Niko Hensel
Sabrina Kubinski1,2
Peter Claus- 1Institute of Neuroanatomy and Cell Biology, Hannover Medical School, Hannover, Germany
- 2Center of Systems Neuroscience (ZSN), Hannover, Germany
Spinal Muscular Atrophy (SMA) is monogenic motoneuron disease caused by low levels of the Survival of Motoneuron protein (SMN). Recently, two different drugs were approved for the treatment of the disease. The antisense oligonucleotide Nusinersen/Spinraza® and the gene replacement therapy Onasemnogene Abeparvovec/Zolgensma® both enhance SMN levels. These treatments result in impressive benefits for the patients. However, there is a significant number of non-responders and an intervention delay has a strong negative impact on the efficacy. Obviously, later stages of motoneuron degeneration cannot be reversed by SMN-restoration. Therefore, complementary, SMN-independent strategies are needed which are able to address such SMN-irreversible degenerative processes. Those are defined as pathological alterations which are not reversed by SMN-restoration for a given dose and intervention delay. It is crucial to tailor SMN-independent approaches to the novel clinical situation with SMN-restoring treatments. On the molecular level, such SMN-irreversible changes become manifest in altered signaling modules as described by molecular systems biology. Based on our current knowledge about altered signaling, we introduce a network approach for an informed decision for the most potent SMN-independent treatment targets. Finally, we present recommendations for the identification of novel treatments which can be combined with SMN-restoring drugs.
Introduction
Spinal Muscular Atrophy (SMA) is a monogenic, autosomal recessive neurodegenerative disease. It has an incidence of 1:6,000−1:10,000, preferentially affects infants and is the most common rare disease in this age cohort (1, 2). The second motoneurons in the spinal cord and brain stem degenerate in SMA patients, resulting in fatigue, paralysis, and atrophy of the proximal muscles (3, 4). Patients harbor homozygous deletions or mutations of the Survival of Motoneuron1 (SMN1) gene. The lack of the corresponding SMN protein causes SMA (5). However, all humans comprise a second very similar gene, SMN2, which encodes the same SMN protein. SMN2 differs from SMN1 in some mutations with a translational silent cytosine to thymine transition within exon 7 (6). This leads to an altered splicing of the vast majority of the SMN2 pre-mRNA resulting in a shortened transcript which lacks exon 7 (Δ7 mRNA) and only a few transcripts of the mature full length SMN2 mRNA (7). While the full-length protein is stable, the SMNΔ7 protein is rapidly degraded. As a consequence, SMN2 produces only about 10–15% of the protein amount compared to SMN1. The SMN2 gene is not able to fully compensate the SMN1 loss in patients leading to the preferential degeneration of motoneurons (6, 7).
The number of the SMN2 gene copies is the most potent genetic modifier of SMA severity (8): the number of gene copies negatively correlates with disease severity. SMA is divided into five different subtypes based on the clinical picture and defined by the age of disease onset, the life expectancy and the motor function milestones which the patients are able to reach (9–11). The most severely affected SMA type 0 patients decease before or within the first month after birth (12). The most common subtype is the severe SMA type 1 with symptoms occurring within the first 3 months after birth. These Patients never gain the ability to sit or to control their head and die within the first 2 to 3 years of life (11, 13). Intermediate type 2 patients show the first symptoms in early childhood between the sixth and eighteenth months of age, are never able to stand and suffer from a marked reduction of life-expectancy (10). Symptoms in mild subtype 3, the juvenile form, typically occur after 18 months of age and these patients can stand and walk independently (10, 11, 14). In contrast, type 4 patients show mild muscle weakness symptoms in adulthood (10).
SMN is a multifunctional protein which localizes to the nucleus, cytoplasm, axon, and the neuromuscular junction (15–18). The loss of more than one of these functions likely contributes to motoneuron degeneration. The multifunctionality of SMN has been excellently reviewed elsewhere (19). Here, we exemplify two different functions: SMN is part of the machinery which assembles spliceosomal components (20). It has been hypothesized that this leads to a general splice deficiency and that motoneurons are specifically sensitive to that (21). However, splicing is not a process which is restricted to neurons or motoneurons. It may thus be possible that this is the “housekeeping” function of the SMN protein affecting all cells and organs. A more specific function is the involvement of the SMN protein in the neuronal actin cytoskeleton (22). SMN directly interacts with profilin2a, an actin-binding protein which is specifically expressed in neurons (23–25). A lack of the SMN protein leads to enhanced accessibility of profilin2a for its upstream Rho-kinase (ROCK). As a consequence, profilin2a becomes hyper-phosphorylated inducing a neuron-specific dysregulation of the actin cytoskeleton (22, 25–27).
The exact molecular mechanism of motoneuron degeneration remains elusive. However, pathohistology reveals distinct degenerative phenotypes in SMA patients which allow reconstructing a “natural history” of motoneuron degeneration (28). The pathohistology of SMA type 1 patients' spinal cords reveals two prominent characteristics of neurodegeneration: a loss of motoneurons in the anterior horn and a chromatolysis of some of the remaining motoneurons (29). The latter is a distinct degenerative process characterized by the loss of rough endoplasmic reticulum and a displacement of the nucleus toward the cell body periphery (30). Chromatolysis in SMA hints for a distal pathology with an axonal damage—an axotomy is the most simple method to experimentally induce chromatolysis in motoneurons (30). In such models, chromatolysis occurs before regeneration and degeneration. Thus, it is supposed that chromatolytic neurons are on the verge of cell death but that a regenerative potential remains. However, it is unclear whether chromatolytic motoneurons can be rescued or not in SMA. Evidence for an axonal dying back mechanism came from studies in fetuses predicted to develop SMA. Muscle histology revealed altered neuromuscular junction phenotypes (31). Moreover, central synapses were altered in pre-symptomatic SMA mice indicating a synaptic pathology (32). Thus, there may be a functional motoneuron degeneration preceding the loss of motoneurons which has been observed in post mortem pathohistology. However, such studies indicated even earlier perturbations in motoneuron development: SMA type 1 and 2 patients displayed heterotopic motoneurons with a round-shaped migratory phenotype and an abnormal localization at the anterior rim of the spinal cord (28).
The SMN protein is ubiquitously expressed and it is not surprising that a lack of SMN protein affects peripheral organs in SMA patients. Those include metabolic alterations (33), muscle (34), heart (35), vasculature (36, 37), pancreas (38), and liver (39). Accordingly, SMA is considered to be a multi-system disease (40, 41). However, motor impairments and muscle atrophy are severe conditions in patients. It is difficult to dissect peripheral organ-intrinsic pathomechanisms from the neuromuscular phenotype. In experimental SMA models, such as SMA mice, it is possible to perform an organ or cell-specific rescue approach which selectively restores SMN protein levels in single cell types. Thereby, some studies showed cell- or organ-intrinsic pathomechanisms including muscle (42, 43) and astrocytes (44). Considering the relation between SMN levels and peripheral organs it has been suggested that there are cell or organ-specific SMN thresholds needed for proper organ function (45). However, motoneurons are preferentially affected independent of the clinical type and are thus an important and common therapeutic target. An elevation of SMN levels in the spinal cord has been a successful strategy for novel therapeutics approved recently.
In this state-of-the-art review, we focus on the approved compounds Nusinersen/Spinraza® and Onasemnogene Abeparvovec/Zolgensma® which both enhance SMN levels in the central nervous system (CNS). Thereby, we exemplify that (i) central SMN-restoration in the CNS is important but may not be sufficient because (ii) a peripheral SMN-restoration may be needed in patients with very low peripheral SMN levels. Moreover, (iii) a SMN-independent regeneration has to be considered in patients with a delayed therapeutic intervention. We will then focus on such SMN-independent approaches. Moreover, we review pre-clinical studies which used interventions in cellular signaling as a strategy to identify SMN-independent treatment options. Thereby, we include pathways with evidence from mammalian SMA models only. Finally, we summarize the experience with SMN-independent pre-clinical approaches with a set of recommendations for their future identification.
Current Therapies Focus on SMN Levels in the CNS: The Importance of Peripheral SMN-Restoration and SMN-Independent Regeneration for Future Therapies
Since the identification of the causality between SMN protein loss and SMA, many treatment strategies focused on restoring SMN levels. Those strategies are generally termed “SMN-dependent.” Since motoneurons are preferentially affected independent of the clinical subtype, they are a common target for a SMN-restoration in the central nervous system and this strategy is important for all SMA cases irrespective of the severity (Table 1). In December 2016, the first treatment for all clinical subtypes of SMA was approved by the US Food and Drug Administration (FDA) and half a year later for Europe as well. The drug Nusinersen/Spinraza® is an antisense oligonucleotide (ASO) which does not cross the blood-brain-barrier. The ASO is directly administered to the CNS by lumbar puncture into the cerebrospinal fluid (CSF) where it enhances central SMN levels only (46). On the molecular level, Nusinersen/Spinraza® modulates the deficient SMN2 pre-mRNA splicing to restore SMN protein levels (47). The half-life time of the ASO within the spinal cord of non-human primates is about 140 days allowing a reduction of application burden by lumbar punctures (48). Currently, Nusinersen/Spinraza® is administered to SMA patients by four loading doses followed by maintenance doses every 4 months (49). In a phase-I study, Nusinersen/Spinraza® enhanced the survival compared to natural history data. The ASO was detected in neurons and glia cells of deceased SMA patients' spinal cords where it induced exon 7 inclusion (46). However, low ASO-levels could also be found in blood indicating some leakiness during the ASO administration procedure or a subsequent CSF clearance into the blood (49, 50). Although there was a significant number of non-responders during the observation period of a placebo-controlled study, over 70% of treated infants improved motor functions and the risk of death or permanent assisted ventilation dropped by 47% compared to the placebo group (49).
Table 1. Severity and time point of intervention critically determines the treatment strategy.
In 2019, the FDA approved Onasemnogene Abeparvovec/Zolgensma®, an Adeno-associated virus 9 (AAV9) delivering a cDNA which codes for the SMN protein, as a gene replacement therapy. Onasemnogene Abeparvovec/Zolgensma® is systemically applied to children less than 2 years. So far, there is one published phase-I study with the AAV9 employed at two different doses which resulted in improvements in motor function and survival compared to natural history data (51). The AAV9 crosses the blood-brain barrier which induces SMN expression in the CNS and in peripheral organs. However, human bioavailability data have not been published so far. Moreover, AAV9 does not integrate into the genome which leads to a dilution effect in mitotic cells. As a consequence, a SMN-restoration by a gene replacement therapy may be of limited sustainability in the periphery. However, in the light of the multi-system character of SMA, a peripheral SMN-restoration may be needed complementing the central SMN-restoration in the CNS (Table 1). According to the hypothesis of organ-specific SMN thresholds, severely affected children with very low peripheral SMN levels are potentially at risk of multi-organ defects while this could be less relevant in milder affected patients.
Importantly, the beneficial effects of Nusinersen/Spinraza® are dependent on disease duration at the time of intervention: the shorter the infants were symptomatic before treatment; the higher was the survival without permanent ventilation as well as the improvement of motor functions (49, 52). This effect was strongest in pre-symptomatic patients with two or three SMN2 copies resulting in impressive benefits and the achievement of motor milestones such as independent walking (53). Similarly, patients treated early with Onasemnogene Abeparvovec/Zolgensma® performed better compared to patients with delayed intervention (51). Taken together, this confirms a number of pre-clinical studies which employed SMN-dependent treatment strategies in SMA mice: disease duration before treatment is critical and a delayed intervention leads to a less efficient rescue (54). This and the occurrence of non-responders clearly demonstrate pathological processes which cannot be reversed by enhancing SMN protein levels and that they increase in number and/or severity with prolonged intervention delay (Figure 1). It is unclear which pathological changes underlie this SMN-irreversibility. However, the complete loss of a motoneuron is a clearly irreversible change. Moreover, this constitutes a severe problem if no newborn screening becomes implemented and for milder affected SMA patients which are symptomatic for years. Complementary strategies are needed which are not based on enhanced SMN protein expression—since this is already accomplished by Nusinersen/Spinraza® or Onasemnogene Abeparvovec/Zolgensma®—but reverse pathological changes independent of SMN (Table 1).
Figure 1. Model for motoneuron degeneration and the underlying signaling network in SMA. Motoneuron loss observed in post mortem analyses is preceded by a functional degeneration of central synapses and the neuromuscular junction. The subsequent axonal damage induces a chromatolytic phenotype of the motoneurons. During disease progression those processes become less reversible indicated by a reduced regenerative capacity. This is reflected by a growing network of dysregulated signaling nodes with an increased fraction of SMN-irreversible (black) vs. SMN-reversible (blue) signaling mediators. SMN-restoration restores blue nodes only. The relative number of SMN-restorable nodes becomes reduced over time as illustrated in this hypothetical scheme. Highly connected SMN-irreversible (black) nodes may be potent treatment targets (arrow). Those nodes may be critical regulators for a module involved in a specific degenerative process.
An “SMN-Independent Treatment Approach” Does not Necessarily Mean That it is Independent From SMN Levels: The Importance of SMN-Irreversible Processes
Since the introduction of SMN-enhancing drugs with an impressive but yet limited effect, SMN-independent treatment approaches attained more attention. Those could be combined with SMN-enhancing drugs for defined patient cohorts (Table 1). However, the definition of an “SMN-independent treatment approach” is not clear yet. Sometimes, a strategy which does not involve the increase of the SMN protein level is included in such definition. This is misleading because there might be strategies which do not rely on enhanced SMN levels but are still SMN-dependent. For example, inhibition of Rho-kinase (ROCK) activity (see below) could be considered as an SMN-independent treatment strategy. However, its activity toward different downstream targets has been demonstrated to be SMN-dependent by direct interaction of SMN with profilin2a, a ROCK binding protein (25). Neurodegeneration could elicit pathway and network perturbations which could not be restored by therapeutic SMN-enhancing intervention (Figure 1). Those signaling modules represent important putative targets for combinatorial treatments. For an optimal outcome, treatment strategies should be adapted to specific pathological changes of a disease. In principle, it is possible that SMN restoration induces a regenerative process which abrogates those changes: the pathological process or symptom may be reversed. Thus, SMN-independent strategies should focus on treatment targets which are SMN-irreversible (Figure 1). A pathomechanistic SMN-reversible change may have already changed back to normal levels by application of antisense oligonucleotide or gene replacement therapies so that there is no process to reverse anymore. This also applies to strategies which target peripheral tissues without enhancing SMN levels. Pre-clinical studies in SMA mice specifically target muscle function with myostatin inhibitors enhancing body- and muscle weight. However, the clinically relevant impact on motor functions is unclear yet (55, 56). Moreover, SMN-irreversibility of the underlying pathological changes such as the loss of muscle function has not been reported so far: It is possible that a central and peripheral restoration of the SMN levels may enhance the muscle functions in a way that myostatin inhibition would not have an extra benefit. As seen by the better response of early treated patients, SMN-irreversibility critically depends on the intervention delay. Thus, an appropriate SMN-independent treatment strategy must rely on a given intervention delay (Figure 1): In fact, a pre-clinical pipeline for the development of combinatorial treatment approaches should detect alterations downstream of SMN deficiency to identify a specific pathomechanistic change (a target), test its SMN-irreversibility in a model reflecting the clinical situation with delayed intervention, and show robust pathophysiological benefits when rescued. In the last years, we and others identified several signaling pathways which are potential treatment targets for Spinal Muscular Atrophy without changing SMN levels. However, there are only limited reports about their SMN-irreversibility.
Intervention in Cellular Signaling as a Strategy for SMN-Independent Treatment Approaches: A Skeptical View on our Current Knowledge About Pathways
There are a number of potential SMA treatment approaches which rely on their interference with cellular signaling. Thereby, two different strategies have been followed: approaches which interfere with an altered pathway downstream of SMN-deficiency and potential treatments focusing on unchanged pathways in SMA. The latter are more likely to be unaffected by SMN-restoration but may be less efficient. However, SMN-irreversibility of these approaches has not been tested yet and this is a pre-requisite for their SMN-independency. Those include the Rho kinase (ROCK) (25, 62–65), the extracellular regulated kinase (ERK) (62, 63, 66, 67), the c-Jun N-terminal Kinase (JNK) (68, 69), and the p53-pathway (70) (Box 1). The Phosphatase and tensin homolog (PTEN) pathway was not altered in SMA but its inhibition may exert some beneficial effects (71). PTEN is a pro-apoptotic protein, involved in Akt signaling. In an ischemic rat model, the death of hippocampal neurons was inhibited by decreased PTEN activity demonstrating general neuroprotective properties of PTEN inhibition (72). However, there are no findings of an altered PTEN signaling in SMA mice. A systemic AAV-based knock-down strategy led to a modest effect on survival and motor functions in SMNΔ7 mice (71). However, it is unclear whether motoneurons mediate those beneficial effects. Moreover, a systemic approach is based on high viral loads and may enhance the risk for cancer especially in non-neuronal cells.
Box 1. An informed decision for the most promising candidate—the advantages of network biology.
Network biology describes the physical and/or functional interaction of a plethora of biological molecular entities. An important application is the network biology of proteins involved in signaling (57). Signaling proteins form nodes which are connected by links or edges. Those edges define the relationship between the nodes. Those can be functional or physical interactions of proteins, normally derived from databases such as the BioGRID, Intact or EMBL-STRING databases (58–60). Graphical analysis algorithms are able to arrange the nodes based on their connectivity. This leads to the formation of modules or clusters which often share a common biological function (57). Hubs are highly connected nodes located within modules—thus being critical master regulators for distinct biological processes. Inter-modular nodes may even be more important since they affect more than one module simultaneously. If applied on a disease, network biology provides a non-reductionist view on molecular processes such as altered signaling. The selection of hubs or inter-modular nodes allows an informed decision for a novel treatment target.
We performed a network analysis based on published reports about altered signaling in SMA. Therefore, we included SMN, JNK3 (MAPK3), p53 (TP53), PTEN, ERK (MAPK1), and ROCK1 as input proteins (red dots). We used the Functional Enrichment Analysis Tool (FunRich) (61) with the EMBL-STRING database for a network analysis (60). Highly connected interactors were added to the network (green dots). Interestingly, a number of them have been connected to SMA pathology before (black outlined green dots). However, the selection of the input proteins may be biased a priori. It is not always clear whether those pathways have been identified in hypothesis-free approaches. An unbiased high-throughput approach may circumvent this drawback.
Another possible target for a SMN-independent treatment is the c-Jun N-terminal kinase 3 (JNK3). JNK3 is a MAP-kinase which is specifically expressed in the central nervous system (CNS) where it becomes up-regulated after traumatic brain injury (73, 74). Within the CNS, it may be expressed in neurons, oligodendrocytes, and astrocytes (75–77). JNK inhibition in an Alzheimer's disease (AD) model partially restored synaptic dysfunctions (78) which are of particular interest with regard to the SMA pathology. As mentioned above, synaptic dysfunctions are an important hallmark of motoneuron degeneration in SMA. Interestingly, SMNΔ7 mice displayed an enhanced JNK3 activation in the spinal cord with an unknown cell type origin. However, enhanced JNK3 activity was measured in severely symptomatic post-natal day 12 mice indicating a reaction to a neurodegenerative trauma rather than being the cause of motoneuron degeneration (68, 69). Altered JNK phosphorylation levels could not be detected in SMA cellular and mouse models or human tissue (79). However, there might be effects in different segments of the spinal cord with the lumbar part showing highest susceptibility. For example, such a pattern has been observed for p-ERK in lumbar segments L3 and L5 (but not in thoracic or L1 segments) (63). Importantly, SMNΔ7 mice with a JNK3 knock-out lived significantly longer than control SMNΔ7 mice (68) while a pharmacological approach with a pan JNK inhibitor did not convincingly enhance their survival (69).
p53 is a major regulator of cell cycle, DNA repair and apoptosis in numerous cell types. In differentiated neurons, p53 may regulate neuronal regeneration vs. apoptosis which is promoted by p53 phosphorylation of N-terminal residues (80). Post mortem analysis of SMA patient spinal cords revealed a nuclear accumulation of p53 in motoneurons (81). This was corroborated in SMNΔ7 mice in which nuclear accumulation was accompanied by a specific phosphorylation at the N-terminus (70). Interestingly, the SMN protein directly interacts with p53 (82). However, this interaction has not been linked to the altered N-terminal p53 phosphorylation. Moreover, in vivo changes in p53 localization and phosphorylation were evaluated in symptomatic SMNΔ7 animals (70). Therefore, altered p53 homeostasis may be the result rather than the cause of motoneuron degeneration. Indeed, amino-terminal p53 phosphorylation is a cell-type specific signal for apoptosis (83) and may become activated due to the degeneration of motoneurons in later stages. In line with that, p53 inhibition rescued motoneuron numbers but not the motor functions and SMNΔ7 mice did not survived longer (70).
One of the first possible SMN-independent targets characterized was the RhoA kinase (ROCK) pathway. ROCK is an important regulator of neuronal actin dynamics which is critical for the function of motoneuron synapses (22). The level of ROCK activity was enhanced in the spinal cord of the intermediate Smn2B/− SMA-mouse model at pre-symptomatic time points (64) but at no time point in the severe Taiwanese mice neither in spinal cord nor muscle (our data, not shown). Consistently, Smn2B/− mice displayed elevated survival rates when treated with small molecule ROCK inhibitors (64, 65) while there were detrimental effects on severe Taiwanese mice (63). ROCK-inhibited Smn2B/− mice did not show elevated SMN levels compared to control Smn2B/− mice. However, SMN-irreversibility has not been checked for the enhanced ROCK activity and the SMN-independency of this effect is therefore not clear yet (64). The changes in ROCK activity have been mechanistically linked to a direct interaction of the SMN protein with the ROCK-target profilin2a: a lack of the SMN protein results in an enhanced binding of ROCK to profilin2a which subsequently mediates the pathological changes (25). Given this molecular model, a restoration of the SMN-levels would also restore dysregulated actin dynamics—this mechanism and the resulting treatment approach would not be SMN-independent. However, the cellular source of the enhanced ROCK activity has not been identified yet. Neurodegeneration often induces a chronic, detrimental neuroinflammation driven by an enhanced glial ROCK activity (84). Enhanced ROCK activity in intermediate Smn2B/− mice may thus reflect neuroinflammation while it is possible that severe Taiwanese SMA mice die before developing such a chronic condition. Chronic neuroinflammation is a process which—once induced by neurodegeneration—sustains itself by inducing further neurodegeneration. This process may not be SMN-irreversible thus being a candidate for an SMN-independent treatment approach.
ERK is another pathway which is up-regulated in SMN knock-down cells (66) and in the spinal cord of two different severe SMA mouse models (63, 67). The ERK pathway is a classical neurotrophic signaling pathway and a positive regulator of neuronal regeneration (85). However, dependent on the localization of activated ERK, it may also trigger neurodegeneration (63). Inhibition of ERK enhanced survival of severe SMA mice and enhanced SMN expression accompanied by neuroprotection of motoneurons within the spinal cord (67). However, we employed a randomized study-design avoiding a litter-wise treatment and found a significant reduction in survival of severe Taiwanese SMA-mice treated with an ERK inhibitor (63). Thus, in our hands, we could indeed detect an enhanced ERK activity. However, ROCK as well as ERK inhibition was detrimental for SMA mice (63). ROCK and ERK are generic kinases expressed in most cells and tissues. In combination with a systemic inhibitory approach, this may produce significant side effects in a chronic treatment regimen. To develop a specific treatment strategy it is indispensable to identify and target the affected cell type in which the altered signaling event localizes. Moreover, ROCK and ERK act in a regulatory network influencing SMA-like pathophysiology in a combined manner rather than acting alone (63). Although both inhibitory regimens were detrimental, a combination of a ROCK and an ERK inhibitor performed better than the ERK inhibitor alone. This was accompanied by a ROCK-mediated rescue of the ERK activity in the spinal cord and confirmed in vitro studies in which we showed a crosstalk between both pathways (62, 63). This is a proof-of-principle of the network character of signaling events in SMA (Box 1).
Outlook: A Set of Recommendations to Identify Novel Targets for Combinatorial SMA Treatment Strategies
Based on the previous comments, one can derive recommendations for the identification of novel signaling pathways as SMN-independent treatment targets:
(i) It is better to choose a SMA-specific alteration downstream of SMN-deficiency as a target rather than selecting an unspecific neuroprotective signaling pathway. It is more efficient to target SMA-specific pathological processes. Those translate into changed network modules.
(ii) The selection of hubs or inter-modular nodes is a promising strategy for the identification of potent treatment targets. Targeting hubs or inter-modular nodes maximizes the beneficial effects on the whole network by restoring the equilibrium (Box 1).
(iii) For a targeted approach excluding compensatory events or epiphenomena, a pre-symptomatic evaluation of the signaling is superior over symptomatic analyses.
(iv) The signaling event must be localized in a disease relevant tissue and cell type. Motoneurons in the spinal cord and brain stem are still the preferred target in SMA. The identification of the cell type is most relevant for the pre-clinical experimental paradigm, since it allows a specific rescue approach thereby reducing side effects.
(v) The target must be SMN-irreversible which has to be tested in an appropriate model in combination with a SMN-enhancing drug. For the latter, suboptimal dosing or intervention delays have to be considered.
(vi) Potency must be tested by a robust pathophysiological benefit in combination with SMN-enhancing drugs.
Author Contributions
NH, SK, and PC wrote the manuscript. All authors contributed to manuscript revision, read, and approved the submitted version.
Funding
We thank the Deutsche Muskelstiftung for financial support.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
References
1. Prior TW. Spinal muscular atrophy: newborn and carrier screening. Obstet Gynecol Clin North Am. (2010) 37:23–36. doi: 10.1016/j.ogc.2010.03.001
2. Sugarman EA, Nagan N, Zhu H, Akmaev VR, Zhou Z, Rohlfs EM, et al. Pan-ethnic carrier screening and prenatal diagnosis for spinal muscular atrophy: clinical laboratory analysis of >72,400 specimens. Eur J Hum Genet. (2012) 20:27–32. doi: 10.1038/ejhg.2011.134
3. D'amico A, Mercuri E, Tiziano FD, Bertini E. Spinal muscular atrophy. Orphanet J Rare Dis. (2011) 6:71. doi: 10.1186/1750-1172-6-71
4. Monani UR. Spinal muscular atrophy: a deficiency in a ubiquitous protein; a motor neuron-specific disease. Neuron. (2005) 48:885–96. doi: 10.1016/j.neuron.2005.12.001
5. Lefebvre S, Burglen L, Reboullet S, Clermont O, Burlet P, Viollet L, et al. Identification and characterization of a spinal muscular atrophy-determining gene. Cell. (1995) 80:155–65. doi: 10.1016/0092-8674(95)90460-3
6. Lorson CL, Hahnen E, Androphy EJ, Wirth B. A single nucleotide in the SMN gene regulates splicing and is responsible for spinal muscular atrophy. Proc Natl Acad Sci USA. (1999) 96:6307–11. doi: 10.1073/pnas.96.11.6307
7. Vitte J, Fassier C, Tiziano FD, Dalard C, Soave S, Roblot N, et al. Refined characterization of the expression and stability of the SMN gene products. Am J Pathol. (2007) 171:1269–80. doi: 10.2353/ajpath.2007.070399
8. Campbell L, Potter A, Ignatius J, Dubowitz V, Davies K. Genomic variation and gene conversion in spinal muscular atrophy: implications for disease process and clinical phenotype. Am J Hum Genet. (1997) 61:40–50. doi: 10.1086/513886
9. Munsat TL, Davies KE. International SMA consortium meeting. (26-28 June 1992, Bonn, Germany). Neuromuscul Disord. (1992) 2:423–8. doi: 10.1016/S0960-8966(06)80015-5
10. Finkel R, Bertini E, Muntoni F, Mercuri E, Group ESWS. 209th ENMC International Workshop: outcome measures and clinical trial readiness in spinal muscular Atrophy 7-9 November 2014, Heemskerk, The Netherlands. Neuromuscul Disord. (2015) 25:593–602. doi: 10.1016/j.nmd.2015.04.009
11. Wang CH, Finkel RS, Bertini ES, Schroth M, Simonds A, Wong B, et al. Consensus statement for standard of care in spinal muscular atrophy. J Child Neurol. (2007) 22:1027–49. doi: 10.1177/0883073807305788
12. Grotto S, Cuisset JM, Marret S, Drunat S, Faure P, Audebert-Bellanger S, et al. Type 0 spinal muscular atrophy: further delineation of prenatal and postnatal features in 16 patients. J Neuromuscul Dis. (2016) 3:487–95. doi: 10.3233/JND-160177
13. Finkel RS, Mcdermott MP, Kaufmann P, Darras BT, Chung WK, Sproule DM, et al. Observational study of spinal muscular atrophy type I and implications for clinical trials. Neurology. (2014) 83:810–7. doi: 10.1212/WNL.0000000000000741
14. Kaufmann P, Mcdermott MP, Darras BT, Finkel RS, Sproule DM, Kang PB, et al. Prospective cohort study of spinal muscular atrophy types 2 and 3. Neurology. (2012) 79:1889–97. doi: 10.1212/WNL.0b013e318271f7e4
15. Liu Q, Dreyfuss G. A novel nuclear structure containing the survival of motor neurons protein. EMBO J. (1996) 15:3555–65. doi: 10.1002/j.1460-2075.1996.tb00725.x
16. Bechade C, Rostaing P, Cisterni C, Kalisch R, La Bella V, Pettmann B, et al. Subcellular distribution of survival motor neuron (SMN) protein: possible involvement in nucleocytoplasmic and dendritic transport. Eur J Neurosci. (1999) 11:293–304. doi: 10.1046/j.1460-9568.1999.00428.x
17. Pagliardini S, Giavazzi A, Setola V, Lizier C, Di Luca M, Debiasi S, et al. Subcellular localization and axonal transport of the survival motor neuron (SMN) protein in the developing rat spinal cord. Hum Mol Genet. (2000) 9:47–56. doi: 10.1093/hmg/9.1.47
18. Fan L, Simard LR. Survival motor neuron (SMN) protein: role in neurite outgrowth and neuromuscular maturation during neuronal differentiation and development. Hum Mol Genet. (2002) 11:1605–14. doi: 10.1093/hmg/11.14.1605
19. Singh RN, Howell MD, Ottesen EW, Singh NN. Diverse role of survival motor neuron protein. Biochim Biophys Acta Gene Regul Mech. (2017) 1860:299–315. doi: 10.1016/j.bbagrm.2016.12.008
20. Pellizzoni L, Kataoka N, Charroux B, Dreyfuss G. A novel function for SMN, the spinal muscular atrophy disease gene product, in pre-mRNA splicing. Cell. (1998) 95:615–24. doi: 10.1016/S0092-8674(00)81632-3
21. Burghes AH, Beattie CE. Spinal muscular atrophy: why do low levels of survival motor neuron protein make motor neurons sick? Nat Rev Neurosci. (2009) 10:597–609. doi: 10.1038/nrn2670
22. Hensel N, Claus P. The actin cytoskeleton in SMA and ALS: how does it contribute to motoneuron degeneration? Neuroscientist. (2018) 24:54–72. doi: 10.1177/1073858417705059
23. Giesemann T, Rathke-Hartlieb S, Rothkegel M, Bartsch JW, Buchmeier S, Jockusch BM, et al. A role for polyproline motifs in the spinal muscular atrophy protein SMN. Profilins bind to and colocalize with smn in nuclear gems. J Biol Chem. (1999) 274:37908–14. doi: 10.1074/jbc.274.53.37908
24. Sharma A, Lambrechts A, Hao Le T, Le TT, Sewry CA, Ampe C, et al. A role for complexes of survival of motor neurons (SMN) protein with gemins and profilin in neurite-like cytoplasmic extensions of cultured nerve cells. Exp Cell Res. (2005) 309:185–97. doi: 10.1016/j.yexcr.2005.05.014
25. Nölle A, Zeug A, Van Bergeijk J, Tonges L, Gerhard R, Brinkmann H, et al. The spinal muscular atrophy disease protein SMN is linked to the Rho-kinase pathway via profilin. Hum Mol Genet. (2011) 20:4865–78. doi: 10.1093/hmg/ddr425
26. Van Bergeijk J, Rydel-Konecke K, Grothe C, Claus P. The spinal muscular atrophy gene product regulates neurite outgrowth: importance of the C terminus. FASEB J. (2007) 21:1492–502. doi: 10.1096/fj.06-7136com
27. Bowerman M, Anderson CL, Beauvais A, Boyl PP, Witke W, Kothary R. SMN, profilin IIa and plastin 3: a link between the deregulation of actin dynamics and SMA pathogenesis. Mol Cell Neurosci. (2009) 42:66–74. doi: 10.1016/j.mcn.2009.05.009
28. Simic G, Mladinov M, Seso Simic D, Jovanov Milosevic N, Islam A, Pajtak A, et al. Abnormal motoneuron migration, differentiation, and axon outgrowth in spinal muscular atrophy. Acta Neuropathol. (2008) 115:313–26. doi: 10.1007/s00401-007-0327-1
29. Harding BN, Kariya S, Monani UR, Chung WK, Benton M, Yum SW, et al. Spectrum of neuropathophysiology in spinal muscular atrophy type I. J Neuropathol Exp Neurol. (2015) 74:15–24. doi: 10.1097/NEN.0000000000000144
30. Moon LDF. Chromatolysis: do injured axons regenerate poorly when ribonucleases attack rough endoplasmic reticulum, ribosomes and RNA? Dev Neurobiol. (2018) 78:1011–24. doi: 10.1002/dneu.22625
31. Martinez-Hernandez R, Bernal S, Also-Rallo E, Alias L, Barcelo MJ, Hereu M, et al. Synaptic defects in type I spinal muscular atrophy in human development. J Pathol. (2013) 229:49–61. doi: 10.1002/path.4080
32. Mentis GZ, Blivis D, Liu W, Drobac E, Crowder ME, Kong L, et al. Early functional impairment of sensory-motor connectivity in a mouse model of spinal muscular atrophy. Neuron. (2011) 69:453–67. doi: 10.1016/j.neuron.2010.12.032
33. Kölbel H, Hauffa BP, Wudy SA, Bouikidis A, Della Marina A, Schara U. Hyperleptinemia in children with autosomal recessive spinal muscular atrophy type I-III. PLoS ONE. (2017) 12:e0173144. doi: 10.1371/journal.pone.0173144
34. Arnold AS, Gueye M, Guettier-Sigrist S, Courdier-Fruh I, Coupin G, Poindron P, et al. Reduced expression of nicotinic AChRs in myotubes from spinal muscular atrophy I patients. Lab Invest. (2004) 84:1271–8. doi: 10.1038/labinvest.3700163
35. Rudnik-Schoneborn S, Vogelgesang S, Armbrust S, Graul-Neumann L, Fusch C, Zerres K. Digital necroses and vascular thrombosis in severe spinal muscular atrophy. Muscle Nerve. (2010) 42:144–7. doi: 10.1002/mus.21654
36. Araujo A, Araujo M, Swoboda KJ. Vascular perfusion abnormalities in infants with spinal muscular atrophy. J Pediatr. (2009) 155:292–4. doi: 10.1016/j.jpeds.2009.01.071
37. Somers E, Lees RD, Hoban K, Sleigh JN, Zhou H, Muntoni F, et al. Vascular defects and spinal cord hypoxia in spinal muscular atrophy. Ann Neurol. (2016) 79:217–30. doi: 10.1002/ana.24549
38. Bowerman M, Swoboda KJ, Michalski JP, Wang GS, Reeks C, Beauvais A, et al. Glucose metabolism and pancreatic defects in spinal muscular atrophy. Ann Neurol. (2012) 72:256–68. doi: 10.1002/ana.23582
39. Deguise MO, Baranello G, Mastella C, Beauvais A, Michaud J, Leone A, et al. Abnormal fatty acid metabolism is a core component of spinal muscular atrophy. Ann Clin Transl Neurol. (2019) 6:1519–1532. doi: 10.1002/acn3.50855
40. Nash LA, Burns JK, Chardon JW, Kothary R, Parks RJ. Spinal muscular atrophy: more than a disease of motor neurons? Curr Mol Med. (2016) 16:779–92. doi: 10.2174/1566524016666161128113338
41. Tizzano EF, Finkel RS. Spinal muscular atrophy: a changing phenotype beyond the clinical trials. Neuromuscul Disord. (2017) 27:883–9. doi: 10.1016/j.nmd.2017.05.011
42. Martinez TL, Kong L, Wang X, Osborne MA, Crowder ME, Van Meerbeke JP, et al. Survival motor neuron protein in motor neurons determines synaptic integrity in spinal muscular atrophy. J Neurosci. (2012) 32:8703–15. doi: 10.1523/JNEUROSCI.0204-12.2012
43. Gavrilina TO, Mcgovern VL, Workman E, Crawford TO, Gogliotti RG, Didonato CJ, et al. Neuronal SMN expression corrects spinal muscular atrophy in severe SMA mice while muscle-specific SMN expression has no phenotypic effect. Hum Mol Genet. (2008) 17:1063–75. doi: 10.1093/hmg/ddm379
44. Rindt H, Feng Z, Mazzasette C, Glascock JJ, Valdivia D, Pyles N, et al. Astrocytes influence the severity of spinal muscular atrophy. Hum Mol Genet. (2015) 24:4094–102. doi: 10.1093/hmg/ddv148
45. Sleigh JN, Gillingwater TH, Talbot K. The contribution of mouse models to understanding the pathogenesis of spinal muscular atrophy. Dis Model Mech. (2011) 4:457–67. doi: 10.1242/dmm.007245
46. Finkel RS, Chiriboga CA, Vajsar J, Day JW, Montes J, De Vivo DC, et al. Treatment of infantile-onset spinal muscular atrophy with nusinersen: a phase 2, open-label, dose-escalation study. Lancet. (2016) 388:3017–26. doi: 10.1016/S0140-6736(16)31408-8
47. Hoy SM. Nusinersen: first global approval. Drugs. (2017) 77:473–9. doi: 10.1007/s40265-017-0711-7
48. Rigo F, Chun SJ, Norris DA, Hung G, Lee S, Matson J, et al. Pharmacology of a central nervous system delivered 2'-O-methoxyethyl-modified survival of motor neuron splicing oligonucleotide in mice and nonhuman primates. J Pharmacol Exp Ther. (2014) 350:46–55. doi: 10.1124/jpet.113.212407
49. Finkel RS, Mercuri E, Darras BT, Connolly AM, Kuntz NL, Kirschner J, et al. Nusinersen versus sham control in infantile-onset spinal muscular atrophy. N Engl J Med. (2017) 377:1723–32. doi: 10.1056/NEJMoa1702752
50. Luu KT, Norris DA, Gunawan R, Henry S, Geary R, Wang Y. Population pharmacokinetics of nusinersen in the cerebral spinal fluid and plasma of pediatric patients with spinal muscular atrophy following intrathecal administrations. J Clin Pharmacol. (2017) 57:1031–41. doi: 10.1002/jcph.884
51. Mendell JR, Al-Zaidy S, Shell R, Arnold WD, Rodino-Klapac LR, Prior TW, et al. Single-dose gene-replacement therapy for spinal muscular atrophy. N Engl J Med. (2017) 377:1713–22. doi: 10.1056/NEJMoa1706198
52. Mercuri E, Darras BT, Chiriboga CA, Day JW, Campbell C, Connolly AM, et al. Nusinersen versus sham control in later-onset spinal muscular atrophy. N Engl J Med. (2018) 378:625–35. doi: 10.1056/NEJMoa1710504
53. De Vivo DC, Bertini E, Swoboda KJ, Hwu WL, Crawford TO, Finkel RS, et al. Nusinersen initiated in infants during the presymptomatic stage of spinal muscular atrophy: interim efficacy and safety results from the Phase 2 NURTURE study. Neuromuscul Disord. (2019) 29:842–56. doi: 10.1016/j.nmd.2019.09.007
54. Hua Y, Sahashi K, Rigo F, Hung G, Horev G, Bennett CF, et al. Peripheral SMN restoration is essential for long-term rescue of a severe spinal muscular atrophy mouse model. Nature. (2011) 478:123–6. doi: 10.1038/nature10485
55. Long KK, O'shea KM, Khairallah RJ, Howell K, Paushkin S, Chen KS, et al. Specific inhibition of myostatin activation is beneficial in mouse models of SMA therapy. Hum Mol Genet. (2019) 28:1076–89. doi: 10.1093/hmg/ddy382
56. Faul F, Erdfelder E, Lang AG, Buchner A. G*Power 3: a flexible statistical power analysis program for the social, behavioral, and biomedical sciences. Behav Res Methods. (2007) 39:175–91. doi: 10.3758/BF03193146
57. Parikshak NN, Gandal MJ, Geschwind DH. Systems biology and gene networks in neurodevelopmental and neurodegenerative disorders. Nat Rev Genet. (2015) 16:441–58. doi: 10.1038/nrg3934
58. Stark C, Breitkreutz BJ, Chatr-Aryamontri A, Boucher L, Oughtred R, Livstone MS, et al. The BioGRID Interaction Database: 2011 update. Nucleic Acids Res. (2011) 39:D698–704. doi: 10.1093/nar/gkq1116
59. Aranda B, Achuthan P, Alam-Faruque Y, Armean I, Bridge A, Derow C, et al. The IntAct molecular interaction database in 2010. Nucleic Acids Res. (2010) 38:D525–D531. doi: 10.1093/nar/gkp878
60. Szklarczyk D, Gable AL, Lyon D, Junge A, Wyder S, Huerta-Cepas J, et al. STRING v11: protein-protein association networks with increased coverage, supporting functional discovery in genome-wide experimental datasets. Nucleic Acids Res. (2019) 47:D607–D613. doi: 10.1093/nar/gky1131
61. Pathan M, Keerthikumar S, Ang CS, Gangoda L, Quek CY, Williamson NA, et al. FunRich: an open access standalone functional enrichment and interaction network analysis tool. Proteomics. (2015) 15:2597–601. doi: 10.1002/pmic.201400515
62. Hensel N, Stockbrugger I, Rademacher S, Broughton N, Brinkmann H, Grothe C, et al. Bilateral crosstalk of rho- and extracellular-signal-regulated-kinase (ERK) pathways is confined to an unidirectional mode in spinal muscular atrophy (SMA). Cell Signal. (2014) 26:540–8. doi: 10.1016/j.cellsig.2013.11.027
63. Hensel N, Baskal S, Walter LM, Brinkmann H, Gernert M, Claus P. ERK and ROCK functionally interact in a signaling network that is compensationally upregulated in Spinal Muscular Atrophy. Neurobiol Dis. (2017) 108:352–61. doi: 10.1016/j.nbd.2017.09.005
64. Bowerman M, Beauvais A, Anderson CL, Kothary R. Rho-kinase inactivation prolongs survival of an intermediate SMA mouse model. Hum Mol Genet. (2010) 19:1468–78. doi: 10.1093/hmg/ddq021
65. Bowerman M, Murray LM, Boyer JG, Anderson CL, Kothary R. Fasudil improves survival and promotes skeletal muscle development in a mouse model of spinal muscular atrophy. BMC Med. (2012) 10:24. doi: 10.1186/1741-7015-10-24
66. Hensel N, Ratzka A, Brinkmann H, Klimaschewski L, Grothe C, Claus P. Analysis of the fibroblast growth factor system reveals alterations in a mouse model of spinal muscular atrophy. PLoS ONE. (2012) 7:e31202. doi: 10.1371/journal.pone.0031202
67. Branchu J, Biondi O, Chali F, Collin T, Leroy F, Mamchaoui K, et al. Shift from extracellular signal-regulated kinase to AKT/cAMP response element-binding protein pathway increases survival-motor-neuron expression in spinal-muscular-atrophy-like mice and patient cells. J Neurosci. (2013) 33:4280–94. doi: 10.1523/JNEUROSCI.2728-12.2013
68. Genabai NK, Ahmad S, Zhang Z, Jiang X, Gabaldon CA, Gangwani L. Genetic inhibition of JNK3 ameliorates spinal muscular atrophy. Hum Mol Genet. (2015) 24:6986–7004. doi: 10.1093/hmg/ddv401
69. Schellino R, Boido M, Borsello T, Vercelli A. Pharmacological c-Jun NH2-Terminal Kinase (JNK) pathway inhibition reduces severity of spinal muscular atrophy disease in mice. Front Mol Neurosci. (2018) 11:308. doi: 10.3389/fnmol.2018.00308
70. Simon CM, Dai Y, Van Alstyne M, Koutsioumpa C, Pagiazitis JG, Chalif JI, et al. Converging mechanisms of p53 activation drive motor neuron degeneration in spinal muscular atrophy. Cell Rep. (2017) 21:3767–80. doi: 10.1016/j.celrep.2017.12.003
71. Little D, Valori CF, Mutsaers CA, Bennett EJ, Wyles M, Sharrack B, et al. PTEN depletion decreases disease severity and modestly prolongs survival in a mouse model of spinal muscular atrophy. Mol Ther. (2015) 23:270–7. doi: 10.1038/mt.2014.209
72. Ning K, Pei L, Liao M, Liu B, Zhang Y, Jiang W, et al. Dual neuroprotective signaling mediated by downregulating two distinct phosphatase activities of PTEN. J Neurosci. (2004) 24:4052–60. doi: 10.1523/JNEUROSCI.5449-03.2004
73. Kuan CY, Yang DD, Samanta Roy DR, Davis RJ, Rakic P, Flavell RA. The Jnk1 and Jnk2 protein kinases are required for regional specific apoptosis during early brain development. Neuron. (1999) 22:667–76. doi: 10.1016/S0896-6273(00)80727-8
74. Long J, Cai L, Li J, Zhang L, Yang H, Wang T. JNK3 involvement in nerve cell apoptosis and neurofunctional recovery after traumatic brain injury. Neural Regen Res. (2013) 8:1491–9. doi: 10.3969/j.issn.1673-5374.2013.16.006
75. Wang Y, Luo W, Reiser G. Proteinase-activated receptor-1 and−2 induce the release of chemokine GRO/CINC-1 from rat astrocytes via differential activation of JNK isoforms, evoking multiple protective pathways in brain. Biochem J. (2007) 401:65–78. doi: 10.1042/BJ20060732
76. Li QM, Tep C, Yune TY, Zhou XZ, Uchida T, Lu KP, et al. Opposite regulation of oligodendrocyte apoptosis by JNK3 and Pin1 after spinal cord injury. J Neurosci. (2007) 27:8395–404. doi: 10.1523/JNEUROSCI.2478-07.2007
77. Gourmaud S, Paquet C, Dumurgier J, Pace C, Bouras C, Gray F, et al. Increased levels of cerebrospinal fluid JNK3 associated with amyloid pathology: links to cognitive decline. J Psychiatry Neurosci. (2015) 40:151–61. doi: 10.1503/jpn.140062
78. Sclip A, Tozzi A, Abaza A, Cardinetti D, Colombo I, Calabresi P, et al. c-Jun N-terminal kinase has a key role in Alzheimer disease synaptic dysfunction in vivo. Cell Death Dis. (2014) 5:e1019. doi: 10.1038/cddis.2013.559
79. Pilato CM, Park JH, Kong L, D'ydewalle C, Valdivia D, Chen KS, et al. Motor neuron loss in SMA is not associated with somal stress-activated JNK/c-Jun signaling. Hum Mol Genet. (2019) 28:3282–92. doi: 10.1093/hmg/ddz150
80. Tedeschi A, Di Giovanni S. The non-apoptotic role of p53 in neuronal biology: enlightening the dark side of the moon. EMBO Rep. (2009) 10:576–83. doi: 10.1038/embor.2009.89
81. Simic G, Seso-Simic D, Lucassen PJ, Islam A, Krsnik Z, Cviko A, et al. Ultrastructural analysis and TUNEL demonstrate motor neuron apoptosis in Werdnig-Hoffmann disease. J Neuropathol Exp Neurol. (2000) 59:398–407. doi: 10.1093/jnen/59.5.398
82. Young PJ, Day PM, Zhou J, Androphy EJ, Morris GE, Lorson CL. A direct interaction between the survival motor neuron protein and p53 and its relationship to spinal muscular atrophy. J Biol Chem. (2002) 277:2852–9. doi: 10.1074/jbc.M108769200
83. Chao C, Herr D, Chun J, Xu Y. Ser18 and 23 phosphorylation is required for p53-dependent apoptosis and tumor suppression. EMBO J. (2006) 25:2615–22. doi: 10.1038/sj.emboj.7601167
84. Hensel N, Rademacher S, Claus P. Chatting with the neighbors: crosstalk between Rho-kinase (ROCK) and other signaling pathways for treatment of neurological disorders. Front Neurosci. (2015) 9:198. doi: 10.3389/fnins.2015.00198
Keywords: spinal muscular atrophy, therapy, survival of motoneuron (SMN), network biology, systems biology, SMN-irreversibility, SMN-independency, neurodegeneration
Citation: Hensel N, Kubinski S and Claus P (2020) The Need for SMN-Independent Treatments of Spinal Muscular Atrophy (SMA) to Complement SMN-Enhancing Drugs. Front. Neurol. 11:45. doi: 10.3389/fneur.2020.00045
Received: 18 July 2019; Accepted: 13 January 2020;
Published: 03 February 2020.
Edited by:
Ulrike Schara, Abteilung Neuropädiatrie, Universitätsklinikum Essen, GermanyReviewed by:
Valeria Ada Sansone, Nemo Clinical Center, ItalyHeike Kölbel, Essen University Hospital, Germany
Laurent Servais, University of Oxford, United Kingdom
Copyright © 2020 Hensel, Kubinski and Claus. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Peter Claus, claus.peter@mh-hannover.de