Myostatin is a transforming growth factor-ß family member that normally acts to limit skeletal muscle growth. Mice genetically engineered to lack myostatin activity have about twice the amount of muscle mass throughout the body, and similar effects are seen in cattle, sheep, dogs, and a human with naturally occurring loss-of-function mutations in the myostatin gene. Hence, there is considerable interest in developing agents capable of inhibiting myostatin activity for both agricultural and human therapeutic applications. We previously showed that the myostatin binding protein, follistatin, can induce dramatic increases in muscle mass when overexpressed as a transgene in mice. In order to determine whether this effect of follistatin results solely from inhibition of myostatin activity, I analyzed the effect of this transgene in myostatin-null mice. Mstn−/− mice carrying a follistatin transgene had about four times the muscle mass of wild type mice, demonstrating the existence of other regulators of muscle mass with similar activity to myostatin. The greatest effect on muscle mass was observed in offspring of mothers homozygous for the Mstn mutation, raising the possibility that either myostatin itself or a downstream regulator may normally be transferred from the maternal to fetal circulations. These findings demonstrate that the capacity for increasing muscle growth by manipulating TGF-ß signaling pathways is much more extensive than previously appreciated and suggest that muscle mass may be controlled at least in part by a systemic mode of action of myostatin.
Citation: Lee S-J (2007) Quadrupling Muscle Mass in Mice by Targeting TGF-ß Signaling Pathways. PLoS ONE 2(8): e789. doi:10.1371/journal.pone.0000789
Academic Editor: Patrick Callaerts, Katholieke Universiteit Leuven, Belgium
Received: June 1, 2007; Accepted: July 25, 2007; Published: August 29, 2007
Copyright: © 2007 Se-Jin Lee. 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 work was supported by grants from the National Institutes of Health (R01HD35887 and U54AR052646), a grant from the Muscular Dystrophy Association (MDA3765), and a gift from Merck Research Laboratories.
Competing interests: Myostatin was licensed by the Johns Hopkins University to MetaMorphix (MMI) and sublicensed to Wyeth. The author is entitled to a share of sales royalty received by the University from sales of this factor. The Johns Hopkins University and the author also own MMI stock, which is subject to certain restrictions under University policy. The author is a paid consultant to MMI and to Merck. The terms of these arrangements are being managed by the University in accordance with its conflict of interest policies.
Myostatin (MSTN) is a transforming growth factor-ß (TGF-ß) family member that plays a critical role in regulating skeletal muscle mass . Mice engineered to carry a deletion of the Mstn gene have about a doubling of skeletal muscle mass throughout the body as a result of a combination of muscle fiber hyperplasia and hypertrophy . Moreover, loss of myostatin activity resulting either from postnatal inactivation of the Mstn gene ,  or following administration of various myostatin inhibitors to wild type adult mice – can also lead to significant muscle growth. Hence, myostatin appears to play as least two distinct roles, one to regulate the number of muscle fibers that are formed during development and a second to regulate growth of muscle fibers postnatally. The function of myostatin appears to have been conserved across species, as inactivating mutations in the myostatin gene have been demonstrated to cause increased muscling in cattle – , sheep , dogs  and humans . As a result, there has been considerable effort directed at developing strategies to modulate myostatin activity in clinical settings where enhancing muscle growth may be beneficial. In this regard, loss of myostatin activity has been demonstrated to improve muscle mass and function in dystrophic mice – and to have beneficial effects on fat and glucose metabolism in mouse models of obesity and type II diabetes .
Myostatin is synthesized as a precursor protein that undergoes proteolytic processing to generate an N-terminal propeptide and a C-terminal dimer, which is the biologically active species. Following proteolytic processing, the propeptide remains bound to the C-terminal dimer and maintains it in an inactive, latent complex , , , which represents one of the major forms of myostatin that circulates in the blood , . In addition to the propeptide, other binding proteins are capable of regulating myostatin activity in vitro, including follistatin , , FLRG , and Gasp-1 . We previously showed that follistatin can also block myostatin activity in vivo; specifically, we showed that follistatin can ameliorate the cachexia induced by high level expression of myostatin in nude mice  and that transgenic mice expressing follistatin in muscle have dramatic increases in muscle mass . Here, I show that overexpression of follistatin can also cause substantial muscle growth in mice lacking myostatin, demonstrating that other TGF-ß related ligands normally cooperate with myostatin to suppress muscle growth and that the capacity for enhancing muscle growth by targeting this signaling pathway is much larger than previously appreciated.
Increased muscle mass in transgenic mice expressing FLRG
Previous studies have identified several proteins that are normally found in a complex with myostatin in the blood , . One of these is the follistatin related protein, FLRG, which has been demonstrated to be capable of inhibiting myostatin activity in vitro. To determine whether FLRG can also inhibit myostatin activity in vivo, I generated a construct in which the FLRG coding sequence was placed downstream of a myosin light chain promoter/enhancer. From pronuclear injections of this construct, a total of four transgenic mouse lines (Z111A, Z111B, Z116A, and Z116B) were obtained containing independently segregating insertion sites. Each of these four transgenic lines was backcrossed at least 6 times to C57 BL/6 mice prior to analysis in order to control for genetic background effects. Northern analysis revealed that in three of these lines the transgene was expressed in skeletal muscles but not in any of the non-skeletal muscle tissues examined (Figure 1); in the fourth line, Z111B, the expression of the transgene was below the level of detection in these blots. As shown in Table 1, all four lines exhibited significant increases in muscle weights compared to wild type control mice. These increases were observed in all four muscles that were examined as well as in both sexes. Moreover, the rank order of magnitude of these increases correlated with the rank order of expression levels of the transgene; in the highest-expressing line, Z116A, muscle weights were increased by 57–81% in females and 87–116% in males compared to wild type mice. Hence, FLRG is capable of increasing muscle growth in a dose-dependent manner when expressed as a transgene in skeletal muscle.
Total RNA was prepared from various tissues from 10-week old female mice, electrophoresed, blotted, and probed with a fragment derived from SV40 corresponding to the processing/polyadenylation sequences present in the transgenic construct. The blots were re-hybridized with a probe for the S26 ribosomal protein to control for loading.
To determine whether the FLRG transgene was causing increased muscle growth by blocking myostatin activity, I examined the effect of combining the FLRG transgene with a loss-of-function mutation in the myostatin gene. To date, using the Z116A line, I have not been able to generate mice that are both positive for the transgene and homozygous for the myostatin deletion mutation. However, I did obtain a number of female Z116A transgenic mice that were heterozygous for the myostatin mutation, and as shown in Table 1 and Figure 2a, these mice exhibited further increases in muscle weights compared to Z116A mice that were wild type for myostatin. Most importantly, in two of the muscles that were examined (quadriceps and gastrocnemius) the observed increases were also greater than those seen in Mstn−/− mice lacking the transgene. Based on this finding, it appears that myostatin cannot be the sole target for FLRG in the transgenic mice and, therefore, that additional ligands must be capable of suppressing muscle growth in vivo.
Numbers represent percent increases relative to wild type mice and were calculated from the data shown in Table 1. (C) Distribution of fiber diameters. Gray bars represent muscles from wild type mice, and red bars represent muscles from Mstn−/−, F66, and F66/Mstn−/− mice.
Effect of follistatin in Mstn null mice
Because I was unable to examine the effect of overexpressing FLRG in the complete absence of myostatin, it was difficult to ascertain the relative importance of these additional ligands compared to myostatin in regulating muscle mass. However, I carried out a similar set of experiments utilizing follistatin transgenic mice, which demonstrated that these additional ligands do play a major role in suppressing muscle growth. In previous studies, we had generated several transgenic founders expressing follistatin from a myosin light chain promoter/enhancer . I was able to establish a transgenic line from one of these founders (F66), and I backcrossed this line extensively to C57 BL/6 mice for subsequent analysis. In this line, the transgene was most likely located on the Y chromosome, as the transgene was transmitted to all of the male offspring and none of the female offspring. F66 transgenic mice were mated with Mstn mutant mice, and F66/Mstn+/− males were then mated with either Mstn+/− or Mstn−/− females. As shown in Table 1, the presence of one or two Mstn mutant alleles in combination with the F66 transgene resulted in increasingly more muscle mass than seen in F66 transgenic mice that were wild type for Mstn. Moreover, muscle weights in either F66/Mstn+/− or F66/Mstn−/− mice were dramatically higher than in Mstn−/− mice lacking the F66 transgene. In the most extreme case, muscle weights in F66/Mstn−/− mice were increased by 250–350% from those seen in wild type mice (Figures 2b and 3). Hence, the presence of the F66 transgene in a Mstn−/− background caused yet another doubling of muscle weights, resulting in mice with approximately quadruple the normal amount of muscle. These findings demonstrate that like FLRG, follistatin must be exerting its effect on muscle growth by targeting other ligands in addition to myostatin and that the effect of blocking these other ligands is comparable in magnitude to that resulting from loss of myostatin.
In previous studies, we showed that the increase in muscle mass in Mstn−/− mice results from a combination of increased fiber numbers and increased fiber sizes . To determine whether the same is true for the additional muscle mass seen upon introduction of the F66 transgene, I carried out morphometric analysis of the gastrocnemius/plantaris muscles. As shown in Table 2 and Figure 2c, total fiber number and mean fiber diameter were increased by about 48% and 19%, respectively, in Mstn−/− mice compared to wild type mice. As the cross-sectional area of the muscle would be expected to be roughly proportional to the square of the diameter, increased fiber diameter in Mstn−/− mice would correspond to an approximately 43% increase in fiber mass. Hence, muscle fiber hyperplasia and hypertrophy appear to contribute roughly equally to give the overall doubling of gastrocnemius/plantaris mass in Mstn−/− mice. In contrast, a similar analysis of F66 transgenic mice revealed that although total fiber number was increased slightly (16%), the overall increase in gastrocnemius/plantaris mass resulted almost entirely from muscle fiber hypertrophy (93% increase in cross-sectional area). In mice in which the F66 transgene was combined with the Mstn null mutation, the two phenotypes appeared to be additive; that is, the quadrupling of muscle mass in F66/Mstn−/− mice resulted from an approximately 73% increase in fiber number and 117% increase in fiber cross-sectional area. These results suggest that the additional muscle mass induced by follistatin in Mstn null mice results from inhibition of additional ligands that act predominantly to regulate muscle fiber growth.
Maternal effect of the Mstn null mutation
In the experiments with F66 transgenic mice, a consistent finding was that muscle weights were higher in animals of the same genotype if they arose from crosses in which the mother had fewer functional Mstn alleles (Table 1). This maternal effect was observed to some extent in all of the muscles examined but was most pronounced in the quadriceps and gastrocnemius. For example, muscle weights of F66/Mstn+/+ males obtained from crosses with Mstn+/− females were higher than those of F66/Mstn+/+ males obtained from crosses with Mstn+/+ females. Similarly, muscle weights of F66/Mstn+/− males obtained from crosses with Mstn−/− females were higher than those of F66/Mstn+/− males obtained from crosses with Mstn+/− females. The most dramatic effects were observed in F66/Mstn−/− mice obtained from crosses with Mstn−/− females, in which muscle weights were approximately quadrupled compared to wild type mice.
To determine whether this maternal effect was specific to the presence of the F66 transgene, I carried out a variety of crosses of Mstn mutant mice lacking the transgene. As shown in Table 3, the maternal effect on muscle weights was observed in these crosses as well. In virtually every case, mice with identical genotypes exhibited higher muscle weights if the mother had fewer functional Mstn alleles. The most clear cut results were obtained in analyses of Mstn+/− offspring derived from crosses of Mstn+/+ males with Mstn−/− females, which showed significantly higher muscle weights than Mstn+/− offspring derived from crosses of Mstn−/− males with Mstn+/+ females. Hence, the maternal effect on muscle mass was not dependent on the presence of the F66 transgene.
Conceivably, this maternal effect could result from transfer of myostatin or a downstream mediator either prenatally from the maternal to fetal circulations or postnatally from the mother to the offspring during nursing; in this respect, myostatin mRNA has been reported to be expressed in the mammary gland of lactating pigs . To distinguish these two possibilities, I analyzed the effect of transferring neonates obtained from crosses with mothers of one Mstn genotype to foster mothers of a different Mstn genotype. In these experiments, all transfers were carried out using neonatal mice less than 24 hours old to mothers that had delivered their own litters also within the previous 24 hours. In order to control for effects of the transfer process per se, I also carried out transfers of neonates obtained from crosses with mothers of one Mstn genotype to foster mothers of the same Mstn genotype. As shown in Table 4, mice of a given genotype and parentage exhibited comparable muscle weights regardless of the genotype of the foster mothers. Hence, if there is a mediator of muscle mass that is transferred through the milk, I was not able to detect any resultant effects on muscle mass in these experiments. Taken together, these results suggest that the maternal effect on muscle mass results most likely from prenatal transfer of some mediator from mother to fetus, perhaps myostatin itself.
Based on the data presented here, two important conclusions can be drawn. The first is that the Mstn loss-of-function mutation exerts a maternal effect such that muscle mass of the fetus is influenced by the number of functional Mstn alleles in the mother. Specifically, I show that offspring with identical Mstn genotypes have higher muscle weights if the mother has fewer functional Mstn alleles. This finding taken together with the results of cross fostering experiments suggest that muscle mass can be influenced by prenatal transfer of some mediator from mother to fetus; although myostatin itself is the most obvious candidate for this mediator, additional experiments will be required to prove this definitively.
We showed previously that myostatin circulates in the blood and that systemic effects can be achieved by implanting myostatin-expressing cells into a single site in the lower limb ; however, there have been no experiments that have demonstrated conclusively that myostatin normally acts systemically. The demonstration that maternal effects can be seen in offspring of mice lacking myostatin is consistent with the possibility that the circulating myostatin protein can enter the active pool. If myostatin does act systemically, the implication would be that local control of muscle growth can be influenced at least in part by myostatin being produced elsewhere in the body and that myostatin functions precisely as a chalone, as originally hypothesized by Bullough ,  for the control for tissue growth in general. This is a critical issue, as it relates to the fundamental reason that the control of muscle growth may have evolved into this rather complex regulatory system. In this respect, I speculated previously that perhaps the myostatin regulatory system may serve two distinct functions, one to regulate local growth of muscle in response to specific physiological stimuli, such as injury, and a second to regulate the overall metabolic balance between fat and muscle in response to general physiological stimuli, such as nutritional status . According to this model, local control of muscle growth would be achieved by regulating the extent to which the latent form of myostatin is activated at the target site, whereas global control of the metabolic homeostatic balance between muscle and other tissues would be achieved by regulating the size of the circulating pool of myostatin.
The second important finding presented here is the demonstration that other ligands work with myostatin to control muscle growth. I have presented data showing that FLRG, like follistatin, can promote muscle growth when expressed as a transgene in skeletal muscle and that both of these molecules appear to act by blocking not only myostatin but also other ligands with similar activity to myostatin. By combining the follistatin transgene with a myostatin null mutation, I have been able to generate mice with quadrupled muscle mass, which represents yet another doubling of muscle mass compared to mice only lacking myostatin. These studies demonstrate that muscle mass in mice is controlled by multiple members of the transforming growth factor-ß superfamily acting in concert. We reached a similar conclusion in an earlier study in which we demonstrated that administration of a soluble form of the ACVR2B receptor to wild type could cause more extensive muscle growth than what had been observed previously using myostatin-specific inhibitors and that this soluble receptor could also increase muscle growth even in mice completely lacking myostatin . The studies presented here demonstrate that the capacity for promoting muscle growth by targeting this general signaling pathway is far greater than previously appreciated.
Because myostatin normally acts to limit muscle growth, there has been considerable interest in targeting this pathway to attempt to enhance muscle growth in human patients with muscle wasting and muscle degenerative diseases. Most efforts in this regard have focused on agents capable of binding specifically to myostatin and inhibiting its activity. The finding that myostatin is not the sole regulator of muscle mass in mice raises the question as to whether targeting myostatin alone will be the most effective strategy for manipulating this signaling pathway in humans. In this respect, it is known that the circulating levels of myostatin protein in humans are considerably lower than in mice , , raising the possibility that the balance of the relative roles played by myostatin and by these other regulators may have shifted further away from myostatin in humans compared to mice. For these reasons, it will be essential to determine the identity of the other ligand or ligands that cooperate with myostatin, as only then will we be able to develop the best possible strategies for manipulating this pathway for the treatment of human diseases in which promoting muscle growth may be beneficial.
Materials and Methods
Pronuclear injections of DNA and embryo transfers were carried out by the Johns Hopkins Transgenic Core Facility. Mstn mutant and F66 and FLRG transgenic mice were backcrossed at least 6 times onto a C57 BL/6 background prior to analysis. All analysis was carried out on 10 week old mice. For measurement of muscle weights, individual muscles from both sides of the animal were dissected, and the average weight was used for each muscle. For morphometric analysis, the gastrocnemius and plantaris muscles were sectioned serially to their widest point using a cryostat, and fiber diameters were measured (as the shortest distance across the fiber passing through the midpoint) from hematoxylin and eosin stained sections. Measurements were carried out on 250 fibers per animal, and all data for a given genotype were pooled.
I thank Kunihiro Tsuchida for providing the FLRG cDNA clone, the Johns Hopkins Transgenic Core Facility for carrying out the pronuclear injections and embryo transfers, and Will Kirk and Jay VanRensselaer for photography of mice.
Conceived and designed the experiments: SL. Performed the experiments: SL. Analyzed the data: SL. Contributed reagents/materials/analysis tools: SL. Wrote the paper: SL.
- 1. Lee S-J (2004) Regulation of muscle mass by myostatin. Annu Rev Cell Dev Biol 20: 61–86.
- 2. McPherron AC, Lawler AM, Lee S-J (1997) Regulation of skeletal muscle mass in mice by a new TGF-ß superfamily member. Nature 387: 83–90.
- 3. Grobet L, Pirottin D, Farnir F, Poncelet D, Royo LJ, et al. (2003) Modulating skeletal muscle mass by postnatal, muscle-specific inactivation gene. Genesis 35: 227–238.
- 4. Welle S, Bhatt K, Pinkert C, Tawil R, Thornton C (2007) Muscle growth after postdevelopmental myostatin gene knockout. Am J Physiol Endocrinol Metab 292: E985–991.
- 5. Whittemore L-A, Song K, Li X, Aghajanian J, Davies MV, et al. (2003) Inhibition of myostatin in adult mice increases skeletal muscle mass and strength. BBRC 300: 965–971.
- 6. Wolfman NM, McPherron AC, Pappano WN, Davies MV, Song K, et al. (2003) Activation of latent myostatin by the BMP-1/tolloid family of metaloproteinases. Proc Natl Acad Sci USA 100: 15842–15846.
- 7. Lee S-J, Reed A, Davies M, Girgenrath S, Goad M, et al. (2005) Regulation of muscle growth by multiple ligands signaling through activin type II receptors. Proc Natl Acad Sci USA 102: 18117–18122.
- 8. Grobet L, Martin LJR, Poncelet D, Pirottin D, Brouwers B, et al. (1997) A deletion in the bovine myostatin gene causes the double-muscled phenotype in cattle. Nature Genet 17: 71–74.
- 9. Kambadur R, Sharma M, Smith TPL, Bass JJ (1997) Mutations in myostatin (GDF8) in double-muscled Belgian Blue and Piedmontese cattle. Genome Res 7: 910–915.
- 10. McPherron AC, Lee S-J (1997) Double muscling in cattle due to mutations in the myostatin gene. Proc Natl Acad Sci USA 94: 12457–12461.
- 11. Grobet L, Poncelet D, Royo LJ, Brouwers B, Pirottin D, et al. (1998) Molecular definition of an allelic series of mutations disrupting the myostatin function and causing double-muscling in cattle. Mamm Genome 9: 210–213.
- 12. Clop A, Marcq F, Takeda H, Pirottin D, Tordoir X, et al. (2006) A mutation creating a potential illegitimate microRNA target site in the myostatin gene affects muscularity in sheep. Nature Genet 38: 813–818.
- 13. Mosher DS, Quignon P, Bustamante CD, Sutter NB, Mellersh CS, et al. (2007) A mutation in the myostatin gene increases muscle mass and enhances racing performance in heterozygote dogs. PloS Genet 3: e79. doi:10.1371/journal.pgen.0030079.
- 14. Schuelke M, Wagner KR, Stolz LE, Hübner C, Riebel T, et al. (2004) Myostatin mutation associated with gross muscle hypertrophy in a child. N Engl J Med 350: 2682–2688.
- 15. Bogdanovich S, Krag TOB, Barton ER, Morris LD, Whittemore L-A, et al. (2002) Functional improvement of dystrophic muscle by myostatin blockade. Nature 420: 418–421.
- 16. Wagner KR, McPherron AC, Winik N, Lee S-J (2002) Loss of myostatin attenuates severity of muscular dystrophy in mdx mice. Ann Neurol 52: 832–836.
- 17. Bogdanovich S, Perkins K, Krag T, Whittemore L-A, Khurana T (2005) Myostatin propeptide-mediated ameliortion of dystophic pathophysiology. FASEB J 19: 543–549.
- 18. McPherron AC, Lee S-J (2002) Suppression of body fat accumulation in myostatin-deficient mice. J Clin Invest 109: 595–601.
- 19. Lee S-J, McPherron AC (2001) Regulation of myostatin activity and muscle growth. Proc Natl Acad Sci USA 98: 9306–9311.
- 20. Thies RS, Chen T, Davies MV, Tomkinson KN, Pearson AA, et al. (2001) GDF-8 propeptide binds to GDF-8 and antagonizes biological activity by inhibiting GDF-8 receptor binding. Growth Factors 18: 251–259.
- 21. Zimmers TA, Davies MV, Koniaris LG, Haynes P, Esquela AF, et al. (2002) Induction of cachexia in mice by systemically administered myostatin. Science 296: 1486–1488.
- 22. Hill JJ, Davies MV, Pearson AA, Wang JH, Hewick RM, et al. (2002) The myostatin propeptide and the follistatin-related gene are inhibitory binding proteins of myostatin in normal serum. J Biol Chem 277: 40735–40741.
- 23. Hill JJ, Qiu Y, Hewick RM, Wolfman NM (2003) Regulation of myostatin in vivo by growth and differentiation factor-associated serum protein-1: a novel protein with protease inhibitor and follistatin domains. Mol Endocrinol 17: 1144–1154.
- 24. Ji S, Losinski RL, Cornelius SG, Frank GR, Willis GM, et al. (1998) Myostatin expression in porcine tissues: tissue specificity and developmental and postnatal regulation. Am J Physiol 275: R1265–1273.
- 25. Bullough WS (1962) The control of mitotic activity in adult mammalian tissues. Biol Rev 37: 307–342.
- 26. Bullough WS (1965) Mitotic and functional homeostasis: A speculative review. Cancer Res 25: 1683–1727.