction while the confocal spot remained stationary and the long axis of the muscle fiber was aligned parallel to the x-axis of the microscope stage. The lateral (X-Y) and axial (Z) resolution of the confocal system was determined in vitro using fluorescently labeled latex beads to be 0.3 and 0.75 μm, respectively (Vergara et al., 2001b).

Measurement and analysis of Ca2+-dependent fluorescence transients

The salt form of the Ca2+ indicator Oregon Green 488 BAPTA-5N (OGB-5N) (Molecular Probes, Invitrogen, OR, USA) was added at 500 μM concentrations to the cut ends and allowed to diffuse into the muscle fiber 45-60 minutes prior to optical measurements being started. The typical experimental protocol used to acquire localized fluorescence transients in response to a single AP stimulation of the muscle fiber and their normalization in terms of ΔF/F is described in detail elsewhere (Vergara et al., 2001b; DiFranco et al., 2002). The amplitude of the transients was characterized by its (ΔF/F)peak value and its specific duration by the full duration at half maximum (FDHM).

To determine the spatial dependence of [Ca2+] changes, the illumination spot was initially focused to within 10 µm from the bottom coverslip and on a random location with respect to the fiber's sarcomere structure. Subsequently, individual fluorescent transients elicited by AP stimulation were recorded every 3-5 s from adjacent sites, separated by 200 nm, along the longitudinal axis of the fiber. The combination of stretching and the use of exogenous intracellular Ca2+ buffers (OGB-5N and EGTA) prevented any fiber movement, as evidenced by direct observation under the microscope and the lack of movement artifacts in the optical records.


Localized AP-evoked Ca2+ transients

Figure 1A shows a family of AP-evoked fluorescence transients from a highly stretched muscle fiber (sarcomere length = 4.2 mm) stained intracellularly with the Ca2+ indicator OGB-5N. The optical traces were recorded from 11 consecutive positions, 200 nm apart, along the longitudinal axis of the fiber. The scan spanned a half sarcomere, from a Z-line (trace 1) to the adjacent M-line (trace 11). Figure 1C is a superposition of the 11 APs that elicited the fluorescence transients. It can be observed in Figures 1A and 1B that the transient recorded at the Z-line is significantly faster and larger than the one recorded at the M-line. Also, the kinetic features of the transients recorded at intermediate locations between the M- and Z-line vary continuously from their extreme values at these positions. It should be noted that the position-dependent properties of the optical traces are not accompanied by any detectable change in the electrical records shown in Figures 1C and 1D; they are identical to within 1 mV. While the rising phases of the AP-evoked Ca2+ transients become slower as the recording position moves from the Z- to the M-line, their falling phases remain relatively constant. The characteristic parameters for Z- and M-line Ca2+ transients were reported previously for fibers with 0.5 mM internal [EGTA] (Vergara et al., 2001b; DiFranco et al., 2002). For experiments in fibers equilibrated with 1 mM internal [EGTA], as is the case in Figure 1, we obtained the following Z- and M-values for amplitude (DF/Fpeak), time to peak, and FDHM: 2.06 ± 0.03 and 0.61 ± 0.02; 4.99 ± 0.28 and 7.49 ± 0.36 ms; 5.93 ± 0.53 and 14.23 ± 1.34, respectively. Finally, the large difference in (ΔF/F)peak between the Z- and M-line transients (2.1 vs. 0.61, respectively) demonstrates the existence of large intrasarcomeric Ca2+ gradients, which develop zoom after stimulation but that dissipate after ~ 15 ms. The gradients in 1 mM [EGTA] are more profound and dissipate faster than previously observed for fibers equilibrated with 0.5 mM [EGTA] (DiFranco et al., 2002)

Figure 1. Positional dependence of fluorescence transients detected from a single sarcomere.

A and B: Superimposed OGB-5N ΔF/F transients (1 through 11) and APs recorded at 11 adjacent spot positions along a line parallel to the fiber axis are shown at two different time scales. Traces 1 and 11 correspond to transients recorded at the Z-line and M-line, respectively. C and D: APs associated with the fluorescence transients in A and B shown superimposed at two time scales. Sarcomere spacing: 4.2 μm; [EGTA]: 1 mM. The stimulus time correspond to t = 0 ms.

AP-evoked Ca2+ domains

The concept of a Ca2+ domain, a localized increase in [Ca2+] as a function of space and time, has been used to characterize Ca2+-entry sites in excitable cells and in presynaptic terminals of the neuromuscular junction (Chad and Eckert, 1984; DiGregorio et al., 1999; DiGregorio et al., 2001) and Ca2+-release sites in skeletal muscle fibers (Escobar et al., 1994; Vergara et al., 2001b; DiFranco et al., 2002). Figure 2A is a three-dimensional plot of localized AP-evoked Ca2+ transients, as a function of the spot position, which clearly portrays the topology of the inter- and intra-sarcomeric Ca2+ dynamics involved in the formation and dissipation of Ca2+ domains in a frog skeletal muscle fiber. Data were obtained from a fiber with 0.5 mM internal [EGTA] and externally bathed in Ringer solution. In this plot, which spans three sarcomeres, three defined regions _ regularly spaced along the muscle fiber _ can be observed where the [Ca2+] changes reported by the fluorescence indicator are most prominent. These regions are what we call Ca2+-release microdomains. We have demonstrated previously that they are centered where the T-SR junctions are located at the Z-line (Vergara et al., 2001b; DiFranco et al., 2002). Figure 2B shows a contour map of the same data in Figure 2A, emphasizing the spatial segregation of these local increases in [Ca2+] and how they progress in time by decaying in amplitude and expanding along the longitudinal axis of the fiber.

Figure 2. Effects of 0.5 mM caffeine on Ca2+-dependent, OGB-5N fluorescence domains.

A and B: 3D and contour map created by juxtaposition of the Ca2+-dependent, OGB-5N fluorescence transients recorded at discrete positions in a muscle fiber along a distance of ~14 μm. Panels A and B show the same three domains. C and D: 3D and contour map representations of Ca2+-dependent fluorescence domains in the presence of 0.5 mM caffeine. E and F: 3D and contour map representations of domains obtained after removal of caffeine from the bath. Sarcomere spacing: 4.4 μm; [EGTA]: 0.5 mM. The grayscale palette represents 128 gray levels corresponding to ΔF/F values ranging from 0.3 to 1.4. The stimulus time correspond to t = 5 ms.

Effects of 0.5 mM caffeine on AP-evoked Ca2+ domains

Figures 2C and 2D are three-dimensional and contour plots of three domains recorded from the same fiber, but after equilibration with 0.5 mM caffeine in the bath. It can be observed that the (ΔF/F)peak of each domain in Figure 2C was larger in the presence of caffeine than in the control condition illustrated in Figure 2A. Furthermore, although it is clear that in 0.5 mM caffeine the AP-evoked domains persist for longer times, their spatial distribution apparently remains unchanged. Figures 2E and 2F finally illustrate that the observed effects of caffeine are readily reversed upon removal of the drug from the external solution.

These qualitative observations are further confirmed in the quantitative analysis provided in Figure 3. The solid and dashed traces in Figure 3A are average Z-line transient calculated from the three domains in Figures 2A (control) and 2C (0.5 mM caffeine), respectively. The comparison between these records demonstrates that caffeine induces a significant increase (16%; p<0.05) in the amplitude of the Z-line transients. In addition, the prolongation of the Ca2+ transients by caffeine is evidenced by the significant increase in the FDHM from 10.7 to 16.5 ms. Figure 3B is a superimposition of the six APs that elicited the transients used to calculate the average Z-line transients in Figure 3A. It can be seen that they are practically identical, ruling out the possibility that the caffeine effects on the Ca2+ transients result from electrical changes in the APs. Altogether, the above observations from Z-line-localized data are concurrent with previous results reporting the effects of 0.5 mM caffeine of frog fibers using global illumination/detection techniques and metallochromic indicators (Delay et al., 1986). This finding is interesting since it circumscribes these caffeine effects to be occurring at specific regions of the muscle fibers where the AP-evoked (physiological) Ca2+ release normally occurs. This observation is further confirmed by the results shown in Figures 3C and 3D, which demonstrated that the full width at half-maximum (FWHM) of domains measured isochronously at the time the Z-line transient peaks (~5 ms after AP stimulation) does not change in the presence of 0.5 mM caffeine.

Figure 3. Effects of 0.5 mM caffeine on Z-line transients and FWHM of Ca2+ micro-domains.

A: Each trace represents the average Z-line transient from three consecutive sarcomeres, scanned before (solid trace) and during (dashed line) the application of 0.5 mM caffeine. B: Superposition of the six APs that elicited the Z-lines transients used to calculated the average traces shown in A. C and D: Isochronal profiles calculated at the time the Z-line transient peaks. Data were obtained before (panel C) and during (panel D) the application of caffeine. The FWHM of the domains is 1.42 ± 0.09 and 1.49 ± 0.07 μm, for control and 0.5 mM caffeine, respectively. The values are not significantly different (p> 0.5). Sarcomere spacing: 4.4 μm; [EGTA]: 0.5 mM. The stimulus time correspond to t = 5 ms.

Changes induced by 1 mM caffeine on AP-evoked Ca2+ domains

Figure 4A is a contour map of a long scan comprising 13 sarcomeres of a muscle fiber transiently exposed (for ~ 5 min) to 1 mM caffeine. The scanning process was done as usual by advancing the spot position in 200 nm steps while the fiber was continuously perfused with solutions of different compositions. The scan started with the fiber in Ringer's solution and the first three domains were acquired (positions 0-12 mm). Without interruption of the scanning process, the external solution was then switched to Ringer + 1 mM caffeine. Five domains (positions 12 to 32 mm) were recorded under these conditions, and finally, the fiber was returned to Ringer's solution where the last five domains were recorded. A salient feature of the exposure to 1 mM caffeine illustrated in Figure 4A is that there is a significant prolongation of the Ca2+ domains. However, this effect is not constant while the fiber is in the presence of caffeine, but decays over time. By comparing the amplitude of the isochronal profiles before (ΔF/F=1.94 ± 0.03, Figure 4B) and during the application of caffeine (ΔF/F= 1.87 ± 0.04, Figure 4C), we conclude that, in contrast to what was observed at 0.5 mM, at 1 mM caffeine does not potentiate Ca2+ release (p>0.2). However, in agreement with what was observed with lower doses of the drug, the Ca2+ domains were not broadened by 1 mM caffeine since the FWHMs measured before (1.43 ± 0.05 µm) and during exposure to caffeine (1.48 ± 0.07 mm) were not significantly different (p>0.5). Curiously, the isochronal profiles obtained after the removal of caffeine from the bath solution (Figure 4D) have the same amplitude but are marginally narrower than those obtained before and during caffeine exposure (p=0.05).


Figure 4. Effects of 1 mM caffeine on Ca2+-release microdomains.

A: Contour map of a continuous scan spanning 13 sarcomeres. From the bottom up, the first three domains were obtained before the application of caffeine, the next five in the presence of caffeine, and the last five, after washing out the drug from the bath. The stimulus time corresponds to t = 0 ms. B to D: Plots of isochronal profiles at the point when the Z-line transients peaked. Panel B data was obtained from domains 1 to 3 in A (Ringer). Panel C data was obtained from domains 6 to 8 in A (Ringer+1mM caffeine). Panel D data was obtained from domains 11 to 13 in A (Ringer). Sarcomere spacing: 4.2 μm; [EGTA]: 1.0 mM.

Unexpected effects of 1 mM caffeine

The ability to record from minute volumes inside the sarcomere permits us to report on drug effects not detectable by global detection methods. While studying the effects of 1 mM caffeine on localized Ca2+ release, we found several unexpected phenomena, and here, we report two of them. An interesting set of observations are illustrated in Figure 5. Figures 5A and 5C show superimposed Z-line transients from two sets of sarcomeres acquired before and during exposure to caffeine, respectively. Besides confirming our observations above on the effect of 1 mM caffeine on the amplitude and kinetics of the transients (Figure 4), these figures demonstrate that there is not too much variability among localized Z-line Ca2+ transients both under control conditions or in the presence of caffeine. These observations are further confirmed by the relatively small values of normalized average variance plotted in Figure 5E, even in the case of caffeine exposure (solid trace). In contrast, when the variability among M-line transients was investigated (Figures 5B, 5D, and 5F), the results are in sharp contrast with those for Z-line transients. Although in the absence of caffeine, M-line transients from different domains are relatively similar to each other (see Figure 5A and dotted trace in Figure 5F), exposure to 1 mM caffeine dramatically increased the variability among them. This is clearly visible in the widely different kinetics and amplitudes of the five different records superimposed in Figure 5D, and quantitatively demonstrated by the significant increase in the normalized variance record (solid trace) of Figure 5F.

Figure 5. Caffeine-induced variance in M-line localized Ca2+ transients.

A to D: Superimposed Z-line transients (panels A and C) and M-line transients (panels B and D) recorded before (panels A and B) and during (panels B and D) the application of 1 mM caffeine. Note the different DF/F scales for Z- and M-line transients. E and F: Normalized average variance calculated from DF/F records obtained before (dotted traces) and during (solid traces) the application of caffeine. Data for E and F was calculated from Z- and M-line transients, respectively. Sarcomere spacing: 4.2 mm; [EGTA]: 1 mM. The stimulus time correspond to t = 5 ms.

Another interesting result is the sporadic observation of extra-triadic Ca2+ release illustrated in Figure 6. It can be observed in the three-dimensional and contour plots (Figures 6A and 6B, respectively) that shortly after the application of caffeine (arrow in Figure 6B), an extra source of Ca2+ release appears at one side of the Z-line transient of three first domains recorded after caffeine application. This Ca2+ source is not only off- centered with respect to the Z-line, but it also was activated with a longer delay after the application of the stimulus (t = 0). On the other hand, as also seen in the Z-line transient, the release of the extra-junctional source is long lasting. These observations are substantiated in Figure 6C, which displays two isochronal profiles of the domains in Figure 6A: one profile was calculated at the time the Z-line transient peaked (~5 ms after AP stimulation, open circles); the other was calculated 25 ms after AP stimulation (filled circles) when the [Ca2+] of the three domains had subsided to basal levels in Ringer solution, but remained elevated in 1 mM caffeine. It should be noted that the spurious Ca2+ source, seen as a secondary peak in the late isochronal profile, is located ~1 µm away from the Z-line (towards the M-line) and has an amplitude comparable to the fluorescence detected at that point in time at the Z-line.

Figure 6. Extra-junctional Ca2+ release activated by 1 mM caffeine.

A: Contour map of a continuous scan spanning 6 sarcomeres. B: 3D plot of the upper four sarcomeres shown in panel A. The point of caffeine application is indicated by the white arrow. The stimulus time in panels A and B correspond to t = 0 ms. C: Isochronal plots obtained at the time when the Z-line transient peaks (open circles) and 24 ms after stimulation (filled circles). Sarcomere spacing: 4.1 mm; [EGTA]: 0.5 mM.


The results presented here emphasize the importance of using localized detection techniques to investigate the effects of caffeine on EC coupling in skeletal muscle. Namely, some of the observations on the amplitude and kinetics of localized Ca2+ transients mimic the effects of the drug observed with global detection methods (Delay et al., 1986; Herrmann-Frank et al., 1999), but other outcomes associated with the spatiotemporal properties of Ca2+-release domains are surprising and have unfathomable implications. Thus, the finding that localized Z-line Ca2+ transients are reversibly affected by caffeine in a concentration-dependent fashion broadly agrees with the effects reported with metallochromic indicators by Delay et al. (1986). At low concentrations (0.5 mM), we observed potentiation (increase in peak ΔF/F) and prolongation (increased FDHM) of the Z-line Ca2+ transients (Figs. 2 and 3), the same as reported by these authors for global transients. Also, at higher doses (1 mM in our case) the potentiation is not so obvious, but the prolongation remains (Figs. 4 and 5). The interesting consequences of the current observations of caffeine effects on localized Z-line transients is that they arise from highly circumscribed regions of the sarcomere where the sources of Ca2+ release are located (triads), thus providing a closer link between caffeine effects in vivo and in vitro observations of an increased open probability of the RyR channel (Rousseau et al., 1988).

It is curious that the caffeine effects on Z-line transients was not accompanied by either an increased fluctuation in their amplitudes, nor by an expansion in the FWHM of the Ca2+ release domains (Figs. 2 to 4) as would be expected from a caffeine-induced sensitization of the RyR channels to Ca2+ (Rousseau et al., 1988). This is important since the enhancement of CICR by caffeine traditionally has been proposed as a mechanism of Ca2+ potentiation by the drug (Herrmann-Frank et al., 1999). What is even more surprising is that, at moderate concentrations (1 mM), caffeine was responsible for striking fluctuations in the amplitude of localized transients detected at the M-lines of the muscle fibers (Fig. 5), arguably the farthest away from the expected location for Ca2+ release channels (Z-line). One way to reconcile these observations with the current understanding of EC coupling in amphibian skeletal muscle is that these doses of caffeine may affect the sequestration of Ca2+ by the Ca2+ ATPase, reportedly located preferentially in this region of the sarcomere (Peachey, 1965; Connolly et al., 1971).

Another tantalizing result was that in the presence of 1 mM caffeine, extra- junctional sources of Ca2+ release were found occasionally (Fig. 6), again in regions of the sarcomere as far as 1 µm away from the Z-line. The presence of these sources of Ca2+ release may be related to the large fluctuations seen at the M-line, but they have a more discrete appearance and are more infrequently observed than the latter. Interestingly, these extra-junctional Ca2+ sources resemble what would be expected for a Ca2+ spark-type of release (as seen with a low affinity Ca2+ indicator), which frequency of appearance reportedly has been enhanced by caffeine exposure in amphibian muscle fibers (Gonzalez et al., 2000).


This work was supported by National Institutes of Health grants AR47664 and GM074706 and a Grant in Aid from the Muscular Dystrophy Association.



CHAD JE, ECKERT R (1984) Calcium domains associated with individual channels can account for anomalous voltage relations of Ca-dependent responses. Biophys J 45: 993-999         [ Links ] GOUGH W, WINEGRAD S (1971) Characteristics of the isometric twitch of skeletal muscle immediately after a tetanus. A study of the influence of the distribution of calcium within the sarcoplasmic reticulum on the twitch. J Gen Physiol 57: 697-709         [ Links ]

DELAY M, RIBALET B, VERGARA J (1986) Caffeine potentiation of calcium release in frog skeletal muscle fibres. J Physiol 375: 535-559         [ Links ]

DIFRANCO M, NOVO D, VERGARA JL (2002) Characterization of the calcium release domains during excitation-contraction coupling in skeletal muscle fibres. Pflugers Arch 443: 508-519         [ Links ]

DIFRANCO M, QUINONEZ M, DIGREGORIO DA, KIM AM, PACHECO R, VERGARA JL (1999) Inverted double-gap isolation chamber for high-resolution calcium fluorimetry in skeletal muscle fibers. Pflugers Arch 438: 412-418         [ Links ]

DIGREGORIO DA, NEGRETE O, JEROMIN A, PENG HB, VERGARA JL (2001) Contact-dependent aggregation of functional Ca2+ channels, synaptic vesicles and postsynaptic receptors in active zones of a neuromuscular junction. Eur J Neurosci 14: 533-546         [ Links ]

DIGREGORIO DA, PESKOFF A, VERGARA JL (1999) Measurement of action potential-induced presynaptic calcium domains at a cultured neuromuscular junction. J Neurosci 19: 7846-7859         [ Links ]

ENDO M, TANAKA M, OGAWA Y (1970) Calcium induced release of calcium from the sarcoplasmic reticulum of skinned skeletal muscle fibres. Nature 228: 34-36         [ Links ]

ESCOBAR AL, MONCK JR, FERNANDEZ JM, VERGARA JL (1994) Localization of the site of Ca2+ release at the level of a single sarcomere in skeletal muscle fibres. Nature 367: 739-741         [ Links ]

FABIATO A, FABIATO F (1975) Contractions induced by a calcium-triggered release of calcium from the sarcoplasmic reticulum of single skinned cardiac cells. J Physiol (Lond) 249: 469-495         [ Links ]

GONZÁLEZ, A, KIRSCH WG, SHIROKOVA N, PIZARRO G, BRUM G, PESSAH IN, STERN MD, CHENG H, RIOS E (2000) Involvement of multiple intracellular release channels in calcium sparks of skeletal muscle. Proc Natl Acad Sci USA 97: 4380-4385         [ Links ]

GUTMANN E, SANDOW A (1965) Caffeine-induced contracture and potentiation of contraction in normal and denervated rat muscle. Life Sci 4: 1149-1156         [ Links ]

HERRMANN-FRANK A, LUTTGAU HC, STEPHENSON DG (1999) Caffeine and excitation-contraction coupling in skeletal muscle: A stimulating story. J Muscle Res Cell Motil 20: 223-237         [ Links ]

KIM AM, VERGARA JL (1998) Supercharging accelerates T-tubule membrane potential changes in voltage clamped frog skeletal muscle fibers. Biophys J 75: 2098-2116         [ Links ]

LÓPEZ JR, ÁLAMO L, CAPUTO C, DIPOLO R, VERGARA JL (1983) Determination of ionic calcium in frog skeletal muscle fibers. Biophys J 43: 1-4         [ Links ]

NOVO D, DIFRANCO M, VERGARA JL (2003) Comparison between the predictions of diffusion-reaction models and localized Ca2+ transients in amphibian skeletal muscle fibers. Biophys J 85: 1080-1097         [ Links ]

PEACHEY LD (1965) The sarcoplasmic reticulum and transverse tubules of the frog's sartorius. J Cell Biol 25: Suppl: 209-231         [ Links ]

RÍOS E, PIZARRO G (1991) Voltage sensor of excitation-contraction coupling in skeletal muscle. Physiol Rev 71: 849-908        [ Links ] LADINE J, LIU QY, MEISSNER G (1988) Activation of the Ca2+ release channel of skeletal muscle sarcoplasmic reticulum by caffeine and related compounds. Arch Biochem Biophys 267: 75-86        [ Links ]

SANDOW A (1970) Skeletal muscle. Annu Rev Physiol 32: 87-138        [ Links ]

SHIROKOVA N, RIOS E (1996) Activation of Ca2+ release by caffeine and voltage in frog skeletal muscle. J Physiol 493: 317-339        [ Links ]

SITSAPESAN R, WILLIAMS AJ (1990) Mechanisms of caffeine activation of single calcium-release channels of sheep cardiac sarcoplasmic reticulum. J Physiol 423: 425-439        [ Links ]

ERGARA JL, DIFRANCO M, NOVO D (2001a) Confocal study of the effects of caffeine on calcium release elicited by action potential stimulation. Biophys J 80: 331a

VERGARA JL, DIFRANCO M, NOVO D (2001b) Dimensions of calcium release domains in frog skeletal muscle fibers. Proceedings of SPIE 4259: 133-143        [ Links ]

WENDT IR, STEPHENSON DG (1983) Effects of caffeine on Ca-activated force production in skinned cardiac and skeletal muscle fibres of the rat. Pflugers Arch 398: 210-216        [ Links ]


Corresponding author: Julio L. Vergara, Department of Physiology, David Geffen School of Medicine, UCLA, 10833 Le Conte Avenue 53-263 CHS, Los Angeles, CA 90095-1751, USA, Tel.: (1-310) 825-9307, Fax: (1-310) 206-3788, Email:

Received: November 30, 2005. Accepted: January 11, 2006

Creative Commons License All the contents of this journal, except where otherwise noted, is licensed under a Creative Commons Attribution License