Effects on lactate metabolism.
Typically, an elevated metabolic rate is associated with a faster glycolytic rate and concomitant lactate production. However, if the metabolic rate is elevated without a large increment in glycolysis, then net lactate utilization could be increased due to a faster rate of pyruvate and NADH oxidation. These requirements are likely met during steady-state submaximal exercise. Net lactate utilization may also be increased during more intense exercise after the contracting muscles have gone through an initial transient period (first 10–15 min) of rapid lactate release (19,31,33,75). Numerous studies of blood [La] decline during exercising recovery (e.g., 22,44,65) support the notion that an increase in muscle metabolic rate stimulates net muscle lactate uptake as do studies of isotopically labeled lactate during exercise in intact animals and across contracting muscle groups (15–17).
Gladden et al. (32,35) have directly addressed the role of metabolic rate in net lactate uptake by the canine gastrocnemius in situ. Lactate/lactic acid was infused to elevate arterial plasma [La] while maintaining normal acid-base status. As illustrated in Figure 1, net lactate uptake was greater (with an elevated arterial [La] of ≈9 mM) during 4-Hz twitch contractions (high metabolic rate) in comparison with 1-Hz twitch contractions (moderate metabolic rate) or rest (low metabolic rate). Because the net lactate uptake measurements were done under steady-state conditions, they imply that the increased uptake represents an increased utilization of lactate. An interesting point of this study (32) is that, after an initial transient period, there was substantial net lactate uptake by a muscle contracting at greater than 90% of V̇O2peak for twitches. Similar experiments have not been done during tetanic contractions. This could be of considerable interest because V̇O2peak for the dog gastrocnemius during tetanic contractions is greater than 240 mL O2·kg−1·min−1 in comparison to only 140 mL O2·kg−1·min−1 for twitch contractions (51).
Effects on lactate transport.
Before the muscle can metabolize lactate from an external source, the lactate must cross the sarcolemmal membrane. Clearly, glucose transport in skeletal muscle is turned on by exercise (30,38,41,64,81). Does exercise similarly activate lactate transport?
Only a few studies (9,62,85) have evaluated the impact of acute exercise or contractions on sarcolemmal lactate transport. Overall, this evidence suggests that any enhancement of lactate transport by exercise is minimal (≈0–28%) when compared with the increases that are typically reported for muscle glucose uptake (≈62–400%) in response to exercise (30,38,64,81). Acute lactate transport responses also appear to be minor in comparison with the increases in lactate production, utilization, and flux that are engendered by muscle contractions. This implies that an increase in lactate transport is not an important, acute regulatory response to exercise (33,48). Instead, it appears that increased transmembrane lactate flux during exercise is more likely due to increased transmembrane [La] and [H+] gradients (8). However, some reservation is warranted given that lactate transport during contractions has not been satisfactorily assessed due to experimental limitations.
Both Juel (48) and Gladden (31) have discussed circumstantial evidence which suggests that lactate exchange, including uptake, might be enhanced by higher muscle blood flow. Most of this evidence is correlational in nature, such as Jorfeldt’s report (45) that the rate of lactate uptake by human forearm muscle during lactate infusion related more closely to the product of arterial [La] and muscle blood flow than with arterial [La] alone. There have been only a couple of studies that have attempted to directly evaluate the potential role of blood flow on lactate exchange (34,85).
In one of these studies, Gladden et al. (34) investigated the effect of blood flow on net lactate uptake in the dog gastrocnemius in situ. In all trials, metabolic rate (1-Hz twitch contractions) and blood [La] (≈12 mM) were elevated and held constant while blood flow was varied. An increase in blood flow to ≈165% of the normal spontaneous level had no significant effect on net lactate uptake, whereas net lactate uptake was increased by 29% when the blood flow was further increased to ≈200% of normal. Altogether, these experiments suggest a minor role for blood flow in determining net lactate uptake in this preparation. It remains uncertain, however, whether or not these results extend to the much higher metabolic rates that are possible in tetanic contractions with a more favorable duty cycle (12,13,23,51) or to asynchronous contractions during exercise in vivo. Furthermore, the potential effect of flow heterogeneity on lactate exchange has not been evaluated. The critical factor would be net lactate uptake/perfusion (L/Q) matching (31).
Possible effects of flow on the transport process for lactate influx into muscle tissue are difficult to evaluate. As an approximation, Watt et al. (85) assessed the effects of perfusate flow on rapid tracer lactate influx into isolated, resting rat hindlimb. Rapid tracer lactate influx as measured by the paired-tracer dilution method was dependent on perfusate flow at rates less than 0.5 mL·g−1·min−1. However, limitations of the paired-tracer method prevent definitive conclusions.
In summary, blood flow and its optimal distribution are theoretically of great importance in net lactate exchange. In the case of net lactate uptake, if all other factors remain constant, an increased blood flow should increase lactate and proton delivery to the muscle, thereby maintaining more favorable extracellular to intracellular lactate and proton gradients, thus promoting net lactate uptake. Lactic acid translocation across the sarcolemma is likely to be rapid due to trans-stimulation or equilibrium exchange conditions between the interstitial and intramuscular spaces. However, net exchange will be enhanced only by maintaining a [La]gradient and/or a proton gradient (48).
BLOOD LACTATE CONCENTRATION
Radioactive tracer studies in dogs (43), rats (29), and humans (20,83) have shown that lactate uptake increases as the blood [La] increases. Pagliassotti and Donovan (67) obtained similar results in perfused muscles of the rabbit. Their results, with a special emphasis on fiber type, are discussed in more detail in another paper in this symposium by Donovan (24).
In addition, Gladden et al. (32,34,35,37) have shown that net lactate uptake by canine gastrocnemius muscle in situ increases in proportion to arterial plasma [La]. Figure 2 (35) illustrates that progressively increasing plasma [La] elevated net lactate uptake, with a tendency for net lactate uptake to approach a plateau at the higher plasma lactate concentrations (≈20–30 mM). The highest asymptote for net lactate uptake was calculated for twitch contractions at a frequency of 4 Hz. This contraction frequency produces V̇O2peak for twitches in this muscle preparation (13). Interestingly, the asymptote for peak net lactate uptake (1.1 mmol·kg−1·min−1) in these twitch contractions is only half the peak net lactate output (2.2 mmol·kg−1·min−1) measured during contractions that elicit tetanic V̇O2peak (13,51). There are several possible reasons for this large difference. First, it is likely that net lactate uptake during the twitches was limited by lactate metabolism within the muscle. There would be no analogous limitation for net lactate output. Also, a more favorable duty cycle for blood flow (12,13,23,51) could have promoted lactate output in the tetanic contractions in comparison to the net lactate uptake during the twitch contractions. Perhaps net lactate uptake during the twitches was limited by membrane transport of lactate. If so, there may have been a greater transmembrane [La] gradient in the experiments with net lactate output during tetanic contractions. There may also have been a greater [H+] gradient in the direction of lactate translocation during the tetanic contractions. It is unlikely that asymmetry of the lactate transport processes causes a faster efflux in comparison to influx (33,46–48). All of these possible differences between tetanic lactate output and twitch lactate uptake point to a need for experiments in which net lactate uptake is assessed with elevated blood [La] during steady state tetanic contractions.
Considering the effect of [La] on membrane transport, it has been well established that transmembrane lactate flux is dependent on the transmembrane [La] gradient. This is apparent as a linear, diffusive component in addition to a saturable component which is the result of monocarboxylate transport protein (MCT) activity (46,48,74,77,78,86). Sarcolemmal lactate transport is described in detail by Bonen (7) in a separate paper of this symposium.
HYDROGEN ION CONCENTRATION
Possible effects of [H+] on lactate utilization are most likely related to intramuscular (intracellular) [H+]. It is a reasonable assumption that if increased intracellular [H+] inhibits lactate production in the presence of an adequate exogenous [La], then lactate utilization will be enhanced. In support of this notion, Graham et al. (39) reported that acidosis, induced by hypercapnia, resulted in net lactate uptake by dog gastrocnemii in situ after 20 min of contractions at 3 Hz. Under normal acid-base conditions, the gastrocnemii were still releasing lactate after 20 min of contraction at 3 Hz. Bonen et al. (11) have also reported that glycogen synthesis from lactate in mouse fast-twitch (EDL) and slow-twitch (soleus) muscles in vitro was stimulated by decreases in external pH over the physiological range. Whether this enhancement of glyconeogenesis was due to a reduced intracellular pH that inhibited PFK activity thus promoting reversal of glycolysis or was due to a greater transmembrane [H+] gradient that increased membrane transport of lactate is unclear. Further study of the interaction between intracellular [H+] and lactate utilization is needed.
Roth and Brooks (79) have shown that the absolute [H+] is of little consequence to sarcolemmal lactate transport. However, increases in the [H+] gradient across the sarcolemma stimulate flux in the direction of high [H+] to low [H+] although the reported magnitude of the effect has varied (9,46,48,50,61,62,79,86). If the direction of the [H+] gradient is counter to the [La] gradient, lactate flux is markedly inhibited (79). Two mechanisms explain the stimulatory lactate transport effect in the direction of a proton gradient. First, diffusion of lactate occurs primarily in the form of undissociated lactic acid (HLa) and is therefore mainly dependent on the concentration of HLa (46,50,79). By the law of mass action, HLa concentration ([HLa]) on the side of higher [H+] will be increased in comparison with [HLa] on the side of lower [H+].
Second, a proton gradient probably also stimulates lactate transport via its effect on the monocarboxylate carrier. As Figure 3 illustrates, H+ probably binds to the carrier first and then the lactate anion follows (8,48). Unloading occurs in the reverse order. In this scheme, high protons on one side of the membrane would speed H+ binding to the carrier and therefore speed lactate binding. On the low [H+] side, H+ unloading after lactate unloading would be enhanced. The effect of proton gradients most likely depends on the combination of the proton gradient and the [La] gradient and therefore the relative contributions of diffusion versus carrier to lactate flux.
MUSCLE FIBER TYPE
Net lactate uptake and disposal.
Donovan (24) addresses the role of muscle fiber type in the net fate of lactate taken up by muscles in another paper in this symposium. Therefore, only a brief summary will be provided here. Oxidative muscle fibers begin to take up lactate at a lower perfusate or blood [La] and take up lactate at faster maximal rates in comparison to glycolytic muscle fibers (33,66,67). Oxidative muscle fibers predominantly oxidize lactate whereas glycolytic fibers primarily convert lactate to glycogen (2,11,33,63,66–68,80). Lactate oxidation is highly correlated with the total LDH H-isozyme activity (2). Both the rate of muscle lactate uptake and the route of disposal for lactate clearly depend on the fiber type composition of the muscle (33).
Only a few studies (9,49,72) have investigated lactate transport in different muscle fiber types, but the findings are consistent. Lactate transport is significantly faster (≈37–109%) in oxidative muscle fibers than in glycolytic fibers. Bonen (7) will provide details on the lactate transport protein in another paper in this symposium. However, it should be noted here that Bonen’s group (58) has shown that muscle content of the Type I monocarboxylate transporter (MCT1) is highly correlated with the percentage of oxidative fibers in the muscle.
At first glance, the finding that lactate transport is faster in oxidative muscle fibers than in glycolytic fibers contradicts the notion that glycolytic muscle fibers are prone to high lactate production rates during contractions/exercise and that they should be equipped for rapid transport of lactate out to the extracellular environment. However, oxidative fibers do produce lactate and they are usually active for longer periods of time than are glycolytic fibers. A greater ability to transport lactate (and H+ ions at the same time) out of oxidative fibers might partially explain the greater resistance to fatigue in oxidative fibers (49). Further, peak lactate production by oxidative muscle fibers may be greater than is usually appreciated. For example, peak lactate output by contracting, oxidative canine gastrocnemius muscle in situ is similar to peak lactate output by contracting, glycolytic feline gastrocnemius muscle in situ (82). Juel (48) notes that if the metabolic ability of muscle fibers to produce lactate is based only on muscle lactate concentration without considering release, differences in maximal lactate production between glycolytic and oxidative muscle fibers may be overestimated. Finally, the faster lactate transport rates in oxidative fibers may reflect the role of lactate as an energy substrate for those fibers, whereas the slower lactate transport rates in glycolytic fibers may contribute to greater retention of lactate during recovery from intense exercise. The retained lactate in glycolytic fibers postexercise is then more likely to be resynthesized into glycogen (67–69).
Endurance training appears to cause an increase in lactate utilization by muscles. Several studies in rats (25–27) as well as humans (55,70) have reported that metabolic clearance rate of lactate is significantly increased after endurance training. Presumably, most of this clearance enhancement is due to adaptations in skeletal muscle. As an example, Donovan and Pagliassotti (27) infused lactate into resting rats at different rates. With increasing rates of lactate infusion, blood [La] rose in a curvilinear fashion, reaching >11 mM in sedentary rats as compared with ≈5.5 mM in endurance trained rats. As shown in Figure 4, this training response was due to a more rapid rise in net lactate removal with increases in blood [La]. The apparent Km for net lactate removal was dramatically lowered after training to a value that was one-third that found in the sedentary animals (4 vs 12 mM).
The mechanisms underlying improved lactate removal by muscle after endurance training are not well-defined. Training-induced metabolic adaptations in skeletal muscle that might be expected to speed lactate utilization include: 1) increased oxidative capacity due to a greater mitochondrial content causing increased oxidative enzyme concentrations, 2) increased pyruvate dehydrogenase activity that could improve pyruvate usage after its production from lactate, 3) increased malate-aspartate shuttle activity that might facilitate oxidation of NADH resulting from lactate to pyruvate conversion, and 4) a shift in the lactate dehydrogenase isozyme pattern from the muscle isoform toward the heart isoform (26,27).
There is almost unanimous agreement that muscle activity pattern (i.e., muscle unweighting, denervation vs chronic stimulation, exercise training) influences lactate transport across the sarcolemma, sometimes quite dramatically (1,28,56,57,59,60,71,73). The largest changes in lactate transport (2–2.8× increase) have been observed after 7 d of chronic electrical stimulation of tibialis anterior muscles of the rat (57,59). However, the pattern of reported effects is not consistent. Among those studies that have made estimates of the kinetics of lactate transport, exercise training has been postulated to lower the Km and increase the Vmax (73), or to reduce the Km with no effect on the Vmax (60). Most of these kinetics values represent crude estimates based on only a few [La] gradients and sometimes on data patterns that do not appear to follow Michaelis-Menten kinetics. Some of the apparent discrepancies may arise from differences in experimental procedures, such as the gender of animals studied, training programs, and methods of lactate transport measurement.
There has been only one study of the effect of training on sarcolemmal lactate transport in humans. Mean lactate efflux rate was significantly higher from the sarcolemmal giant vesicles of athletes as compared with vesicles from untrained and trained control groups. However, no subject with V̇O2max less than 68 mL·kg−1·min−1 had a greater than average lactate transport capacity. Specific comparisons among the athletes revealed that both a high volume (frequency and duration) and regular high intensity of training were required to improve lactate transport capability. The highest lactate efflux rates were found in two 4-km bicyclists, one of whom was a bronze medalist at the 1992 Olympic Games.
The reported improvements in lactate transport ability due to increased muscle activity could result from an increase in the percentage of slow twitch, oxidative muscle fibers (48,71,73). However, it seems more likely that increased substrate affinity of the carrier (↓Km), increased intrinsic activity of the carrier (↑Vmax), increased density of carriers in the sarcolemma (↑Vmax), or changes in the isoform distribution of the carrier (↓Km and/or ↑Vmax) could account for the changes (48,57,59,60,73).
The underlying stimulus for the transport alterations is clearly related to the repeated contractions. However, it is unlikely that the stimulus is increased glycolytic activity and concomitant changes in tissue [La] (48,57). Regardless of causation, improved membrane transport of lactate could promote lactate efflux from muscles that are producing lactate, and aid influx into less active muscles for oxidation and/or glyconeogenesis (33,48,60).
In summary, the evidence suggests that net consumption of lactate by skeletal muscle is likely to be enhanced by:
1) A high steady-state metabolic rate that does not engender an elevated endogenous lactate production that interferes with exogenous lactate utilization. Effects of increased metabolic rate on sarcolemmal lactate transport appear to be minimal.
2) Blood flow that is adequate to maintain optimal outside to inside [La] and [H+] gradients. The blood flow should ideally be matched to the rate of net lactate uptake; that is, the L/Q ratio should be optimized. Whether or not higher than normal spontaneous blood flow will facilitate lactate exchange is not clear.
3) An elevated [La] gradient at least to the point of saturation of either the metabolic pathways for lactate utilization or the sarcolemmal monocarboxylate transport system. Whether metabolism or transport is the key limiting factor is not known.
4) An increased intracellular [H+] to the extent that it inhibits endogenous lactate production without inhibiting muscle function or limiting inward sarcolemmal lactate transport. Probably more importantly, a significant outside to inside [H+] gradient will stimulate sarcolemmal lactate influx.
5) A predominance of oxidative muscle fibers. Oxidative muscle fibers are metabolically tuned for lactate oxidation and have a greater capacity for sarcolemmal lactate transport than do glycolytic muscle fibers.
6) Endurance training. Metabolically, endurance training improves muscle capacity for lactate utilization. In terms of membrane transport, increased muscle activity has a positive impact but whether or not this impact is realized in humans except under conditions of both high volume and high-intensity training is not clear.
THE NEXT CHALLENGE
Presently, we know a great deal about the processes involved in lactate exchange, including the various pathways of metabolism and the sarcolemmal transport process. However, we do not know exactly how lactate exchange is regulated under various conditions. Specifically, what role if any does the MCT family play in the regulation or limitation of net lactate exchange?
Typically, if a [La] gradient across a membrane is observed, it is inferred that there is a transport limitation. Although this may be the case, it is not necessarily true that unidirectional lactate flux is limiting just because a [La] gradient exists. For example, it has been proposed that lactate is distributed as an inverse function of the transmembrane [H+] ratio (76). If true, this could be due to the fact that transport via diffusion depends on the concentration of the undissociated lactic acid ([HLa]), which increases as the [H+] increases and/or the fact that MCT transport of lactate is enhanced in the direction of the [H+] gradient due to a faster binding of H+ to MCT (see section on Hydrogen Ion Concentration above). At least one implication of this hypothesis is that even in a steady state in which the net lactate flux is zero and transmembrane lactate translocation is not limiting, the intracellular and extracellular concentrations of lactate are unlikely to be equal. Is it possible that cellular pH regulation drives steady state transmembrane lactate distribution? However, Juel (48) presents strong arguments (which will not be repeated here) in favor of the notion that transmembrane lactate distribution is a function not only of the [H+] gradient but also of blood flow and the balance between lactate transport and metabolism (see Juel’s review, ref. 48, pp. 333–339 and associated citations).
Based on the evidence to date, it seems most likely that lactate transport is limiting during and after high-intensity exercise. Under such conditions, the rate of lactate production apparently outstrips maximal net efflux of lactate (48). Whether or not membrane transport of lactate limits net lactate uptake is less certain. It is a universal finding that intramuscular [La] is lower than external [La] during periods of elevated perfusate or blood [La] (3,21,32,37,52,63,76). The ratio between intracellular [La] and extracellular [La] covers a broad interval with several reported values in the range of 0.4–0.6 (3,32,37,48,37). Does this mean that lactate transport is limiting? Again, at least a portion of this [La] gradient may be attributable to the prevailing [H+] gradient (31,76) or alternatively to the balance between net lactate influx and intramuscular lactate removal due to metabolism (48). For working hearts using lactate as a major energy source, Halestrap et al. (40) have estimated that lactate influx may exceed the maximal capacity of MCT. However, if diffusive flux is included, transport may not be limiting. Recent reports from Bonen’s laboratory (1,7,8,10,59) relative to the effects of chronic muscle stimulation and exercise training on muscle MCT1 content lend credence to the notion of a regulatory role for lactate transport per se.
I believe that our speculations about limiting factors for transmembrane lactate flux are being made on the basis of weak or nonexistent data. I am unaware of any studies that have validly evaluated intracellular, interstitial, and plasma lactate concentrations under a variety of physiological conditions. A careful determination of intracellular to extracellular [La] ratios requires as a minimum accurate measurements of total muscle water, interstitial water, and plasma water along with rapid separation of plasma from red blood cells. This would allow correction of measured muscle [La] for interstitial lactate assuming that interstitial [La] is equal to plasma [La]. However, a) interstitial [La] may not always be equilibrated with plasma [La] (48,54), and b) interstitial [H+ ] may also be different from plasma [H+] (31,84).
How can we assess the possible role of lactate transport as a limiter of lactate exchange and metabolism? Sarcolemmal vesicles offer many advantages: a) they allow studies of sarcolemmal transfer alone, b) they eliminate confounding problems of metabolism, capillary diffusional resistance and flow, interstitial concentration variabilities, and uncontrolled intracellular solute compositions, and c) they have provided the material for isolation, purification, and sequencing of the lactate transporter protein (33,48,77,78). However, sarcolemmal membrane preparations represent only a small sample of the total membrane surface. Also, they separate the lactate transport processes from the metabolic processes that they serve. This removes regulatory interaction between transport and metabolism (33,62). Some questions regarding lactate transport require models other than sarcolemmal vesicles. For example, there is presently no way to estimate the physiological lactate transport capacity from vesicle studies. Furthermore, experiments with sarcolemmal vesicles do not provide any method for direct evaluation of the possible effects of physiological factors such as blood flow, muscle contractions, and changes in hormonal concentrations on the lactate transport process.
Promising possibilities are offered by multiple tracer methods and models such as those developed by Bassing-thwaighte’s group (4,5,53). These techniques employ realistic and necessarily complex models of capillary-tissue exchange. One such model is the MMID4 model (6); that is, M ultiple path, M ultiple tracer, I ndicator D ilution, 4 region model (see Bassingthwaighte et al. (6) for illustration and details). Data collection is similar to that of the less precise paired tracer technique (36,42,87) except that an intravascular tracer is used as well. Ideally, comprehensive data collection (including microsphere measurement of blood/perfusate flow heterogeneity) will allow quantitative, accurate estimation of capillary permeability, sarcolemmal permeability, and rapid metabolism of lactate. Typical data are presented in Figure 5. Although modeling and parameter estimation have not yet been done, there does appear to be measurable lactate influx that is inhibited by the lactate transport blocker PCMBS. Preliminary results suggest that metabolism of lactate to CO2 and H2O accounts for less than 5% of the counts throughout the lactate curve. It also appears that only a small amount of the counts are attributable to pyruvate (<5%). Perhaps this model as well as other experimental approaches will provide information on the possible regulatory role of lactate transport in the near future.
This work was supported in part by National Institutes of Health grant 1R01AR40342. I am grateful to Dr. Mike Hogan for his evaluation of the manuscript.
1. Baker, S. K., K. J. A. McCullagh, and A. Bonen. Training intensity-dependent and tissue-specific increases in lactate uptake and MCT-1 in heart and muscle. J. Appl. Physiol. 84:987–994, 1998.
2. Baldwin, K. M., A. M. Hooker, and R. E. Herrick. Lactate oxidative capacity in different types of muscle. Biochem. Biophys. Res. Commun. 83:151–157, 1978.
3. Bangsbo, J., T. Aagaard, M. Olsen, B. Kiens, L. P. Turcotte, and E. A. Richter. Lactate, and h+
uptake in inactive muscles during intense exercise in man. J. Physiol. (London) 481:219–229, 1995.
4. Bassingthwaighte, J. B., I. S. J. Chan, and C. Y. Wang. Computationally efficient algorithms for convection-permeation diffusion models for blood-tissue exchange. Ann. Biomed. Eng. 20:687–725, 1992.
5. Bassingthwaighte, J. B., C. A. Goresky, and J. H. Linehan. Modeling in the analysis of the processes of uptake and metabolism in the whole organ. In: Whole Organ Approaches to Cellular Metabolism, J. Bassingthwaighte, C. A. Goresky, and J. H. Linehan (Eds.). New York: Springer, 1998, pp. 3–27.
6. Bassingthwaighte, J. B., C. Y. Wang, and I. S. Chan. Blood-tissue exchange via transport and transformation by capillary endothelial cells. Circ. Res. 65:997–1020, 1989.
7. Bonen, A. Lactate transporters (MCT proteins) in heart and skeletal muscles. Med. Sci. Sports Exerc. 32:778–789, 2000.
8. Bonen, A., S. K. Baker, and H. Hatta. Lactate transport and lactate transporters in skeletal muscle. Can. J. Appl. Physiol. 22:531–552, 1997.
9. Bonen, A., and K. J. A. McCullagh. Effects of exercise on lactate transport into mouse skeletal muscles. Can. J. Appl. Physiol. 19:275–285, 1994.
10. Bonen, A., K. J. A. McCullagh, C. T. Putnam, E. Hultman, N. L. Jones, and G. J. F. Heigenhauser. Short-term training increases human muscle MCT1 and femoral venous lactate in relation to muscle lactate. Am. J. Physiol. 274:E102–E107, 1998.
11. Bonen, A., J. C. McDermott, and M. H. Tan. Glycogenesis and glyconeogenesis in skeletal muscle: effects of pH and hormones. Am. J. Physiol. 258:E693–E700, 1990.
12. Brechue, W. F., B. T. Ameredes, J. K. Barclay, and W. N. Stainsby. Blood flow and pressure relationships which determine V̇O2max
. Med. Sci. Sports Exerc. 27:37–42, 1995.
13. Brechue, W. F., J. K. Barclay, D. M. O’Drobinak, and W. N. Stainsby. Differences between V̇O2
maxima of twitch and tetanic contractions are related to blood flow. J. Appl. Physiol. 71:131–135, 1991.
14. Brooks, G. A. Lactate. Glycolytic product and oxidative substrate during sustained exercise in mammals–the “lactate shuttle.” In:Comparative Physiology and Biochemistry: Current Topics and Trends
, Volume A, Respiration-Metabolism-Circulation, R. Gilles (Ed.). Berlin: Springer-Verlag, 1985, pp. 208–218.
15. Brooks, G. A. Lactate production under fully aerobic conditions: the Lactate Shuttle during rest and exercise. Fed. Proc. 45:2924–2929, 1986.
16. Brooks, G. A. The lactate shuttle during exercise and recovery. Med. Sci. Sports Exerc. 18:360–368, 1986.
17. Brooks, G. A. Current concepts in lactate exchange. Med. Sci. Sports Exerc. 23:895–906, 1991.
18. Brooks, G. A. Intra- and extra-cellular shuttles. Med. Sci. Sports Exerc. 32:790–799, 2000.
19. Brooks, G. A., G. E. Butterfield, R. R. Wolfe, et al. Decreased reliance on lactate during exercise after acclimatization to 4,300 m. J. Appl. Physiol. 71:333–341, 1991.
20. Brooks, G. A., E. E. Wolfel, B. M. Groves, et al. Muscle accounts for glucose disposal but not blood lactate appearance during exercise after acclimatization to 4,300 m. J. Appl. Physiol. 72:2435–2445, 1992.
21. Chin, E. R., M. I. Lindinger, and G. J. F. Heigenhauser. Lactate metabolism in inactive skeletal muscle during lactacidosis. Am. J. Physiol. 261:R98–R105, 1991.
22. Dodd, S., S. K. Powers, T. Callender, and E. Brooks. Blood lactate disappearance at various intensities of recovery exercise. J. Appl. Physiol. 57:1462–1465, 1984.
23. Dodd, S. L., S. K. Powers, and M. P. Crawford. Tension development and duty cycle affect Q̇peak
in contracting muscle. Med. Sci. Sports Exerc. 26:997–1002, 1994.
24. Donovan, C. M., and M. J. Pagliassotti. Quantitative assessment of pathways for lactate disposal in skeletal muscle fiber types. Med. Sci. Sports Exerc. 32:772–777, 2000.
25. Donovan, C. M., and G. A. Brooks. Endurance training affects lactate clearance, not lactate production. Am. J. Physiol. 244:E83–E92, 1983.
26. Donovan, C. M., and M. J. Pagliassotti. Endurance training enhances lactate clearance during hyperlactatemia. Am. J. Physiol. 257:E782–E789, 1989.
27. Donovan, C. M., and M. J. Pagliassotti. Enhanced efficiency of lactate removal after endurance training. J. Appl. Physiol. 68:1053–1058, 1990.
28. Dubouchaud, H., P. Granier, J. Mercier, C. Le Peuch, and C. Préfaut. Lactate uptake by skeletal muscle sarcolemmal vesicles decreases after 4 wk of hindlimb unweighting in rats. J. Appl. Physiol. 80:416–421, 1996.
29. Freminet, A., E. Bursaux, and C. F. Poyart. Effect of elevated lactataemia in the rates of lactate turnover and oxidation in rats. Pfluegers Arch. 346:75–86, 1974.
30. Gao, J., J. Ren, E. A. Gulve, and J. O. Holloszy. Additive effect of contractions and insulin on GLUT-4 translocation into the sarcolemma. J. Appl. Physiol. 77:1597–1601, 1994.
31. Gladden, L. B. Lactate uptake by skeletal muscle. Exerc. Sport Sci. Rev. 17:115–155, 1989.
32. Gladden, L. B. Net lactate uptake during progressive steady-level contractions in canine skeletal muscle. J. Appl. Physiol. 71:514–520, 1991.
33. Gladden, L. B. Lactate transport and exchange during exercise. In: Handbook of Physiology. Section 12: Exercise: Regulation and Integration of Multiple Systems, L. B. Rowell and J. T. Shepherd (Eds.). New York: Oxford University Press, 1996, pp. 614–648.
34. Gladden, L. B., R. E. Crawford, and M. J. Webster. Effect of blood flow on net lactate uptake during steady-level contractions in canine skeletal muscle. J. Appl. Physiol. 72:1826–1830, 1992.
35. Gladden, L. B., R. E. Crawford, and M. J. Webster. Effect of lactate concentration and metabolic rate on net lactate uptake by canine skeletal muscle. Am. J. Physiol. 266:R1095–R1101, 1994.
36. Gladden, L. B., R. E. Crawford, M. J. Webster, and P. W. Watt. Rapid tracer lactate influx into canine skeletal muscle. J. Appl. Physiol. 78:205–211, 1995.
37. Gladden, L. B., and J. W. Yates. Lactic acid infusion in dogs: effects of varying infusate pH. J. Appl. Physiol. 54:1254–1260, 1983.
38. Goodyear, L. J., M. F. Hirshman, P. A. King, E. D. Horton, C. M. Thompson, and E. S. Horton. Skeletal muscle plasma membrane glucose transport and glucose transporters after exercise. J. Appl. Physiol. 68:193–198, 1990.
39. Graham, T. E., J. K. Barclay, and B. A. Wilson. Skeletal muscle lactate release and glycolytic intermediates during hypercapnia. J. Appl. Physiol. 60:568–575, 1986.
40. Halestrap, A. P., X. Wang, R. C. Poole, V. N. Jackson, and N. T. Price. Lactate transport in heart in relation to myocardial ischemia. Am. J. Cardiol. 80 (3A):17A–25A, 1997.
41. Hirshman, M. F., H. Wallberg-Henriksson, L. J. Wardzala, E. D. Horton, and E. S. Horton. Acute exercise increases the number of plasma membrane glucose transporters in rat skeletal muscle. FEBS Lett. 238:235–239, 1988.
42. Hundal, H. S., M. J. Rennie, and P. W. Watt. Characteristics of L-glutamine transport in perfused rat skeletal muscle. J. Physiol. (Lond.) 393:283–305, 1987.
43. Issekutz, B., Jr., W. A. S. Shaw, and A. C. Issekutz. Lactate metabolism in resting and exercising dogs. J. Appl. Physiol. 40:312–319, 1976.
44. Jervell, O. Investigation of the concentration of lactic acid in blood and urine under physiologic and pathologic conditions. Acta Med. Scand. Suppl. 24:1–135, 1928.
45. Jorfeldt, L. Metabolism of L(+)-lactate in human skeletal muscle during exercise. Acta Physiol. Scand. Suppl. 338:1–167, 1970.
46. Juel, C. Muscle lactate transport studied in sarcolemmal giant vesicles. Biochim. Biophys. Acta 1065:15–20, 1991.
47. Juel, C. Symmetry and pH dependency of the lactate/proton carrier in skeletal muscle studied with rat sarcolemmal giant vesicles. Biochim. Biophys. Acta 1283:106–110, 1996.
48. Juel, C. Lactate-proton cotransport in skeletal muscle. Physiol. Rev. 77:321–358, 1997.
49. Juel, C., A. Honig, and H. Pilegaard. Muscle lactate transport studied in sarcolemmal giant vesicles: dependence on fibre type and age. Acta Physiol. Scand. 143:361–365, 1991.
50. Juel, C., S. Kristiansen, H. Pilegaard, J. Wojtaszewski, and E. A. Richter. Kinetics of lactate transport in sarcolemmal giant vesicles obtained from human skeletal muscle. J. Appl. Physiol. 76:1031–1036, 1994.
51. Kelley, K. M., J. J. Hamann, W. G. Aschenbach, and L. B. Gladden. Canine gastrocnemius muscle in situ
(Abstract). Med. Sci. Sports Exerc. 28(Suppl):S62, 1996.
52. Koch, A., B. Webster, and S. Lowell. Cellular uptake of L-lactate in mouse diaphragm. Biophys. J. 36:775–796, 1981.
53. Kuikka, J., M. Levin, and J. B. Bassingthwaighte. Multiple tracer dilution estimates of D- and 2-deoxy-D-glucose uptake by the heart. Am. J. Physiol. 250:H29–H42, 1986.
54. MacLean, D. A., B. Saltin, and J. Bangsbo. Interstitial muscle glucose and lactate levels during dynamic exercise in humans determined by microdialysis (Abstract). Pfluegers Arch. 430:240, 1995.
55. MacRae, H. S.-H., S. C. Dennis, A. N. Bosch, and T. D. Noakes. Effects of training on lactate production and removal during progressive exercise in humans. J. Appl. Physiol. 72:1649–1656, 1992.
56. McCullagh, K. J. A., and A. Bonen. Reduced lactate transport in denervated rat skeletal muscle. Am. J. Physiol. 268:R884–R888, 1995.
57. McCullagh, K. J. A., C. Juel, M. O’Brien, and A. Bonen. Chronic muscle stimulation increases lactate transport in rat skeletal muscle. Mol. Cell. Biochem. 156:51–57, 1996.
58. McCullagh, K. J. A., R. C. Poole, A. P. Halestrap, M. O’Brien, and A. Bonen. Role of the lactate transporter (MCT1) in skeletal muscles. Am. J. Physiol. 271:E143–E150, 1996.
59. McCullagh, K. J. A., R. C. Poole, A. P. Halestrap, K. F. Tipton, M. O’Brien, and A. Bonen. Chronic electrical stimulation increases MCT1 and lactate uptake in red and white skeletal muscle. Am. J. Physiol. 273:E239–E246, 1997.
60. McDermott, J. C., and A. Bonen. Endurance training increases skeletal muscle lactate transport. Acta Physiol. Scand. 147:323–327, 1993.
61. McDermott, J. C., and A. Bonen. Lactate transport by skeletal muscle sarcolemmal vesicles. Mol. Cell. Biochem. 122:113–121, 1993.
62. McDermott, J. C., and A. Bonen. Lactate transport in rat sarcolemmal vesicles and intact skeletal muscle, and after muscle contraction. Acta Physiol. Scand. 151:17–28, 1994.
63. McLane, J. A., and J. O. Holloszy. Glycogen synthesis from lactate in the three types of skeletal muscle. J. Biol. Chem. 254:6548–6553, 1979.
64. Nesher, R., I. E. Karl, and D. M. Kipnis. Dissociation of effects of insulin and contraction on glucose transport in rat epitrochlearis muscle. Am. J. Physiol. 249:C226–C232, 1985.
65. Newman, E. V., D. B. Dill, H. T. Edwards, and F. A. Webster. The rate of lactic acid removal in exercise. Am. J. Physiol. 118:457–462, 1937.
66. Pagliassotti, M. J., and C. M. Donovan. Influence of cell heterogeneity on skeletal muscle lactate kinetics. Am. J. Physiol. 258:E625–E634, 1990.
67. Pagliassotti, M. J., and C. Donovan. Role of cell type in net lactate removal by skeletal muscle. Am. J. Physiol. 258:E635–E642, 1990.
68. Pagliassotti, M. J., and C. M. Donovan. Glycogenesis from lactate in rabbit skeletal muscle fiber types. Am. J. Physiol. 258:R903–R911, 1990.
69. Pascoe, D. D., and L. B. Gladden. Muscle glycogen resynthesis after short term, high intensity exercise and resistance exercise. Sports Med. 21:98–118, 1996.
70. Phillips, S. M., H. J. Green, M. A. Tarnopolsky, and S. M. Grant. Increased clearance of lactate after short-term training in men. J. Appl. Physiol. 79:1862–1869, 1995.
71. Pilegaard, H., J. Bangsbo, E. A. Richter, and C. Juel. Lactate transport studied in sarcolemmal giant vesicles from human muscle biopsies: relation to training status. J. Appl. Physiol. 77:1858–1862, 1994.
72. Pilegaard, H., and C. Juel. Lactate transport studied in sarcolemmal giant vesicles from rat skeletal muscles: effect of denervation. Am. J. Physiol. 269:E679–E682, 1995.
73. Pilegaard, H., C. Juel, and F. Wibrand. Lactate transport studied in sarcolemmal giant vesicles from rats: effect of training. Am. J. Physiol. 264:E156–E160, 1993.
74. Poole, R. C., and A. P. Halestrap. Transport of lactate and other monocarboxylates across mammalian plasma membranes. Am. J. Physiol. 264:C761–C782, 1993.
75. Richter, E. A., B. Kiens, B. Saltin, N. J. Christensen, and G. Savard. Skeletal muscle glucose uptake during dynamic exercise in humans: role of muscle mass. Am. J. Physiol. 254:E555–E561, 1988.
76. Roos, A. Intracellular pH and distribution of weak acids across cell membranes: a study of D- and L-lactate and of DMO in rat diaphragm. J. Physiol. (Lond.) 249:1–25, 1975.
77. Roth, D. A. The sarcolemmal lactate transporter: transmembrane determinants of lactate flux. Med. Sci. Sports Exerc. 23:925–934, 1991.
78. Roth, D. A., and G. A. Brooks. Lactate transport is mediated by a membrane-bound carrier in rat skeletal muscle sarcolemmal vesicles. Arch. Biochem. Biophys. 279:377–385, 1990.
79. Roth, D. A., and G. A. Brooks. Lactate and pyruvate transport is dominated by a pH gradient-sensitive carrier in rat skeletal muscle sarcolemmal vesicles. Arch. Biochem. Biophys. 279:386–394, 1990.
80. Shiota, M., S. Golden, and J. Katz. Lactate metabolism in the perfused rat hindlimb. Biochem. J. 222:281–292, 1984.
81. Slentz, C. A., E. A. Gulve, K. J. Rodnick, E. J. Henriksen, J. H. Youn, and J. O. Holloszy. Glucose transporters and maximal transport are increased in endurance-trained rat soleus. J. Appl. Physiol. 73:486–492, 1992.
82. Stainsby, W. N., and P. D. Eitzman. Lactic acid output of cat gastrocnemius-plantaris during repetitive twitch contractions. Med. Sci. Sports Exerc. 18:668–673, 1986.
83. Stanley, W. C., E. W. Gertz, J. A. Wisneski, R. A. Neese, D. L. Morris, and G. A. Brooks. Lactate extraction during net lactate release by the exercising legs of man. J. Appl. Physiol. 60:1116–1120, 1986.
84. Steinhagen, C., H. Hirche, H. W. Nestle, U. Bovenkamp, and I. Hosselmann. The interstitial pH of the working gastrocnemius muscle of the dog. Pfluegers Arch. 367:151–156, 1976.
85. Watt, P. W., L. B. Gladden, H. S. Hundal, and R. E. Crawford. Effects of flow and contraction on lactate transport in the perfused rat hindlimb. Am. J. Physiol. 267:E7–E13, 1994.
86. Watt, P. W., P. A. Maclennan, H. S. Hundal, C. M. Kuret, and M. J. Rennie. L(+)-Lactate transport in perfused rat skeletal muscle: kinetic characteristics and sensitivity to pH and transport inhibitors. Biochim. Biophys. Acta 944:213–222, 1988.
87. Yudilevich, D. L., and G. E. Mann. Unidirectional uptake of substrates at the blood side of secretory epithelia: stomach, salivary gland, pancreas. Fed. Proc. 41:3045–3053, 1982.
Chair: L. Bruce Gladden