We report the case of a young woman with CMV infection, high level of creatine kinase and myopathy. Electromyography showed a myopathic pattern. Muscle biopsy showed a marked increase of NADH enzymatic activity in the central area of almost all type I fibres, few degenerative and necrotic fibres and scattered mononuclear cell infiltrates. Ultrastructural analysis showed a marked disarrangement of sarcomeric structure and large inclusions of thin filaments in some fibres, while immunohistochemistry evidenced alteration in desmin, actin and αB-crystallin protein signals. PCR for CMV detection on muscle sections was negative. Histological, immunological and ultrastructural evaluations were compatible with a necrotic inflammatory myopathy. The correlations between CMV liver infection and the myopathic pattern are discussed. This case underscores the need to consider CMV infection in the differential diagnosis of myopathy with undetermined aetiology, quickly providing directions for a targeted muscle pharmacological intervention.
Viral infections have been frequently reported in association with development of secondary myopathies characterized by different forms of muscle involvement that can vary from mild to severe inflammatory myopathy. Literature reported evidences of nemaline myopathy and myositis after human immunodeficiency infection (HIV) 1, myositis after infection by hepatitis B and C 2, Epstein-Barr virus 3, herpes simplex virus 4 and, less frequently, cytomegalovirus (CMV) 5. Few cases of severe rhabdomyolysis in association with CMV infection 6,7, and a case of polymyositis associated with primary CMV infection were reported 5.
Herein, we describe the case of a young woman with hepatitis by primary CMV infection, muscle weakness, myalgia, oedema and increased serum creatine kinase (CK) levels associated with severe and marked structural alterations in skeletal muscle, whose symptoms improved after immunomodulatory treatment (intravenous immunoglobulin followed by steroid).
Materials and methods
A 29-year-old female, with a medical history of asymptomatic SARS-CoV-2 infection (September 2020) and Raynaud’s syndrome, was hospitalized in February 2021 because of a CMV hepatitis associated with asymmetrical upper limb muscle weakness. She reported a three-week history of asthenia, myalgia, local swelling, marked oedema in the upper limbs and low-grade fever without any dyspnoea or dysphagia. Needle electromyography (EMG) showed myopathic pattern in the proximal and distal muscles of the four limbs with abundant signs of denervation in the active phase. During hospitalization, haematological analyses showed a progressive macrocytic anemia (up to a Hb 8.8 g/dL, MCV 99.7), reduced blood cell count (leukocyte 3.200/μL, platelets 162.000/μL), and high levels of D-dimer, most likely attributable to a systemic inflammatory state. No myoglobinuria was detected.
Laboratory examinations showed an increase in CK (3371 U/L, n.v. = 26-192) and lactate dehydrogenase (LDH = 536 U/L, n.v. = 125-250) levels and a deranged liver function (ALT = 220 U/L and AST = 549 U/L). Renal function was normal. A full body CT-scan indicated a slightly enlarged spleen.
The serological viral panel for CMV, EBV, HCV, HIV showed positivity for CMV (anti-CMV IgG 80.00 U/mL, IgM 53.70 U/mL). RT-PCR investigation for CMV in skeletal muscle was negative. The screening for autoantibodies (ASMA, AMA, ANA, ANCA, ENA, anti CCP, anti ds-DNA, anti-beta2 glycoprotein and rheumatoid factor) was negative and so was the screening for autoimmune myositis (antibodies anti-PL-7, PL-12, SRP, Mi-2, EJ, MDA-5, TIF-g, SAE1, SAE2, NXP-2). There were no skin lesions suggesting dermatomyositis.
The patient was treated with intravenous immunoglobulins 0.4 mg/kg for 5 days and with steroid therapy (methylprednisolone 500 mg intravenous for 5 days followed by oral prednisone 50 mg daily) with progressive improvement of asthenia and normalization of CK levels (58 U/L).
At the follow-up two months after discharge, the patient reported an almost complete recovery, with normal walking also possible on toes and heels. Haematological analyses were within normal range except for platelets (141.000/μL). A control EMG three months after dismissal showed regression of spontaneous activity in both proximal and distal muscles of four limbs, only modest myopathic signs being evident in the right ileopsoas muscle.
Skeletal muscle biopsy from left quadriceps was performed at the Neurologia-Stroke Unit of Lecco Hospital and sent to our Neuromuscular and Rare Disease Unit for histological, immunohistochemical and electron microscopy evaluations.
Muscle sections from patients without any detectable muscle diseases were used as normal controls while muscle sections from three patients with diagnosed inflammatory myopathy served as pathological controls (all patients had signed written informed consent when they had undergone muscle biopsy).
Tissue specimen was frozen in isopentane-cooled liquid nitrogen and processed according to standard techniques, as previously described 8. For histological analysis, 8 μm-thick cryosections were picked and processed for routine staining with Haematoxylin and Eosin (H&E), Modified Gomori Trichrome (MGT), myosin ATPase (pH 9.4-4.6-4.3), cytochrome c oxidase (COX), succinate dehydrogenase (SDH), phosphatase acid (PA), NADH, Oil Red O, Periodic Acid Schiff (PAS) and Congo Red.
For ultrastructural examination, a small part of muscle sample was fixed in 2.5% glutaraldehyde (pH 7.4), post fixed in 2% osmium tetroxide and then, after dehydration in a graded series of ethanol, embedded in Epon’s resin. Finally, ultrathin sections were stained with lead citrate and uranyl acetate and examined with Zeiss EM109 transmission electron microscope.
Immunohistochemical staining was performed for evaluation of inflammatory component using the following mouse monoclonal antibodies: anti-HLA-ABC Antigen/RPE (1:10), anti-MAC (1:50), anti-CD4 (1:50), anti-CD8 (1:10) and anti-CD68 (1:50), all from Dako Agilent (Santa Clara, CA, USA). Mouse monoclonal anti-cytomegalovirus antibody (not diluted, clone CCH2+DDG9; Dako) was used to detect the presence of virus in muscle sections.
For muscle structural evaluation the following antibodies were tested: actin (1:500 rabbit polyclonal; ThermoFisher, Rockford, IL, USA), myotilin (1:10 mouse monoclonal; Novocastra Laboratories, Newcastle upon Tyne, UK), desmin (1:100 mouse monoclonal; Chemicon, Millipore, Billerica, MA, USA), αB-crystallin (1:100 rabbit polyclonal; Chemicon). Slides were then incubated with the appropriate secondary antibody conjugated to Alexa 488 or Alexa 568 (1:200, Invitrogen Life Technologies, Carlsbad, CA, USA).
The outstanding feature of muscle biopsy was the strong increase of NADH enzymatic activity in the central area of almost all type I fibres while subsarcolemmal areas of reduced enzymatic activity were appreciated in rare type I fibres (Fig. 1D). H&E and MGT stains showed a few degenerative and necrotic fibres and scattered mononuclear infiltration (Figs. 1A-B). No centronucleated fibres were observed. Fibres were normal in shape with a physiological variability in size. Endomysial and perimysial connective tissue was normal. Rare splitting fibres were also observed. ATP-ase staining showed a normal distribution of type I and type II fibres. Diffuse and moderate increase in acid phosphatase activity in necrotic fibres and in the interstitial tissue were detected (Fig. 1C). COX activity was reduced in scattered fibres with normal SDH (Figs. 1E-F). No changes in glycogen and lipid content were observed.
Ultrastructural examination showed alteration of sarcomeric structure in several muscle fibres. In particular, we observed three main types of structural changes. In a fair number of fibres, we found thin filamentous inclusions, localized either in the sarcoplasm or at subsarcolemmal level (Figs. 2B, and E). Also, we detected focal areas of myofibrillar disorganization in the centre of otherwise normal muscle fibres (Figs. 2A, C and F). Lastly, as shown in figure 2D, in some areas we observed a disruption of the Z-bands with longitudinal streaming of Z-band material along the sarcomere. Additional observations include a slight increase in lipid droplets (Fig. 2D) and rare lipofuscines (Fig. 2E). Nuclei showed a normal aspect with the exception of those located in the necrotic fibres.
Infiltrating cells were predominantly CD68-positive (Fig. 1G), while rare positivity was observed for CD4 and CD8. Anti-MAC stained some capillaries and anti-HLA showed positivity at the sarcolemma of nearly all muscle fibres and in the cytoplasm of necrotic fibres. Sarcoplasmic HLA-positivity was occasionally observed in some non-necrotic fibres (Figs. 1H-I). No positivity was observed in muscle biopsy tissue from controls.
In addition, several other alterations in fluorescent signals were detected compared to control muscles. In particular, anti-desmin staining showed a discontinuous signal at membrane level as well as a diffuse cytoplasmic signal mostly localized in the central area of several fibres. This positivity was different from the vacuolar staining observed in diagnosed inflammatory myopathies. In control muscles desmin staining was localized only at membrane level (Fig. 3).
Anti-actin staining showed areas of strong positivity in a discrete number of fibres, mainly localized at subsarcolemmal level. No alterations were detectable in both control muscles and in inflammatory myopathy specimens (Fig. 3).
With αB-crystallin staining, many fibres showed a diffuse strong positivity in aggregate-like structures, in some other fibres, however, the staining was localized either in subsarcolemmal areas, or extended to the almost totality of the cytoplasm. This pattern is totally different from what we see in inflammatory myopathies (Fig. 3).
We report the case of a young woman, hospitalized because of a CMV hepatitis and muscle weakness, discharged with a diagnosis of autoimmune myositis. Routine muscle histology was suggestive of a primary necrotizing inflammatory myopathy with peculiar central areas of increased NADH activity in type I fibres. Further investigation by ultrastructural analysis showed, in several fibres, large inclusions of thin filaments, focal areas of myofibrillar disorganization and disruption of the Z-bands with longitudinal streaming of Z-band material along the sarcomere. Immunofluorescence showed marked alterations in desmin, actin and αB-crystallin expression and localization in several fibres.
These findings are quite unique for a primary myositis and, to our knowledge, no cases of similar “secondary myopathies” have ever been associated with CMV hepatitis. A previous single case of muscle weakness, diffuse myalgia with rhabdomyolysis and acute respiratory paralysis probably associated with CMV infection was reported 7.
Although the presence of viral particles has not been confirmed in skeletal muscle by real-time PCR or immunohistochemistry, and the mechanism through which the virus could affect skeletal muscle is still unknown, we can hypothesize that the CMV infection has caused the observed alterations in skeletal muscle as an indirect host-derived effect. Indeed, besides the direct viral liver infection, indirect effects probably mediated by the immunological response can cause detrimental consequences including skeletal muscle alterations 9. However, a possible direct viral muscle infection cannot be completely excluded. Indeed, viral count could have remained below threshold detection level due to methodological limits and/or very low (latent) viral activity when PCR was performed. Ultrastructural changes have been reported in different types of CMV-infected cells as direct effects: in human bone marrow fibroblasts, mitochondrial enlargement, production of dense bodies and cytoplasmic accumulation were observed 10. During in vitro CMV infection, a rapid and progressive alteration of actin, microfilaments and cytoskeleton was observed in both human embryo and lung fibroblasts 11, however what happens in cells and tissues not directly invaded by the virus is still poorly understood.
The clear improvement of the electromyographic pattern following the acute phase, confirms the non-primary nature of the myopathy.
To summarize, several issues – clinical presentation, serological and neurophysiological evidence, skeletal muscle findings and progressive improvement of clinical and instrumental parameters after therapy – favour the hypothesis of an autoimmune/inflammatory myopathy. We could not demonstrate the presence of viral particles in skeletal muscle, but, as explained, an indirect host-derived effect is likely implicated, not to mention concomitance between liver infection and onset of myopathic symptoms.
The study of this case has an important implication for the medical internist approach towards primary CMV viral infection; indeed, the presence of symptoms induced by viral hepatitis could cause underestimation of severe effects on other tissues/organs including skeletal muscle.
Also, our report underscores the need to consider CMV infection in the differential diagnosis of myopathy with undetermined aetiology, providing directions for a targeted muscle pharmacological intervention.
This work is promoted within the European Reference Network for Neuromuscular Diseases (ERN-NMD), MS as HCP Representative for the Italian ERN-NMD.
We also thank the “Bank of muscle tissue, peripheral nerve, DNA and cell culture”, member of Telethon network of Genetic Biobanks, at Fondazione IRCCS Ca’ Granda, Ospedale Maggiore Policlinico, Milano, Italy and the Associazione Amici del Centro Dino Ferrari.
We thank Patrizia Ciscato, BSc, for performing histology-histochemistry reactions. We thank Prof. G. P. Comi, Dr M. Moggio, Dr A. Rigamonti and Dr A. Salmaggi for contribution to discussion.
Figures and tables
- Johnson R, Williams F, Kazi S. Human immunodeficiency virus-associated polymyositis: a longitudinal study of outcome. Arthritis Rheum. 2003;49:172-178. doi:https://doi.org/10.1002/art.11002
- Nojima T, Hirakata M, Sato S. A case of polymyositis associated with hepatitis B infection. Clin Exp Rheumatol. 2000;18:86-88.
- Uchiyama T, Arai K, Yamamoto-Tabata T. Generalized myositis mimicking polymyositis associated with chronic active Epstein-Barr virus infection. J Neurol. 2005;252:519-525. doi:https://doi.org/10.1007/s00415-005-0679-1
- Schlesinger J, Gandara D, Bensch K. Myoglobinuria associated with herpes-group viral infections. Arch Intern Med. 1978;138:422-424.
- Maeda M, Maeda A, Wakiguchi H. Polymyositis associated with primary cytomegalovirus infection. Scand J Infect Dis. 2000;32:212-214. doi:https://doi.org/10.1080/003655400750045367
- Hughes G, Hunt R. Cytomegalovirus infection with rhabdomyolisis and myoglobinuria. Ann Intern Med. 1984;101:276-277. doi:https://doi.org/10.7326/0003-4819-101-2-276_2
- Hirohama D, Shimizu T, Hashimura K. Reversibile respiratory failure due to rhabdomyolysis associated with cytomegalovirus infection. Inter Med. 2008;47. doi:https://doi.org/10.2169/internalmedicine.47.1349
- Napoli L, Crugnola V, Lamperti C. Ultrastructural mitochondrial abnormalities in patients with sporadic amyotrophic lateral sclerosis. Arch Neurol. 2011;68:1612-1613. doi:https://doi.org/10.1001/archneur.68.12.1612
- Freeman R. The ‘indirect’ effects of cytomegalovirus infection. Am J Transplantation. 2009;9:2453-2458. doi:https://doi.org/10.1111/j.1600-6143.2009.02824.x
- Gilloteaux J, Nassiri M. Human bone marrow fibroblasts infected by cytomegalovirus: ultrastructural observations. J Submicrosc Cytol Pathol. 2000;32:17-45.
- Jones N, Lewis J, Kilpatrick B. Cytoskeletal disruption during human cytomegalovirus infection of human lung fibroblasts. Eur J Cell Biol. 1986;41:304-312.
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