Glycosaminoglycan Storage Disorders: A Review

Coutinho, Maria Francisca; Lacerda, Lúcia; Alves, Sandra

doi:https://doi.org/10.1155/2012/471325

Biochemistry Research International

On this page

Abstract Introduction Conclusion References Copyright Related Articles

Special Issue

Glycosaminoglycans Metabolism

View this Special Issue

Review Article | Open Access

Volume 2012 | Article ID 471325 | https://doi.org/10.1155/2012/471325

Glycosaminoglycan Storage Disorders: A Review

Maria Francisca Coutinho,¹Lúcia Lacerda,²and Sandra Alves¹

Academic Editor: Laura Alaniz

Received02 Jun 2011

Accepted09 Aug 2011

Published05 Oct 2011

Abstract

Impaired degradation of glycosaminoglycans (GAGs) with consequent intralysosomal accumulation of undegraded products causes a group of lysosomal storage disorders known as mucopolysaccharidoses (MPSs). Characteristically, MPSs are recognized by increased excretion in urine of partially degraded GAGs which ultimately result in progressive cell, tissue, and organ dysfunction. There are eleven different enzymes involved in the stepwise degradation of GAGs. Deficiencies in each of those enzymes result in seven different MPSs, all sharing a series of clinical features, though in variable degrees. Usually MPS are characterized by a chronic and progressive course, with different degrees of severity. Typical symptoms include organomegaly, dysostosis multiplex, and coarse facies. Central nervous system, hearing, vision, and cardiovascular function may also be affected. Here, we provide an overview of the molecular basis, enzymatic defects, clinical manifestations, and diagnosis of each MPS, focusing also on the available animal models and describing potential perspectives of therapy for each one.

1. Introduction

The mucopolysaccharidoses (MPSs) are a group of lysosomal storage disorders caused by deficiency of enzymes catalyzing the stepwise degradation of glycosaminoglycans (GAGs) and characterized by intralysosomal accumulation and increased excretion in urine of partially degraded GAGs, which ultimately results in cell, tissue, and organ dysfunction [1].

Glycosaminoglycans (previously called mucopolysaccharides), with the exception of hyaluronic acid, are the degradation products of proteoglycans that exist in the extracellular matrix and are proteolytic cleaved, giving origin to GAGs, which enter the lysosome for intracellular digestion. There are four different pathways of lysosomal degradation of GAGs, depending on the molecule to be degraded: dermatan sulfate, heparan sulfate, keratan sulfate, and chondroitin sulfate. The stepwise degradation of glycosaminoglycans requires 10 different enzymes: four glycosidases, five sulfatases, and one nonhydrolytic transferase, whose structure, biosynthesis, processing, and cDNA sequence have already been extensively documented. Deficiencies of each one of these enzymes have already been reported and result in seven different MPSs, all of them sharing a series of clinical features, even though in variable degrees (summarized in Table 1) [1, 2].

Usually, MPSs are characterized by a chronic and progressive course, with different velocities of progression depending on the severity of each one. The typical symptoms include organomegaly, dysostosis multiplex, and a characteristic abnormal facies. Hearing, vision, and cardiovascular function may also be affected. Additionally, joint mobility may also be compromised. The majority of symptoms may be explained by abnormal accumulation of undegraded substrates within the lysosomes. In fact, the continued presentation of GAGs to cell for degradation results in storage, which gives rise to an enlargement of lysosomes. As substrates accumulate, the lysosomes swell and occupy more and more of the cytoplasm. As a consequence of this increased number and size of lysosomes, other cellular organelles may be obscured, and the nuclear outline may be deformed. As the process continues, the enlarged cells lead to organomegally. Abnormalities observed in heart cells and function may also be explained by GAGs accumulation. The increase of storage material within the cells of the heart valves causes an alteration of the cell’s outline, changing them from fusiform to round. As a consequence, the valve leaflet and cordae tendinea become thickener and interfere with normal cardiac function, producing valvular stenosis. At corneal level, also, storage of undegraded GAGs results in reflection and refraction of light, leading to the cloudiness which is so typical of these pathologies. Also at the CNS level, swollen neurons and lysosomes may produce lesions that include the development of meganeurites and neurite sprouting (reviewed in [3, 4]).

Traditionally, MPSs are recognized through analysis of urinary GAGs. Several methods have been devised, to precise qualitative identification and quantitative measurements. These analyses of urinary GAGs allow discrimination between broad classes of MPSs but cannot distinguish subgroups. Definitive diagnosis is usually accessed through enzymatic assays of the defective enzyme in cultured fibroblasts, leukocytes, and serum or plasma (reviewed in [1]). During the last decade; however, dried blood spot technology was also introduced for enzymatic assays, allowing cheaper, easier, feasible diagnosis and opening the possibility for large population screenings (see Section 11 for more details).

In general, MPSs are transmitted in an autosomal recessive fashion, except for MPS II, which is X-linked.

This paper provides an overview of the molecular basis, enzymatic defects, clinical manifestations, and diagnosis of each glycosaminoglycan storage disease, focusing also on the respective animal models and describing potential perspectives of therapy which are being tested as well as the ones which are already available (summarized in Table 2).

2. Mucopolysaccharidosis I

Mucopolysaccharidosis I is caused by a deficiency of α-L-iduronidase (IDUA; EC 3.2.1.76) and can result in a wide range of phenotypic involvement with three major recognized clinical entities: Hurler (MPS IH; MIM#607014), Hurler-Scheie (MPS IH/S; MIM#607015), and Scheie (MPS IS) syndromes. Hurler and Scheie syndromes represent phenotypes at the severe and mild ends of the MPS I clinical spectrum; respectively, and the Hurler-Scheie syndrome is intermediate in phenotypic expression [20]. It is important to stress that, although MPS I may be subdivided into these three clinically diverse entities, the underlying enzymatic defect is common to all of them, being all caused by mutation in the gene encoding α-L-iduronidase (IDUA).

Functionally, α-L-iduronidase is essential to the correct metabolism of both dermatan sulfate and of heparan sulfate, hydrolyzing the terminal α-L-iduronic acid residues of the above-referred glycosaminoglycans [1].

In 1992, Scott and colleagues [21] were able to clone and purify the gene that encodes this enzyme, IDUA, demonstrating that it spans approximately 19 kb and contains 14 exons. The first 2 exons are separated by an intron of 566 bp, a large intron of approximately 13 kb follows, and the last 12 exons are clustered within 4.5 kb. Previously, this gene was mapped to 4p16.3, through unequivocal in situ hybridization and southern blot analysis of mouse-human cell hybrids [22].

There are, presently, several animal models known for MPS I.

In 1979, Haskins and colleagues [5] described α-L-iduronidase deficiency in a cat, and, few years later, Shull et al. [6] and Spellacy et al. [23] reported a similar deficiency in the dog. Subsequent studies lead to cloning and characterization of the canine IDUA gene as well as the mutation causing the observed phenotype [24, 25] and proved it to be a good model for study of human MPS I. So, in 1994, Shull and collaborators [26] published the first results of enzyme replacement therapy in the canine model. Through intravenous administration of recombinant human α-L-iduronidase, these authors managed to obtain a remarkable resolution of lysosomal storage in both hepatocytes and Kupffer’s cells. In the same year, Grosson et al. [27] mapped the homologous IDUA locus in the mouse to chromosome 5. That knowledge was later used to create a knock-out mouse presenting the characteristic MPS I features [7, 28].

Currently, both hematopoietic stem cell transplantation (HSCT) and enzyme replacement therapy (ERT) using laronidase (recombinant human α-L-iduronidase, Aldurazyme) are available for MPS I. HSCT is the recommended treatment for patients with severe MPS I, before 2 years of age [29–32]. ERT is recommended for the other cases, and it has been shown to be effective in ameliorating some of the clinical manifestations of MPS disease. Among positive effects are decreased hepatosplenomegaly, improved respiratory and myocardial function and physical capacity [33–35] as well as improvement in active movement followed by enhanced self-care [36]. Recently, several reports have been published trying to evaluate long-term effect of ERT on the natural history of treated patients. From those studies, several conclusions have been reached. Concerning treated patients’ growth pattern, it became clear that children with MPS I grow considerably slower than healthy individuals, and differences between healthy and affected children increase with age [37]. Other relevant evidences show that early treatment of attenuated MPS I may significantly delay or prevent the onset of the major clinical signs, substantially modifying the natural history of the disease [38]. Additional investigation is needed to clarify the mechanisms by which improvements are achieved in laronidase-treated patients. Such knowledge may support the development of ERT directly targeting the brain.

2.1. Hurler’s Syndrome (MPS IH)

Hurler’s syndrome is the most severe form of MPS I and has been, over the last decades, the prototype description of MPS. Nevertheless, this may be misleading, since not all MPSs share the same features, and this pathology in particular is not representative of all of them, but only of the most severe end of a broad clinical spectrum (reviewed in [1]). Like all other MPSs, the clinical course of this disease is progressive, with multiple organ and tissue involvement. Hallmark clinical features of Hurler syndrome include coarse facies, corneal clouding, mental retardation, hernias, dysostosis multiplex, and hepatosplenomegaly. Children with Hurler’s syndrome appear normal at birth and develop the characteristic appearance over the first years of life [39]. Length is often normal until about 2 years of age when growth stops; by age of 3 years, height is under the third percentile [40]. Cardiac disease and respiratory complications are common. Acute cardiomyopathy associated with endocardial fibroelastosis has been a presenting condition in some infants with MPS I less than 1 year of age [41]. Upper and lower respiratory tract infections are also frequent [42]. Developmental delay is often apparent by 12 to 24 months of age, with a maximum functional age of 2 to 4 years followed by progressive deterioration. Most children develop limited language as a consequence of developmental delay, chronic hearing loss, and enlarged tongue [1]. Dermal melanocytosis may also be found in Hurler patients [43], as well as in patients suffering from other LSDs, such as GM1 gangliosidosis. Nevertheless, Hurler’s syndrome is the most common lysosomal storage disease associated with dermal melanocytosis, as revealed by a literature analysis.

2.2. Hurler-Scheie’s Syndrome (MPS IH/S)

MPS IH/S corresponds to a clinical phenotype which is intermediate between the Hurler and the Scheie syndromes. It is characterized by progressive somatic involvement with dysostosis multiplex but little or no mental retardation. First symptoms usually occur between 3 and 8 years. Characteristic features of Hurler’s syndrome, such as corneal clouding, joint stiffness, deafness, and valvular heart disease, can also appear in MPS IH/S patients. Nevertheless, the onset of these symptoms occurs much later than that in the severe MPS I type, beginning in the midteens and leading to significant impairment and loss of function. Other clinical features, such as micrognathism, pachymeningitis cervicalis, and compression of the cervical cord due to GAG accumulation in the dura, may also occur. Cardiac and respiratory complications may explain the high clinical mortality (reviewed in [1]).

2.3. Scheie’s Syndrome (MPS IS)

Scheie’s syndrome was earlier thought to be a separate entity designated MPS V, instead of a phenotypical subtype of MPS I [44]. This pathology is characterized by a mild phenotype in which dysostosis multiplex can be present. Joint involvement is marked in the hand with a claw-hand deformity. Patients also have genu valgum, stiff, painful feet, and pes cavus [1]. Cardiac and respiratory complications are much milder than in the Hurler syndrome, with aortic and mitral valvular disease being a common feature [45]. At a respiratory level, Perks et al. [46] have reported two brothers with Scheie’s syndrome suffering from sleep apnea, but no other complications are known. Intelligence is normal [1]. Pachymeningitis cervicalis (compression of the cervical cord secondary to glycosaminoglycan accumulation in the dura) may also occur.

3. Mucopolysaccharidosis II (Hunter’s Syndrome)

Mucopolysaccharidosis II is the sole MPS transmitted in an X-linked manner and is caused by deficiency of the lysosomal enzyme iduronate sulfatase, which is crucial to the correct degradation of heparan and dermatan sulfate, by cleaving their O-linked sulfate. As a result, there is a progressive accumulation of glycosaminoglycans in nearly all cell types, tissues, and organs. Patients with MPS II excrete excessive amounts of dermatan sulfate and heparan sulfate in the urine [20, 47]. Hunter syndrome is caused by mutation in the gene encoding iduronate-2-sulfatase (IDS).

Although the disease is known since the early 1970s, being the first MPS to be defined clinically in humans, it was not until the 1990s that the IDS was cloned. In 1991, Wilson et al. [48] localized the gene to Xq28. Two years later, Flomen and coworkers [49] described the gene’s structure as containing 9 exons and characterized the intron sequences surrounding them. In the same year, Wilson et al. [50] reported the complete sequence of the IDS gene, which spans approximately 24 kb. The potential promoter for IDS lacks a TATA box but contains GC box consensus sequences, which are consistent with its role as a housekeeping gene.

Curiously, a second IDS gene (IDS2) was identified by Bondeson et al. [51]. It is a pseudogene and is located within 90 kb telomeric region of the IDS gene and involved in a recombination event with the primary IDS gene in about 13% of patients with the Hunter syndrome.

Traditionally, the Hunter syndrome comprises 2 recognized clinical entities, according to the severity of symptoms: mild and severe. Although largely used, this nomenclature does have its difficulties, since the mild and severe forms represent the two ends of a wide and continuous spectrum of clinical severity. Also, in terms of iduronate deficiency, these forms cannot be distinguished since the enzyme’s activity is equally deficient in both (reviewed in [1]). They are, though, separated almost exclusively on clinical grounds, although nowadays mutation analysis may help distinguish them.

This classification of MPS goes back to 1972, when McKusick distinguished between the severe form (which he called MPS IIA), with progressive mental retardation and physical disability and death before age 15 years in most cases, and the mild form (called MPS IIB) compatible with survival to adulthood and in which intellect is impaired minimally, if at all. He also pointed out the lack of corneal clouding in the X-linked form of MPS as opposed to the autosomal forms.

Presently, this classification has become obsolete since, in 2008, Wraith et al. [47] stated that MPS II should be regarded as a continuum between the two extremes (severe and attenuated). They noted that, although the clinical course for the more severely affected patients is relatively predictable, there is considerable variability in the clinical phenotype and progression of the more attenuated form of the disease and, so, it would not be correct to consider the milder form as a separate entity but, instead, look at Hunter’s disease as a phenotypical continuum, with several possible degrees of severity.

In 1998, Wilkerson et al. [8] described Hunter’s syndrome in a Labrador retriever, with the typical clinical features observed in humans: coarse facies, macrodactyly, corneal dystrophy, progressive CNS deterioration, and positive biochemical diagnosis for MPS through urine analysis.

After the successful results obtained in improving certain disease manifestations in patients with MPS I, including visceral manifestations and attenuation of neurologic disease progression [29, 52], hematopoietic stem cells transplantation (HSCT) has also been performed in several patients with MPS II. Unfortunately, although the transplantation of hematopoietic stem cells provides some enzymatic reconstruction in many target tissues with decreased excretion of GAGs in urine, decreased liver and spleen volumes, diminished facial coarsening, and improved respiratory function and joint mobility [53, 54], the results at neurological level were disappointing (reviewed in [55]). The additional risk of morbidity and mortality associated to this procedure led investigators to focus their attention in ERT for this pathology, with much better results, as discussed below.

A knock-out mouse model for MPS II was developed by replacing exon 4 and a portion of exon 5 of IDS with the neomycin-resistance gene [9, 56]. Affected mice exhibit a phenotype with notorious similarities to human disease, both at the biochemical and the clinical levels [9]. Several studies with this knock-out mouse model were done to assess the effect of ERT [56] as well as dose and various dosing regimens of idursulfase in urine and tissue GAG levels [57]. The results of these studies were quite promising, with a marked decrease in urinary GAGs as well as decreased GAG accumulation in several tissues [56] verified for several idursulfase doses and several dosing frequencies [57]. These studies have been used to support the first clinical trial of recombinant IDS in Hunter’s syndrome patients. At the moment, both phase I/II [58] and phase II/III [59] clinical studies have proven not only the efficacy but also the safety of idursulfase replacement therapy. Consequently, ERT with recombinant human iduronate sulfatase (Elaprase, idursulfase, Shire Human Genetic Therapies Inc.) was approved in the US (July, 2006) and the European Union (January, 2007) for the treatment and the management of MPS II. The recommended dose is 0.5 mg/kg administered once weekly as an intravenous infusion (reviewed in [55]). As time goes by, additional evidence on the efficacy of ERT for MPS II patients is being published, as long-term treatments are successful. This is the case of a recently published report on the improvements observed in a 7 years and 10 months old child who began a 36 months’ treatment with Elaprase at 4 years and 10 months. At the end of the treatment, the child presented normal excretion of GAGs in urine, normal-sized liver and spleen, and significant bone remodeling. Cardiac and neurological development, however, still progressively deteriorated [60]. This year, protective effects of ERT in MPS II patients were also reported for DNA damaging in leukocytes [61] and oxidative stress [62].

4. Mucopolysaccharidosis III (Sanfilippo’s Syndrome)

The Sanfilippo syndrome, or mucopolysaccharidosis III, is caused by impaired degradation of heparan sulfate [1] and includes 4 subtypes, each due to the deficiency of a different enzyme: heparan N-sulfatase (type A; MIM no. 252900), α-N-acetylglucosaminidase (type B; MIM no. 252920), acetyl CoA: α-glucosaminide acetyltransferase (type C; MIM no. 252930), and N-acetylglucosamine-6-sulfatase (type D; MIM#252940). At a clinical level, the four subtypes are quite similar, with a characteristic severe central nervous system degeneration associated with mild somatic disease. Onset of clinical features usually occurs between 2 and 6 years, severe neurologic degeneration occurs in most patients between 6 and 10 years of age, and death occurs typically during the second or third decade of life. Type A has been reported to be the most severe, with earlier onset and rapid progression of symptoms and shorter survival [63].

4.1. Mucopolysaccharidosis IIIA (Sanfilippo A)

General MPS IIIA clinical features include severe mental retardation with relatively mild somatic features (moderately severe claw hand and visceromegaly, little or no corneal clouding, little or no vertebral change). Usually, this pathology is characterized by marked overactivity, destructive tendencies, and other behavioral aberrations.

MPS IIIA phenotype is caused by mutations in the gene encoding N-sulfoglucosamine sulfohydrolase, also named heparan sulfate sulfatase (SGSH; 605270). This enzyme is specific for sulfate groups linked to the amino group of glucosamine.

In 1995, the gene encoding N-sulfoglucosamine sulfohydrolase, SGSH, was isolated, sequenced, and cloned [64]. Later, it was shown to contain 8 exons spanning approximately 11 kb [65].

There are two animal models known for MPS IIIA. The first to be discovered was the canine model when Fischer et al. [10] identified sulfaminidase deficiency in two adult wire-haired dachshund littermates. Subsequently, Aronovich et al. [66] determined the normal sequence of the canine heparan sulfate sulfatase gene and cDNA, through PCR-based approaches. Another model was described in 2001, when Bhattacharyya and collaborators [11] found a spontaneous mouse mutant of MPS IIIA resulting from a missense mutation (D31N) in the murine sulfatase gene. Affected mice die at about 10 months of age, exhibiting notorious visceromegaly, distended lysosomes and heparan sulfate accumulation in urine. Hemsley and Hopwood [67] found that these mice had severe brain involvement, with impaired open field locomotor activity and behavioral changes, suggesting axonal degeneration. Later, Settembre et al. [68] observed increased autophagosomes resulting from autophagosome-lysosome function in these mice. Similar findings were observed in another mouse model of another lysosomal storage disorder (multiple sulfatase deficiency; MSD; MIM no. 272200), reinforcing the recent idea that these diseases are disorders of autophagy, which may be a common mechanism for neurodegenerative lysosomal storage disorders.

MPS IIIA mice were recently tested for substrate deprivation therapy with both genistein and rhodamine B, two chemicals that inhibit GAG synthesis ([4, 69], reviewed in [70]). Encouraging results were obtained with both compounds, and this therapeutic approach started to be considered for several MPSs (see Section 11 for more details). Other interesting results were also obtained when siRNAs were used to reduce GAG synthesis in MPS IIIA mice. Last year, this approach was tested by Dziedzic et al. [71], who managed to reduce mRNA levels of four genes, XYLT1, XYLT2, GALTI, and GALTII, whose products are involved in GAG synthesis. This decrease of levels of transcripts corresponded to a decrease in levels of proteins encoded by them. Moreover, efficiency of GAG production in these fibroblasts was considerably reduced after treatment of the cells with siRNA. Either way, substrate deprivation therapy seems to be a promising approach for Sanfilippo’s syndrome type A.

Gene therapy approaches are also being tested in MPS IIIA mice. Recently, promising results have been reported by Fraldi et al. [72], who performed experiments with intracerebral adeno-associated-virus- (AAV-) mediated delivery of SGSH gene, together with SMUF1 gene, which exhibits an enhancing effect on sulfatase activity when coexpressed with sulfatases. They observed a visible reduction in lysosomal storage and inflammatory markers in transduced brain regions, together with an improvement in both motor and cognitive functions.

4.2. Mucopolysaccharidosis IIIB (Sanfilippo B)

With a phenotype quite similar to MPS IIIA, the Sanfilippo syndrome B is characterized by deficiencies of α-N-acetylglucosaminidase, caused by mutations in the NAGLU gene that encodes this enzyme. α-N-Acetylglucosaminidase is required for the removal of the N-acetylglucosamine residues that exist in heparan sulfate or are generated during lysosomal degradation of this polymer by the action of heparan acetyl-CoA: α-glucosaminide N-acetyltransferase (reviewed in [1]).

The NAGLU gene was cloned in 1995 by Zhao and colleagues [73]. The deduced 743-amino acid protein has a 20- to 23-residue leader sequence, consistent with a signal peptide, and 6 potential N-glycosylation sites. It contains 6 exons and spans 8.3 kb on chromosome 17q21 [74].

Similarly to the above-referred MPS III syndrome, there is also a natural occurring mutant for Sanfilippo B. It was described by Ellinwood and coworkers, in 2003, in Schipperke’s dogs [12].

During the last decade, Li et al. [75] created a laboratorial murine MPS IIIB was also constructed trough targeted disruption of the NAGLU gene [76]. With a phenotype quite similar to that of patients with MPS IIIB, this model began immediately to be used for therapeutic approaches as well as for pathogenesis studies. The first studies were done to evaluate the potential of ERT for this pathology [76]. The results, however, were quite disappointing since the recombinant NAGLU produced in Chinese hamster ovary (CHO) cells was not efficiently captured by MPS IIIB cells, either in vitro [77, 78] or in vivo [76]. This difficulty has turned the search for a treatment for MPS IIIB even more challenging. Presently, several therapies are under evaluation for this disease, including cell-mediated therapy, enzyme enhancement therapy, substrate deprivation therapy, and viral gene therapy (reviewed in [79]).

Promising results are being achieved through gene therapy approaches in MPS IIIB mice, namely, through direct microinjection into the brain of adeno-associated virus (AAV) vectors coding for NAGLU [80–82] and intravenous injections and intracranial gene delivery of lentiviral (LV) vector of NAGLU [83–85].

4.3. Mucopolysaccharidosis IIIC (Sanfilippo C)

Sanfilippo syndrome C is, in general, characterized by the same clinical features described to MPS IIIA. Nevertheless, the enzyme deficiency in this pathology is different from the one causing the latter. Type C disease is caused by mutations in the gene encoding heparan acetyl-CoA: α-glucosaminide N-acetyltransferase (HGSNAT; 610453). This is the only known lysosomal enzyme that is not a hydrolase. It catalyzes the acetylation of the glucosamine amino groups that have become exposed by the action of heparan-N-sulfatase (reviewed in [1]).

The HGSNAT gene was cloned in parallel by two different groups, during the last decade: Fan et al. [86] and Hřebíček et al. [87]. The molecular defects underlying MPS IIIC remained unknown for almost three decades due to the low tissue content and the instability of HGSNAT [88].

To date, 54 HGSNAT sequence variants have been identified including 13 splice-site mutations, 11 insertions and deletions with consequent frameshifts and premature termination of translation, 8 nonsense, and 18 missense (reviewed in [89]).

Recently, two independent studies from Feldhammer et al. [88] and Fedele and Hopwood [90] have performed exhaustive functional analysis of the majority of the missense mutations already reported for the HGSNAT gene. Attention was focused in this particular type of mutations since there are several MPS IIIC patients carrying only missense mutations, either homozygous or heterozygous, who present an unexpected severe phenotype. In fact, although splicing and frameshift mutations are usually associated to that type of phenotype, since they give rise to premature termination codons and trigger nonsense-mediated mRNA decay (NMD); missense mutations are traditionally associated to milder disease. Nevertheless, this typical/general pattern is not observed for MPS IIIC. That is why these alterations were specifically cloned, expressed, and analyzed for their folding, targeting, and enzymatic activities. As a result, Fedele and Hopwood [90] have observed that the expression levels and enzymatic activity of most mutants were extremely low or even negligible. Feldhammer and colleagues [88], on the other hand, have observed that those mutations cause a misfolding of the enzyme, which is not correctly glycosylated. As a consequence, HGSNAT is not targeted to the lysosome but, instead, stays in the endoplasmic reticulum (ER). Thus, enzyme folding defects due to missense mutations, together with NMD seem to be the major molecular mechanisms underlying MPS IIIC. This makes MPS IIIC a good candidate for enzyme enhancement therapy, where active site-specific inhibitors are used as pharmacological chaperones to modify the conformation of the mutant lysosomal enzymes usually retained and degraded in the ER, in order to increase the level of the residual activity to a point which is sufficient to reverse the clinical phenotypes [88]. Together with inhibitors of heparan sulphate synthesis, pharmacological chaperones are currently being tested to reduce storage of this polymer in the CNS to levels sufficient to stop neuronal death and reverse inflammation.

4.4. Mucopolysaccharidosis IIID (Sanfilippo D)

Like the previous MPS III subtypes, Sanfilippo’s syndrome D presents a phenotype similar to MPS IIIA, with a singular enzyme deficiency underlying it: mutation in the gene encoding N-acetylglucosamine-6-sulfatase (GNS; 607664). The enzyme was originally described as specific for the 6-sulphated N-acetylglucosamine residues of heparan sulphate. However, the early data have been reinterpreted, and given that this sulfatase is in fact able to desulphate the 6-sulphated N-acetylglucosamine present in α- or in β-linkage or even as a free monosaccharide (reviewed in [1]).

N-Acetylglucosamine-6-sulfatase (EC 3.1.6.14) was purified and characterized by Freeman et al. [91], who identified 4 different forms of the enzyme in liver. Its catalytic properties were studied by Freeman and Hopwood [92]. Afterwards, Robertson et al. [93] assigned the glucosamine-6-sulfatase gene, which they symbolized G6S, to chromosome 12q14 by in situ hybridization of a tritium-labeled G6S cDNA probe. The localization was confirmed by using the cDNA clone in analyses of DNA from human/mouse hybrid cell lines. More recently, that information was completed by the work of Mok et al. [94], who amplified and sequenced the promoter and 14 exons of the GNS gene from a patient with MPS IIID. By analyzing that patient, it was also possible to identify a homozygous nonsense mutation in exon 9, predicted to result in premature termination at codon 355, as well as two common synonymous coding SNPs. At the same time, another group identified a 1-bp deletion in the GNS gene in another affected individual [95].

A naturally occurring large animal model was described by Thompson et al. [13], who reported type D Sanfilippo’s syndrome in a Nubian goat. Later, caprine MPS IIID was used to evaluate the efficacy of ERT in this pathology. Recombinant caprine N-acetylglucosamine-6-sulfatase was administered intravenously to one MPS IIID goat at 2, 3, and 4 weeks of age. As a result, a marked reduction of lysosomal storage vacuoles was observed in hepatic cells, but no amelioration was noticed concerning the CNS lesions. No residual enzyme activity was observed either in brain or liver. Taking this preliminary results into account, it was considered that other treatment regimens will be necessary for MPS IIID [96].

5. Mucopolysaccharidosis IV

Mucopolysaccharidosis IV, or Morquio’s syndrome, is caused by impaired degradation of keratan sulphate. Presently, there are two known enzyme deficiencies causing 2 different subtypes of Morquio’s syndrome: deficiency in N-acetylglucosamine-6-sulfatase (causing Morquio’s disease type A; MIM no. 253000) and deficiency in β-galactosidase (causing Morquio’s disease type B; MIM no. 253010). Both MPS IV subtypes present a wide spectrum of clinical manifestations, but there are some characteristic common features: short trunk dwarfism, fine corneal deposits, spondyloepiphyseal dysplasia. Actually, the predominant clinical features of Morquio’s syndrome are the ones related to the skeleton. Most of the times, this severe somatic disease is accompanied by a normal intelligence [1]. Patients with the severe phenotype do not normally survive past the second or third decade of life [97].

5.1. Morquio’s Syndrome Type A

Morquio’s syndrome A is caused by mutations in the gene encoding galactosamine-6-sulphate sulfatase (GALNS), which plays a crucial role on the degradation of both keratan sulphate and chondroitin sulphate.

The gene coding for human galactosamine-6-sulphate sulfatase (GALNS), was mapped to chromosome 16q24.3 trough fluorescence in situ hybridization assays [98]. Its structure was described at the same time by independent groups as comprising 14 exons and spanning approximately 40–50 kb [99, 100]. Curiously, the GALNS gene contains an Alu repeat in intron 5 and a VNTR-like sequence in intron 6 [100].

No natural occurring model is known for either type A or type B Morquio’s syndrome. Nevertheless, a laboratorial murine model for type A syndrome was created from an induced disruption in exon 2 of the GALNS gene. Mutants presented no detectable enzyme activity and showed increased GAG levels in urine. GAGs accumulation was also detected in several tissues including liver, kidney, spleen, heart, brain, and bone marrow [14]. These mice were later tested for enzyme replacement therapy and, after a 12-week long treatment with native GALNS or SUMF1-modified GALNS, showed manifest clinical improvement, demonstrated by a marked reduction of storage material in visceral organs, bone marrow, heart valves, ligaments, and connective tissue. The clearance of stored material in brain was dose dependent, and the keratan sulphate blood levels were reduced to normal [101].

Presently, there is no effective therapy for MPS IVA and care has been palliative, as in the majority of LSDs. Enzyme replacement therapy (ERT) and hematopoietic stem cells therapy (HSCT) have been considered as potential therapeutic approaches for MPS IVA (reviewed in [102]), ERT being, though, the most attractive candidate, since affected patients lack CNS involvement.

Recently, Rodríguez et al. [103] have produced a recombinant GALNS enzyme in Escherichia coli BL21. To produce sufficient amounts of purified GALNS enzyme, high level expression of GALNS in Chinese hamster ovary (CHO) cells has been established as a source of selectively secreted human recombinant enzyme. This recombinant enzyme has already been tested in the murine knock-out model, with consequent clearance of tissue and blood keratan sulphate [101]. These results provided important preclinical data for the design of GALNS ERT trials, which are now in course.

5.2. Morquio’s Syndrome Type B

Although presenting overlapping clinical features, Morquio’s syndrome B is genetically distinct from Morquio’s syndrome A, being caused by impairments in another enzyme involved in the stepwise degradation of keratan sulphate: β-galactosidase, which is coded by the GLB1 gene. Beta galactosidase hydrolases terminal β-linked galactose residues found in GM1 ganglioside, glycoproteins, and oligosaccharides, as well as in keratan sulphate (reviewed in [1]).

The GLB1 gene spans 62.5 kb and contains 16 exons [104, 105] and maps to chromosome 3p21.33 [106]. The deduced 677-residue protein has a calculated molecular mass of 75 kD and contains a putative 23-residue signal sequence and 7 potential asparagine-linked glycosylation sites. It may be interesting to refer that the GLB1 gene gives rise to 2 alternatively spliced mRNAs: a major 2.5-kb transcript that encodes the classic lysosomal form of the enzyme of 677 amino acids, and a minor 2.0-kb transcript that encodes a β-galactosidase-related protein (elastin-binding protein, EBP) of 546 amino acids with no enzymatic activity and a different subcellular localization. Exons 3, 4, and 6 are absent in the 2.0-kb mRNA as a consequence of alternative splicing of the pre-mRNA [107–109].

Presently, there are no known animal models for MPS IVB, either natural or engineered.

6. Mucopolysaccharidosis V

The designation MPS V is no longer used. In fact, the phenotype which was first classified as MPS V, was later found to be the milder form of MPS I (Scheie’s syndrome), caused by deficiencies in α-L-iduronidase, with the typical stiff joints, clouding of the cornea most dense peripherally, survival to a late age with little if any impairment of intellect and aortic regurgitation [44].

7. Mucopolysaccharidosis VI (Maroteaux-Lamy Syndrome)

Mucopolysaccharidosis type VI is an autosomal recessive lysosomal storage disorder resulting from a deficiency of arylsulfatase B (N-acetylgalactosamine-4-sulfatase). Clinical features and severity are variable but usually include short stature, hepatosplenomegaly, dysostosis multiplex, stiff joints, corneal clouding, cardiac abnormalities, and facial dysmorphism. Intelligence is usually normal [110].

Arylsulfatase B is a lysosomal enzyme that removes the C4 sulphate ester group from the N-acetylgalactosamine sugar residue at the nonreducing terminus of dermatan sulphate and chondroitin sulphate, during lysosomal degradation [111]. The gene that codes for this enzyme was first mapped to chromosome 5q11-q13 [112] and is now known to contain 8 exons and span about 206 kb [111].

In 2002, a 3-year-old Siamese/short-haired European cat was referred for clinical disease characterized by dwarfism, facial dysmorphia, paralysis, small and curled ears, corneal clouding, and large areas of alopecia. X-ray examination showed multiple bone dysplasias. These features lead to suspect from a mucopolysaccharide storage disorder. Subsequent analysis proved it to be a natural occurring form of the Maroteaux-Lamy syndrome [15].

This MPS VI model has been extensively used over the last years to test ERT for this specific pathology. In 2003, Auclair and colleagues [113] have evaluated the cats’ response to infusions of recombinant human N-acetylgalactosamine-4-sulfatase (rhASB) and observed an overall improvement in the disease condition at physical, neurological, and skeletal levels. Later, the same team has demonstrated that a high rate of immunotolerance towards rhASB can be achieved in MPS VI cats with a short-course tolerisation regimen [114], which may help the implementation of such procedures. Another interesting approach was designed, specifically to ameliorate joint disease in MPS IVA, through long-term articular administration of rhASB, leading to a notorious improvement in feline joint disease [115]. These successful results lead to the development of clinical trials in MPS VI patients, and three clinical studies including 56 patients have evaluated the efficacy and safety. As a consequence, enzyme replacement therapy (ERT) became available. The specific ERT for MPS VI, galsulfase (Naglazyme, Biomarin Pharmaceutical) was approved in 2005 by FDA and in 2006 by EMA. Long-term follow-up data with patients treated up to 5 years showed that ERT is well tolerated and associated with sustained improvements in the patients' clinical condition [2, 116].

Even though presently there is ERT available for these patients, other therapeutic approaches are being tested in animal models for MPS VI. In 2009, the first attempt of successful gene therapy was performed through lentiviral-mediated gene transfer to joint tissues of the rat, with consequent correction of MPS VI cells [117]. This year, another study, involving intravascular administration of adeno-associated viral vectors in MPS VI cats, was published. After gene transfer the authors observed clearance of GAG storage, improvement of long bone length, reduction of heart valve thickness, and improvement in spontaneous mobility [118]. Either way, promising therapeutic strategies for MPS VI patients may be arising.

8. Mucopolysaccharidosis VII (Sly’s Syndrome)

MPS VII, also known as Sly’s syndrome, is characterized by the impossibility to degrade glucuronic acid-containing GAGs, due to impaired function of β-glucuronidase, which removes the glucuronic acid residues present in dermatan sulphate as well as in heparan and chonroitin sulphates (reviewed in [1]). Clinical features are highly variable, with phenotypes ranging from severe fetal hydrops to mild forms allowing survival into adulthood. Typical features include hepatomegaly, skeletal abnormalities, coarse facial features, and variable degrees of mental impairment [119].

MPS VII was first reported by Sly and collaborators in 1973, in a boy with skeletal changes consistent with MPS, hepatosplenomegaly, and granular inclusions in granulocytes. Additional features included hernias, unusual facies, protruding sternum, thoracolumbar gibbus, vertebral deformities, and mental deficiency. When β-glucuronidase activity was measured in fibroblasts, obtained values were less than 2% of control values. Both parents and several sibs of the mother showed an intermediate level of the enzyme [120].

In 1990, Miller et al. [121] reported that the gene encoding β-glucuronidase (GUSB) is 21 kb long, contains 12 exons, and gives rise to two different types of cDNAs, through an alternate splicing mechanism. Speleman et al. [122] used fluorescence in situ hybridization to map the GUSB gene to 7q11.21-q11.22. This map position was confirmed by dual-color hybridization of β-glucuronidase and another gene which had been mapped proximal to it: elastin (7q11.23).

Several pseudogenes, located on chromosomes 5, 6, 7, 20, 22, and Y, were also detected by Shipley et al. [123], when amplifying exons 2–4, 3, 6-7, and 11.

In 2009, Tomatsu et al. [124] provided a review of mutations in the GUSB gene that cause MPS type VII. Forty-nine different pathogenic mutations have been reported in the literature, with approximately 90% of them being missense mutations. Approximately 40% of the known GUSB mutations occur at CpG sites within the gene. The most common mutation is L176F, which has been found in several populations: American (Caucasian), Brazilian, British, Chilean, French, Mexican, Polish, Spanish, and Turkish ([125–127], reviewed in [124]). Genotype/phenotype analysis indicated that the most severe phenotype was associated with truncating mutations and with mutations affecting either the hydrophobic core or the modification of packing.

In 1984, mucopolysaccharidosis type VII (Sly syndrome) was described in a mixed-breed dog [16]. Since then, several other affected dogs have been studied, in the animal colony established at the University of Pennsylvania, the School of Veterinary Medicine [128] and, later, in a 12-week-old male German Shepherd dog studied in the same school [129]. All dogs shared the same missense mutation and developed similar phenotypes with skeletal deformities, corneal cloudiness, cytoplasmic granules in the neutrophils and lymphocytes of blood and CSF, and glycosaminoglycans in urine [129]. Another animal model was described as naturally occurring: the gus^mps/mps mouse, which has a 1 bp deletion in exon 10 resulting in a progressive degenerative disease that reduces lifespan and causes facial dysmorphism, growth retardation, deafness, and behavioral defects [17]. Nevertheless, opportunities for experimental therapies were greatly expanded by the work of Tomatsu et al., in 2006 [18], who developed a new MPS VII mouse model, which is tolerant to both human and murine GUS, without the characteristic immune responses that complicated evaluation of the long-term benefits of enzyme replacement or gene therapy when the naturally occurring mice were used. Ever since, several therapeutic approaches have been attempted in MPS VII mice, and the results have been encouraging. That is the case of the works by Bosch and collaborators, who have been working on gene therapy for this pathology, in order to correct brain lesions. They have used both adeno-associated virus (AAV) [130] and lentivirus-mediated gene transfer [131] and observed that there was a significant correction of pathology in the brain of affected mice.

Other therapeutic approaches had already been attempted, but their results were not as promising. In fact, in 1998, allogenic bone marrow transplantation was reported in a 12-year-old Japanese girl with consequent improvement of motor function and daily life activities, decrease of upper respiratory and ear infections, but no improvement at all in cognitive function [132].

9. Mucopolysaccharidosis VIII

The clinical entity once known as MPS VIII was described in a single patient, in the late 1970s. The patient, a 5-year-old child, presented short stature, coarse hair, hepatomegaly, mild dysostosis multiplex, mental retardation, and no signs of corneal clouding. Biochemical analysis of the urine revealed increased excretion of keratan and heparan sulphate [133, 134]. The biochemical findings described by this group lead to suspect the existence of two hexosamine sulfatases and propose the existence of this novel MPS, caused by glucosamine-6-sulfatase [133].

Nevertheless, subsequent analysis on Diferrante’s laboratory brought this idea down, and the designation MPS VIII was abandoned [135].

10. Mucopolysaccharidosis IX

Mucopolysaccharidosis IX, also known as hyaluronidase deficiency, is caused by mutations in the HYAL1 gene.

This disease was first discovered by Natowicz et al. [136] in a 14-year-old girl with short stature and multiple periarticular soft-tissue masses. Radiographic analysis showed nodular synovia, acetabular erosions, and a popliteal cyst. Lysosomal storage of hyaluronan (HA) was evident within the macrophages and fibroblasts of biopsied soft-tissue masses, and serum concentrations were elevated 38–90-fold. She was proven to have a storage disease of hyaluronan (hyaluronic acid) due to a genetic deficiency of hyaluronidase. The descriptions of hyaluronidase deficiency in this family are consistent with autosomal recessive inheritance.

In order to determine the molecular basis of MPS IX, Triggs-Raine et al. [137] analyzed 2 different candidate genes tandemly distributed on chromosome 3p21.3, both encoding proteins with homology to a sperm enzyme with hyaluronidase activity. These genes, HYAL1 and HYAL2, encode 2 distinct lysosomal hyaluronidases with different substrate specificities. When characterizing the patient with hyaluronidase deficiency originally reported in [136], they verified that he was a compound heterozygote for 2 mutations in the HYAL1 gene: a missense mutation (c.1412G>A), which introduced a nonconservative amino acid substitution in a putative active site residue (p.Glu268Lys) and a complex intragenic rearrangement, 1361del37ins14, which resulted in a premature termination codon. Through this work, they have also showed that these 2 hyaluronidase genes, together with a third adjacent HYAL3 gene, had markedly different tissue expression patterns, consistent with differing roles in the metabolism of hyaluronan. These findings allowed this team not only to explain the unexpectedly mild phenotype of MPS IX but also to predict the existence of other hyaluronidase-deficiency disorders.

Presently, three other hyaluronidase-related genes (HYAL4, HYALP1, SPAM1) have been identified at 7q31.3 [138]. These genes are predicted to encode hyaluronidases, endoglycosidases that initiate the degradation of HA, a large negatively charged GAG found in the extracellular matrix (ECM) of all vertebrate cells [19].

Since there is only one patient reported to date, the development and characterization of a model of Hyal1 deficiency was the first logical step in understanding the main phenotypic symptoms associated with MPS IX. During this decade, a mouse model for MPS IX has become available and was fully characterized [19]. Overall, it was observed that the murine MPS IX model displays the key features of the human disease. Nevertheless, during the same year, another mutant mouse suffering from a hyaluronidase deficiency was described, this one deficient in HYAL2 [139]. Skeletal and hematological anomalies were described in this model, raising the possibility that a similar defect, defining a new MPS disorder, exists in humans [139].

11. Conclusion

The elucidation of enzyme deficiencies underlying mucopolysaccharidoses was crucial to unveil the normal pathways of glycosaminoglycan catabolism. In fact, only through the consequences of their absence became the role of several enzymes evident. The majority of these enzyme deficiencies were discovered during the 1970s. Over the last decades the enzyme deficiencies underlying each disease, and the molecular defects causing them have been identified and extensively analyzed and characterized. As a result, six different MPS are known, caused by deficiencies in one of the ten different enzymes necessary to intralysosomal degradation of GAGs through one of the four different degradation pathways.

Each disease has its own hallmark features. Nevertheless, a common pattern arouses: MPS are usually chronic, with a progressive course and different severity degrees. Organomegaly, dysostosis multiplex, and CNS involvement are common but not necessary features.

Over the years, several MPS have been recognized in animals as naturally occurring diseases, and others were created by knock-out technology. Most animal colonies have been established from single related heterozygous animals, in such a way that the affected offspring is homozygous for the same mutant allele. All these models present disease pathology similar to that seen in humans, making the animals extremely valuable for both investigation of disease pathogenesis and testing of therapies. Large animal homologues are similar to humans in natural genetic diversity, approaches to therapy and care, and possibility of evaluating long-term effects of treatment. Presently, therapeutic strategies for MPS include enzyme replacement therapy, heterologous bone marrow transplantation, and somatic cell gene transfer, all of which have been tested in animals with some success. During the 80s, transplantation of hematopoietic stem cells was tested for several MPSs. Theoretically, haematopoietic stem cells taken from a normal compatible donor and transplanted into an enzyme-deficient recipient can provide a safe, permanent, and self-replicating source of bone marrow-derived cells. By secreting active lysosomal enzymes, these cells cross-connect nonbone marrow-derived cells. Several animal models for GAGs storage diseases have already been subjected to/undergone BMT. From those experiments, along with human clinical trials already tried, it was possible to verify that there are important variations in therapeutic response among different pathologies with some diseases with CNS pathology which can be successfully treated by BMT (the severe form of MPS I, being the example for the GAG storage disorders; [140]) whereas others cannot (MPS II and III in which BMT was tested with few success; [3, 141]). These variations are usually attributed to the different capacities of secretion, stability, and uptake of each specific enzyme. Nevertheless, important conclusions could be drawn from the collective experience of postnatal transplantation including the idea that the earlier the transplants are performed, the better the clinical response. In the 90s; however, a novel approach started to be tested: ERT. Nowadays, it has been the most tested approach in animal models of GAG storage disorders. Until now, the obtained results have been highlighting the potential of administered recombinant enzyme to reduce GAG accumulation. ERTs are presently available for MPS I (since 2003), II (since 2005), and VI (since 2006). Clinical trials are also in course for MPS IVA treatment through ERT. Nevertheless, this approach is ineffective for the brain since recombinant enzymes are not able to cross the blood-brain barrier (BBB). This is one of the reasons why other therapies are being tested for MPS with CNS involvement. ERT with direct administration of the recombinant enzyme into the brain (intrathecal injections) is also being considered in order to overcome that difficulty. Presently, such approaches are being considered for MPS IIIA and to overcome the cognitive deficit of MPS II and MPS I (reviewed in [142]).

Somatic cell gene transfer is another possible approach, but a long way needs yet to be travelled towards such a therapy is applicable to patients.

Finally, substrate deprivation therapy (or substrate reduction therapy) is also being considered for some MPSs. This approach is being tested with both genistein and rhodamine B (reviewed in [70]). Genistein, a chemical from the group of isoflavones, has been shown to inhibit the synthesis of GAGs in fibroblasts of patients with various forms of MPSs, namely, types I, II, IIIA, and IIIB [4, 143]. Similar results were obtained with rhodamine B, an inhibitor with an unknown mechanism of action. Remarkably, in MPS IIIA mice treated with rhodamine B, GAG storage decreased not only in somatic tissues, but also in brain, with improved behaviours of the animals [144, 145]. These encouraging results lead to the development of open-label pilot clinical studies with children suffering from Sanfilippo’s syndrome types A and B in which a genistein-rich isoflavone extract (SE-2000, Biofarm, Poland) orally administered for 12 months. After one year of treatment, statistically significant improvement in all tested parameters was demonstrated (reviewed in [70]).

In order to better quantify and assess the efficacy of these therapeutic approaches, investigators have been trying to indentify suitable biomarkers for MPS, which allow the evaluation of short- and long-term treatment effects. This is also assuming particular importance since early detection of MPS is an important factor in treatment success. Recently discovered biomarkers include heparin cofactor II-thrombin complex and dermatan sulphate:chondroitin sulphate ratio [146]. Other biomarkers and/or therapeutic targets for MPS joint and bone disease recently identified through animal studies include several proinflammatory cytokines, nitric oxide, and matrix metalloproteinases (MMPs; [147]).

Another hot topic which is recently being discussed refers to the possibility of including some MPSs (particularly type I, IIIA, IIIB, and VI) in neonatal screening programs [148]. The ongoing development of enzyme replacement therapy and other treatments for several LSDs, including MPSs combined with the growing evidence that early commencement of therapy improves outcomes, has increased the pressure for the introduction of newborn screening programs, and a number of pilot studies are ongoing [148–152]. This is only possible thanks to the significant advances that were made in last decade since dried blood spot technology was introduced for enzymatic assays and lysosomal protein profile was developed.

Overall, there are encouraging results, with some therapeutic approaches already approved and others under development. Either way, it is important to stress that the management of MPS requires lifelong attention to the multisystemic involvement by a team of specialists experienced in dealing with these diseases, since none of the therapeutic options currently available result in complete resolution of morbidity.

References

E. F. Neufeld and J. Muenzer, “The mucopolysaccharidoses,” in The Metabolic & Molecular Bases of Inherited Disease, C. R. Scriver, A. L. Beaudet, W. S. Sly, and D. Valle, Eds., vol. 3, McGraw–Hill, New York, NY, USA, 8th edition, 2001.
View at: Google Scholar
R. Giugliani, C. G. Carvalho, S. Herber, and L. L. de Camargo Pinto, “Recent advances in treatment approaches of mucopolysaccharidosis VI,” Current Pharmaceutical Biotechnology, vol. 12, no. 6, pp. 956–962, 2011.
View at: Publisher Site | Google Scholar
M. Haskins, M. Casal, N. M. Ellinwood, J. Melniczek, H. Mazrier, and U. Giger, “Animal models for mucopolysaccharidoses and their clinical relevance,” Acta Paediatrica, vol. 91, no. 439, supplement, pp. 88–97, 2002.
View at: Google Scholar
E. Piotrowska, J. Jakóbkiewicz-Banecka, S. Barańska et al., “Genistein-mediated inhibition of glycosaminoglycan synthesis as a basis for gene expression-targeted isoflavone therapy for mucopolysaccharidoses,” European Journal of Human Genetics, vol. 14, no. 7, pp. 846–852, 2006.
View at: Publisher Site | Google Scholar
M. E. Haskins, P. F. Jezyk, R. J. Desnick, S. K. McDonaugh, and D. F. Patterson, “Alpha L iduronidase deficiency in a cat: a model of mucopolysaccharidosis I,” Pediatric Research, vol. 13, no. 11, pp. 1294–1297, 1979.
View at: Google Scholar
R. M. Shull, R. J. Munger, and E. Spellacy, “Canine α-L-iduronidase deficiency. A model of mucopolysaccharidosis I,” American Journal of Pathology, vol. 109, no. 2, pp. 244–248, 1982.
View at: Google Scholar
L. A. Clarke, C. S. Russell, S. Pownall et al., “Murine mucopolysaccharidosis type I: targeted disruption of the murine α-L-iduronidase gene,” Human Molecular Genetics, vol. 6, no. 4, pp. 503–511, 1997.
View at: Publisher Site | Google Scholar
M. J. Wilkerson, D. C. Lewis, S. L. Marks, and D. J. Prieur, “Clinical and morphologic features of mucopolysaccharidosis type II in a dog: naturally occurring model of Hunter syndrome,” Veterinary Pathology, vol. 35, no. 3, pp. 230–233, 1998.
View at: Google Scholar
A. R. Garcia, J. Pan, J. C. Lamsa, and J. Muenzer, “The characterization of a murine model of mucopolysaccharidosis II (Hunter syndrome),” Journal of Inherited Metabolic Disease, vol. 30, no. 6, pp. 924–934, 2007.
View at: Publisher Site | Google Scholar
A. Fischer, K. P. Carmichael, J. F. Munnell et al., “Sulfamidase deficiency in a family of dachshunds: a canine model of mucopolysaccharidosis IIIA (Sanfilippo A),” Pediatric Research, vol. 44, no. 1, pp. 74–82, 1998.
View at: Google Scholar
R. Bhattacharyya, B. Gliddon, T. Beccari, J. J. Hopwood, and P. Stanley, “A novel missense mutation in lysosomal sulfamidase is the basis of MPS III A in a spontaneous mouse mutant,” Glycobiology, vol. 11, no. 1, pp. 99–103, 2001.
View at: Google Scholar
N. M. Ellinwood, P. Wang, T. Skeen et al., “A model of mucopolysaccharidosis IIIB (Sanfilippo syndrome type IIIB): N-acetyl-α-D-glucosaminidase deficiency in Schipperke dogs,” Journal of Inherited Metabolic Disease, vol. 26, no. 5, pp. 489–504, 2003.
View at: Publisher Site | Google Scholar
J. N. Thompson, M. Z. Jones, G. Dawson, and P. S. Huffman, “N-acetylglucosamine 6-sulphatase deficiency in a Nubian goat: a model of Sanfilippo syndrome type D (mucopoly-saccharidosis IIID),” Journal of Inherited Metabolic Disease, vol. 15, no. 5, pp. 760–768, 1992.
View at: Google Scholar
S. Tomatsu, K. O. Orii, C. Vogler et al., “Mouse model on N-acetylgalactosamine-6-sulfate sulfatase deficiency (Galns-/-) produced by targeted disruption of the gene defective in Morquio A disease,” Human Molecular Genetics, vol. 12, no. 24, pp. 3349–3358, 2003.
View at: Publisher Site | Google Scholar
B. MacRì, F. Marino, G. Mazzullo et al., “Mucopolysaccharidosis VI in a Siamese/short-haired European cat,” Journal of Veterinary Medicine A, vol. 49, no. 8, pp. 438–442, 2002.
View at: Publisher Site | Google Scholar
M. E. Haskins, R. J. Desnick, and N. DiFerrante, “β-glucuronidase deficiency in a dog: a model of human mucopolysaccharidosis VII,” Pediatric Research, vol. 18, no. 10, pp. 980–984, 1984.
View at: Google Scholar
E. H. Birkenmeier, M. T. Davisson, W. G. Beamer et al., “Murine mucopolysaccharidosis type VII. Characterization of a mouse with β-glucuronidase deficiency,” Journal of Clinical Investigation, vol. 83, no. 4, pp. 1258–1266, 1989.
View at: Google Scholar
S. Tomatsu, K. Sukegawa, G. G. Trandafirescu et al., “Differences in methylation patterns in the methylation boundary region of IDS gene in hunter syndrome patients: implications for CpG hot spot mutations,” European Journal of Human Genetics, vol. 14, no. 7, pp. 838–845, 2006.
View at: Publisher Site | Google Scholar
D. C. Martin, V. Atmuri, R. J. Hemming et al., “A mouse model of human mucopolysaccharidosis IX exhibits osteoarthritis,” Human Molecular Genetics, vol. 17, no. 13, pp. 1904–1915, 2008.
View at: Publisher Site | Google Scholar
V. A. McKusick, Heritable Disorders of Connective Tissue, Mosby, St. Louis, Mo, USA, 4th edition, 1972.
H. S. Scott, X. H. Guo, J. J. Hopwood, and C. P. Morris, “Structure and sequence of the human α-L-iduronidase gene,” Genomics, vol. 13, no. 4, pp. 1311–1313, 1992.
View at: Publisher Site | Google Scholar
H. S. Scott, L. J. Ashton, H. J. Eyre et al., “Chromosomal localization of the human α-L-iduronidase gene (IDUA) to 4p16.3,” American Journal of Human Genetics, vol. 47, no. 5, pp. 802–807, 1990.
View at: Google Scholar
E. Spellacy, R. M. Shull, G. Constantopoulos, and E. F. Neufeld, “A canine model of human α-L-iduronidase deficiency,” Proceedings of the National Academy of Sciences of the United States of America, vol. 80, no. 19, pp. 6091–6095, 1983.
View at: Google Scholar
L. J. Stoltzfus, B. Sosa-Pineda, S. M. Moskowitz et al., “Cloning and characterization of cDNA encoding canine α-L-iduronidase. mRNA deficiency in mucopolysaccharidosis I dog,” Journal of Biological Chemistry, vol. 267, no. 10, pp. 6570–6575, 1992.
View at: Google Scholar
K. P. Menon, P. T. Tieu, and E. F. Neufeld, “Architecture of the canine IDUA gene and mutation underlying canine mucopolysaccharidosis I,” Genomics, vol. 14, no. 3, pp. 763–768, 1992.
View at: Publisher Site | Google Scholar
R. M. Shull, E. D. Kakkis, M. F. McEntee, S. A. Kania, A. J. Jonas, and E. F. Neufeld, “Enzyme replacement in a canine model of Hurler syndrome,” Proceedings of the National Academy of Sciences of the United States of America, vol. 91, no. 26, pp. 12937–12941, 1994.
View at: Publisher Site | Google Scholar
C. L. S. Grosson, M. E. MacDonald, M. P. Duyao, C. M. Ambrose, S. Roffler Tarlov, and J. F. Gusella, “Synteny conservation of the Huntington's disease gene and surrounding loci on mouse chromosome 5,” Mammalian Genome, vol. 5, no. 7, pp. 424–428, 1994.
View at: Google Scholar
C. Russell, G. Hendson, G. Jevon et al., “Murine MPS I: insights into the pathogenesis of Hurler syndrome,” Clinical Genetics, vol. 53, no. 5, pp. 349–361, 1998.
View at: Google Scholar
C. Peters, E. G. Shapiro, and W. Krivit, “Neuropsychological development in children with Hurler syndrome following hematopoietic stem cell transplantation,” Pediatric Transplantation, vol. 2, no. 4, pp. 250–253, 1998.
View at: Google Scholar
C. Peters, E. G. Shapiro, and W. Krivit, “Hurler syndrome: past, present, and future,” Journal of Pediatrics, vol. 133, no. 1, pp. 7–9, 1998.
View at: Publisher Site | Google Scholar
S. L. Staba, M. L. Escolar, M. Poe et al., “Cord-blood transplants from unrelated donors in patients with Hurler's syndrome,” New England Journal of Medicine, vol. 350, no. 19, pp. 1960–1969, 2004.
View at: Publisher Site | Google Scholar
J. J. Boelens, R. F. Wynn, A. O'Meara et al., “Outcomes of hematopoietic stem cell transplantation for Hurler's syndrome in Europe: a risk factor analysis for graft failure,” Bone Marrow Transplantation, vol. 40, no. 3, pp. 225–233, 2007.
View at: Publisher Site | Google Scholar
L. A. Clarke, J. E. Wraith, M. Beck et al., “Long-term efficacy and safety of laronidase in the treatment of mucopolysaccharidosis I,” Pediatrics, vol. 123, no. 1, pp. 229–240, 2009.
View at: Publisher Site | Google Scholar
J. E. Wraith, L. A. Clarke, M. Beck et al., “Enzyme replacement therapy for mucopolysaccharidosis I: a randomized, double-blinded, placebo-controlled, multinational study of recombinant human α-L-iduronidase (laronidase),” Journal of Pediatrics, vol. 144, no. 5, pp. 581–588, 2004.
View at: Publisher Site | Google Scholar
H. Harada, H. Uchiwa, M. Nakamura et al., “Laronidase replacement therapy improves myocardial function in mucopolysaccharidosis I,” Molecular Genetics and Metabolism, vol. 103, no. 3, pp. 215–219, 2011.
View at: Publisher Site | Google Scholar
A. Tylki-Szymanska, J. Marucha, A. Jurecka, M. Syczewska, and B. Czartoryska, “Efficacy of recombinant human α-L-iduronidase (laronidase) on restricted range of motion of upper extremities in mucopolysaccharidosis type i patients,” Journal of Inherited Metabolic Disease, vol. 33, no. 2, pp. 151–157, 2010.
View at: Publisher Site | Google Scholar
A. Tylki-Szymanska, A. Rozdzynska, A. Jurecka, J. Marucha, and B. Czartoryska, “Anthropometric data of 14 patients with mucopolysaccharidosis I: retrospective analysis and efficacy of recombinant human α-l-iduronidase (laronidase),” Molecular Genetics and Metabolism, vol. 99, no. 1, pp. 10–17, 2010.
View at: Publisher Site | Google Scholar
O. Gabrielli, L. A. Clarke, S. Bruni, and G. V. Coppa, “Enzyme-replacement therapy in a 5-month-old boy with attenuated presymptomatic MPS I: 5-year follow-up,” Pediatrics, vol. 125, no. 1, pp. e183–e187, 2010.
View at: Publisher Site | Google Scholar
J. E. Wraith, J. G. Rogers, and D. M. Danks, “The mucopolysaccharidoses,” Australian Paediatric Journal, vol. 23, no. 6, pp. 329–334, 1987.
View at: Google Scholar
R. J. Gorlin, M. M. Cohen Jr., and R. C. M. Hennekam, Syndromes of the Head and Neck, Oxford University Press, New York, NY, USA, 4th edition, 2001.
M. D. C. Donaldson, C. A. Pennock, P. J. Berry, A. W. Duncan, J. E. Cawdery, and J. V. Leonard, “Hurler syndrome with cardiomyopathy in infancy,” Journal of Pediatrics, vol. 114, no. 3, pp. 430–432, 1989.
View at: Google Scholar
J. Shapiro, M. Strome, and A. C. Crocker, “Airway obstruction and sleep apnea in Hurler and Hunter syndromes,” Annals of Otology, Rhinology and Laryngology, vol. 94, no. 5 I, pp. 458–461, 1985.
View at: Google Scholar
M. Hanson, J. R. Lupski, J. Hicks, and D. Metry, “Association of dermal melanocytosis with lysosomal storage disease: clinical features and hypotheses regarding pathogenesis,” Archives of Dermatology, vol. 139, no. 7, pp. 916–920, 2003.
View at: Publisher Site | Google Scholar
V. A. McKusick, D. Kaplan, D. Wise et al., “The genetic mucopolysaccharidoses,” Medicine, vol. 44, no. 6, pp. 445–483, 1965.
View at: Google Scholar
C. B. Whitley, “The mucopolysaccharidoses,” in McKusick's Heritable Disorders of Connective Tissue, P. Beighton, Ed., Mosby, St. Louis, Mo, USA, 5th edition, 1993.
View at: Google Scholar
W. H. Perks, R. A. Cooper, and S. Bradbury, “Sleep apnoea in Scheie's syndrome,” Thorax, vol. 35, no. 2, pp. 85–91, 1980.
View at: Google Scholar
J. E. Wraith, M. Scarpa, M. Beck et al., “Mucopolysaccharidosis type II (Hunter syndrome): a clinical review and recommendations for treatment in the era of enzyme replacement therapy,” European Journal of Pediatrics, vol. 167, no. 3, pp. 267–277, 2008.
View at: Publisher Site | Google Scholar
P. J. Wilson, G. K. Suthers, D. F. Callen et al., “Frequent deletions at Xq28 indicate genetic heterogeneity in Hunter syndrome,” Human Genetics, vol. 86, no. 5, pp. 505–508, 1991.
View at: Google Scholar
R. H. Flomen, E. P. Green, P. M. Green, D. R. Bentley, and F. Giannelli, “Determination of the organisation of coding sequences within the iduronate sulphate sulphatase (IDS) gene,” Human Molecular Genetics, vol. 2, no. 1, pp. 5–10, 1993.
View at: Google Scholar
P. J. Wilson, C. A. Meaney, J. J. Hopwood, and C. P. Morris, “Sequence of the human iduronate 2-sulfatase (IDS) gene,” Genomics, vol. 17, no. 3, pp. 773–775, 1993.
View at: Publisher Site | Google Scholar
M. L. Bondeson, H. Malmgren, N. Dahl, B. M. Carlberg, and U. Pettersson, “Presence of an IDS-related locus (IDS2) and Xq28 complicates the mutational analysis of Hunter syndrome,” European Journal of Human Genetics, vol. 3, no. 4, pp. 219–227, 1995.
View at: Google Scholar
C. Peters, M. Balthazor, E. G. Shapiro et al., “Outcome of unrelated donor bone marrow transplantation in 40 children with Hurler syndrome,” Blood, vol. 87, no. 11, pp. 4894–4902, 1996.
View at: Google Scholar
G. V. Coppa, O. Gabrielli, L. Zampini et al., “Bone marrow transplantation in Hunter syndrome (mucopolysaccharidosis type II): two year follow-up of the first Italian patient and review of the literature,” Pediatria Medica e Chirurgica, vol. 17, no. 3, pp. 227–235, 1995.
View at: Google Scholar
E. J. R. McKinnis, S. Sulzbacher, J. C. Rutledge, J. Sanders, and C. R. Scott, “Bone marrow transplantation in Hunter syndrome,” Journal of Pediatrics, vol. 129, no. 1, pp. 145–148, 1996.
View at: Google Scholar
T. A. Burrow and N. D. Leslie, “Review of the use of idursulfase in the treatment of mucopolysaccharidosis II,” Biologics, vol. 2, pp. 311–320, 2008.
View at: Google Scholar
J. Muenzer, J. C. Lamsa, A. Garcia, J. Dacosta, J. Garcia, and D. A. Treco, “Enzyme replacement therapy in mucopolysaccharidosis type II (Hunter syndrome): a preliminary report,” Acta Paediatrica, vol. 91, no. 439, supplement, pp. 98–99, 2002.
View at: Google Scholar
A. R. Garcia, J. M. DaCosta, J. Pan, J. Muenzer, and J. C. Lamsa, “Preclinical dose ranging studies for enzyme replacement therapy with idursulfase in a knock-out mouse model of MPS II,” Molecular Genetics and Metabolism, vol. 91, no. 2, pp. 183–190, 2007.
View at: Publisher Site | Google Scholar
J. Muenzer, M. Gucsavas-Calikoglu, S. E. McCandless, T. J. Schuetz, and A. Kimura, “A phase I/II clinical trial of enzyme replacement therapy in mucopolysaccharidosis II (Hunter syndrome),” Molecular Genetics and Metabolism, vol. 90, no. 3, pp. 329–337, 2007.
View at: Publisher Site | Google Scholar
J. Muenzer, J. E. Wraith, M. Beck et al., “A phase II/III clinical study of enzyme replacement therapy with idursulfase in mucopolysaccharidosis II (Hunter syndrome),” Genetics in Medicine, vol. 8, no. 8, pp. 465–473, 2006.
View at: Publisher Site | Google Scholar
F. Papadia, M. S. Lozupone, A. Gaeta, D. Capodiferro, and G. Lacalendola, “Long-term enzyme replacement therapy in a severe case of mucopolysaccharidosis type II (Hunter syndrome),” European Review for Medical and Pharmacological Sciences, vol. 15, no. 3, pp. 253–258, 2011.
View at: Google Scholar
L. Filippon, C. A. Y. Wayhs, D. M. Atik et al., “DNA damage in leukocytes from pretreatment mucopolysaccharidosis type II patients; protective effect of enzyme replacement therapy,” Mutation Research, vol. 721, no. 2, pp. 206–210, 2011.
View at: Publisher Site | Google Scholar
L. Filippon, C. S. Vanzin, G. B. Biancini et al., “Oxidative stress in patients with mucopolysaccharidosis type II before and during enzyme replacement therapy,” Molecular Genetics and Metabolism, vol. 103, no. 2, pp. 121–127, 2011.
View at: Publisher Site | Google Scholar
J. J. P. Van De Kamp, M. F. Niermeijer, K. Von Figura, and M. A. H. Giesberts, “Genetic heterogeneity and clinical variability in the Sanfilippo syndrome (types A, B, and C),” Clinical Genetics, vol. 20, no. 2, pp. 152–160, 1981.
View at: Google Scholar
H. S. Scott, L. Blanch, X. H. Guo et al., “Cloning of the sulphamidase gene and identification of mutations in Sanfilippo A syndrome,” Nature Genetics, vol. 11, no. 4, pp. 465–467, 1995.
View at: Google Scholar
L. E. Karageorgos, X. H. Guo, L. Blanch et al., “Structure and sequence of the human sulphamidase gene,” DNA Research, vol. 3, no. 4, pp. 269–271, 1996.
View at: Google Scholar
E. L. Aronovich, K. P. Carmichael, H. Morizono et al., “Canine heparan sulfate sulfamidase and the molecular pathology underlying Sanfilippo syndrome type A in Dachshunds,” Genomics, vol. 68, no. 1, pp. 80–84, 2000.
View at: Publisher Site | Google Scholar
K. M. Hemsley and J. J. Hopwood, “Development of motor deficits in a murine model of mucopolysaccharidosis type IIIA (MPS-IIIA),” Behavioural Brain Research, vol. 158, no. 2, pp. 191–199, 2005.
View at: Publisher Site | Google Scholar
C. Settembre, A. Fraldi, L. Jahreiss et al., “A block of autophagy in lysosomal storage disorders,” Human Molecular Genetics, vol. 17, no. 1, pp. 119–129, 2008.
View at: Publisher Site | Google Scholar
A. L. K. Roberts, B. J. Thomas, A. S. Wilkinson, J. M. Fletcher, and S. Byers, “Inhibition of glycosaminoglycan synthesis using rhodamine B in a mouse model of mucopolysaccharidosis type IIIA,” Pediatric Research, vol. 60, no. 3, pp. 309–314, 2006.
View at: Publisher Site | Google Scholar
J. Jakóbkiewicz-Banecka, A. Wegrzyn, and G. Wegrzyn, “Substrate deprivation therapy: a new hope for patients suffering from neuronopathic forms of inherited lysosomal storage diseases,” Journal of Applied Genetics, vol. 48, no. 4, pp. 383–388, 2007.
View at: Google Scholar
D. Dziedzic, G. Wgrzyn, and J. Jakóbkiewicz-Banecka, “Impairment of glycosaminoglycan synthesis in mucopolysaccharidosis type IIIA cells by using siRNA: a potential therapeutic approach for Sanfilippo disease,” European Journal of Human Genetics, vol. 18, no. 2, pp. 200–205, 2010.
View at: Publisher Site | Google Scholar
A. Fraldi, K. Hemsley, A. Crawley et al., “Functional correction of CNS lesions in an MPS-IIIA mouse model by intracerebral AAV-mediated delivery of sulfamidase and SUMF1 genes,” Human Molecular Genetics, vol. 16, no. 22, pp. 2693–2702, 2007.
View at: Publisher Site | Google Scholar
H. G. Zhao, H. H. Li, A. Schmidtchen, G. Bach, and E. F. Neufeld, “The gene encoding alpha-N-acetylglucosaminidase and mutations underlying Sanfilippo B syndrome,” American Journal of Human Genetics, vol. 57, p. A185, 1995.
View at: Google Scholar
H. G. Zhao, H. H. Li, G. Bach, A. Schmidtchen, and E. F. Neufeld, “The molecular basis of Sanfilippo syndrome type B,” Proceedings of the National Academy of Sciences of the United States of America, vol. 93, no. 12, pp. 6101–6105, 1996.
View at: Publisher Site | Google Scholar
H. H. Li, W. H. Yu, N. Rozengurt et al., “Mouse model of Sanfilippo syndrome type B produced by targeted disruption of the gene encoding alpha-N-acetylglucosaminidase,” Proc Natl Acad Sci USA, vol. 96, no. 5, pp. 14505–14510, 1999.
View at: Google Scholar
W. H. Yu, K. W. Zhao, S. Ryazantsev, N. Rozengurt, and E. F. Neufeld, “Short-term enzyme replacement in the murine model of sanfilippo syndrome type B,” Molecular Genetics and Metabolism, vol. 71, no. 4, pp. 573–580, 2000.
View at: Publisher Site | Google Scholar
K. W. Zhao and E. F. Neufeld, “Purification and characterization of recombinant human α-N-acetylglucosaminidase secreted by Chinese hamster ovary cells,” Protein Expression and Purification, vol. 19, no. 1, pp. 202–211, 2000.
View at: Publisher Site | Google Scholar
B. Weber, J. J. Hopwood, and G. Yogalingam, “Expression and characterization of human recombinant and α-N-actylglucosaminidase,” Protein Expression and Purification, vol. 21, no. 2, pp. 251–259, 2001.
View at: Publisher Site | Google Scholar
M. Beck, “New therapeutic options for lysosomal storage disorders: enzyme replacement, small molecules and gene therapy,” Human Genetics, vol. 121, no. 1, pp. 1–22, 2007.
View at: Publisher Site | Google Scholar
H. Fu, R. J. Samulski, T. J. McCown, Y. J. Picornell, D. Fletcher, and J. Muenzer, “Neurological correction of lysosomal storage in a mucopolysaccharidosis IIIB mouse model by adeno-associated virus-mediated gene delivery,” Molecular Therapy, vol. 5, no. 1, pp. 42–49, 2002.
View at: Publisher Site | Google Scholar
A. Cressant, N. Desmaris, L. Verot et al., “Improved behavior and neuropathology in the mouse model of sanfilippo type IIIB disease after adeno-associated virus-mediated gene transfer in the striatum,” Journal of Neuroscience, vol. 24, no. 45, pp. 10229–10239, 2004.
View at: Publisher Site | Google Scholar
C. D. Heldermon, K. K. Ohlemiller, E. D. Herzog et al., “Therapeutic efficacy of bone marrow transplant, intracranial AAV-mediated gene therapy, or both in the mouse model of MPS IIIB,” Molecular Therapy, vol. 18, no. 5, pp. 873–880, 2010.
View at: Publisher Site | Google Scholar
P. Di Natale, C. Di Domenico, N. Gargiulo et al., “Treatment of the mouse model of mucopolysaccharidosis type IIIB with lentiviral-NAGLU vector,” Biochemical Journal, vol. 388, no. 2, pp. 639–646, 2005.
View at: Publisher Site | Google Scholar
G. R. D. Villani, A. Follenzi, B. Vanacore, C. Di Domenico, L. Naldini, and P. Di Natale, “Correction of mucopolysaccharidosis type IIIB fibroblasts by lentiviral vector-mediated gene transfer,” Biochemical Journal, vol. 364, no. 3, pp. 747–753, 2002.
View at: Publisher Site | Google Scholar
C. Di Domenico, G. R. D. Villani, D. Di Napoli et al., “Intracranial gene delivery of LV-NAGLU vector corrects neuropathology in murine MPS IIIB,” American Journal of Medical Genetics A, vol. 149, no. 6, pp. 1209–1218, 2009.
View at: Publisher Site | Google Scholar
X. Fan, H. Zhang, S. Zhang et al., “Identification of the gene encoding the enzyme deficient in mucopolysaccharidosis IIIC (Sanfilippo disease type C),” American Journal of Human Genetics, vol. 79, no. 4, pp. 738–744, 2006.
View at: Publisher Site | Google Scholar
M. Hřebíček, L. Mrázová, V. Seyrantepe et al., “Mutations in TMEM $76^{*}$ cause mucopolysaccharidosis IIIC (Sanfilippo C syndrome),” American Journal of Human Genetics, vol. 79, no. 5, pp. 807–819, 2006.
View at: Publisher Site | Google Scholar
M. Feldhammer, S. Durand, and A. V. Pshezhetsky, “Protein misfolding as an underlying molecular defect in mucopolysaccharidosis III type C,” PloS one, vol. 4, no. 10, article e7434, 2009.
View at: Google Scholar
S. Durand, M. Feldhammer, E. Bonneil, P. Thibault, and A. V. Pshezhetsky, “Analysis of the biogenesis of heparan sulfate acetyl-CoA: α- glucosaminide N-acetyltransferase provides insights into the mechanism underlying its complete deficiency in mucopolysaccharidosis IIIC,” Journal of Biological Chemistry, vol. 285, no. 41, pp. 31233–31242, 2010.
View at: Publisher Site | Google Scholar
A. O. Fedele and J. J. Hopwood, “Functional analysis of the HGSNAT gene in patients with mucopolysaccharidosis IIIC (Sanfilippo C syndrome),” Human Mutation, vol. 31, no. 7, pp. E1574–E1586, 2010.
View at: Publisher Site | Google Scholar
C. Freeman, P. R. Clements, and J. J. Hopwood, “Human liver N-acetylglucosamine-6-sulphate sulphatase. Purification and characterization,” Biochemical Journal, vol. 246, no. 2, pp. 347–354, 1987.
View at: Google Scholar
C. Freeman and J. J. Hopwood, “Human liver N-acetylglucosamine-6-phosphate sulphatase. Catalytic properties,” Biochemical Journal, vol. 246, no. 2, pp. 355–365, 1987.
View at: Google Scholar
D. A. Robertson, D. F. Callen, E. G. Baker, C. P. Morris, and J. J. Hopwood, “Chromosomal localization of the gene for human glucosamine-6-sulphatase to 12q14,” Human Genetics, vol. 79, no. 2, pp. 175–178, 1988.
View at: Google Scholar
A. Mok, H. Cao, and R. A. Hegele, “Genomic basis of mucopolysaccharidosis type IIID (MIM 252940) revealed by sequencing of GNS encoding N-acetylglucosamine-6-sulfatase,” Genomics, vol. 81, no. 1, pp. 1–5, 2003.
View at: Publisher Site | Google Scholar
C. E. Beesley, D. Burke, M. Jackson, A. Vellodi, B. G. Winchester, and E. P. Young, “Sanfilippo syndrome type D: identification of the first mutation in the N-acetylglucosamine-6-sulphatase gene,” Journal of Medical Genetics, vol. 40, no. 3, pp. 192–194, 2003.
View at: Google Scholar
E. Downs-Kelly, M. Z. Jones, J. Alroy et al., “Caprine mucopolysaccharidosis IIID: a preliminary trial of enzyme replacement therapy,” Journal of Molecular Neuroscience, vol. 15, no. 3, pp. 251–262, 2000.
View at: Publisher Site | Google Scholar
A. M. Montaño, S. Tomatsu, A. Brusius, M. Smith, and T. Orii, “Growth charts for patients affected with Morquio A disease,” American Journal of Medical Genetics A, vol. 146, no. 10, pp. 1286–1295, 2008.
View at: Publisher Site | Google Scholar
S. Tomatsu, S. Fukuda, M. Masue, K. Sukegawa, M. Masuno, and T. Orii, “Mucopolysaccharidosis type IVA: characterization and chromosomal localization of N-acetylgalactosamine-6-sulfate sulfatase gene and genetic heterogeneity,” American Journal of Human Genetics, vol. 51, p. A178, 1992.
View at: Google Scholar
Y. Nakashima, S. Tomatsu, T. Hori et al., “Mucopolysaccharidosis IV A: molecular cloning of the human N- acetylgalactosamine-6-sulfatase gene (GALNS) and analysis of the 5'-flanking region,” Genomics, vol. 20, no. 1, pp. 99–104, 1994.
View at: Publisher Site | Google Scholar
C. P. Morris, X. H. Guo, S. Apostolou, J. J. Hopwood, and H. S. Scott, “Morquio A syndrome: cloning, sequence, and structure of the human N- acetylgalactosamine 6-sulfatase (GALNS) gene,” Genomics, vol. 22, no. 3, pp. 652–654, 1994.
View at: Publisher Site | Google Scholar
S. Tomatsu, A. M. Montaño, A. Ohashi et al., “Enzyme replacement therapy in a murine model of Morquio A syndrome,” Human Molecular Genetics, vol. 17, no. 6, pp. 815–824, 2008.
View at: Publisher Site | Google Scholar
S. Tomatsu, A. M. Montaño, H. Oikawa et al., “Mucopolysaccharidosis type IVA (morquio a disease): clinical review and current treatment: a special review,” Current Pharmaceutical Biotechnology, vol. 12, no. 6, pp. 931–945, 2011.
View at: Publisher Site | Google Scholar
A. Rodríguez, A. J. Espejo, A. Hernández et al., “Enzyme replacement therapy for Morquio A: an active recombinant N-acetylgalactosamine-6-sulfate sulfatase produced in Escherichia coli BL21,” Journal of Industrial Microbiology and Biotechnology, vol. 37, no. 11, pp. 1193–1201, 2010.
View at: Publisher Site | Google Scholar
A. Oshima, A. Tsuji, Y. Nagao, H. Sakuraba, and Y. Suzuki, “Cloning, sequencing, and expression of cDNA for human β-galactosidase,” Biochemical and Biophysical Research Communications, vol. 157, no. 1, pp. 238–244, 1988.
View at: Google Scholar
R. Santamaria, M. Blanco, A. Chabas, D. Grinberg, and L. Vilageliu, “Identification of 14 novel GLB1 mutations, including five deletions, in 19 patients with GM1 gangliosidosis from South America,” Clinical Genetics, vol. 71, no. 3, pp. 273–279, 2007.
View at: Publisher Site | Google Scholar
T. Takano and Y. Yamanouchi, “Assignment of human β-galactosidase-A gene to 3p21.33 by fluorescence in situ hybridization,” Human Genetics, vol. 92, no. 4, pp. 403–404, 1993.
View at: Publisher Site | Google Scholar
H. Morreau, N. J. Galjart, N. Gillemans, R. Willemsen, G. T. J. Van Der Horst, and A. D'Azzo, “Alternative splicing of β-galactosidase mRNA generates the classic lysosomal enzyme and a β-galactosidase-related protein,” Journal of Biological Chemistry, vol. 264, no. 34, pp. 20655–20663, 1989.
View at: Google Scholar
E. Hinek, “Biological roles of the non-integrin elastin/laminin receptor,” Biological Chemistry, vol. 377, no. 7-8, pp. 471–480, 1996.
View at: Google Scholar
S. Privitera, C. A. Prody, J. W. Callahan, and A. Hinek, “The 67-kDa enzymatically inactive alternatively spliced variant of β- galactosidase is identical to the elastin/laminin-binding protein,” Journal of Biological Chemistry, vol. 273, no. 11, pp. 6319–6326, 1998.
View at: Publisher Site | Google Scholar
A. C. M. M. Azevedo, I. V. Schwartz, L. Kalakun et al., “Clinical and biochemical study of 28 patients with mucopolysaccharides type VI,” Clinical Genetics, vol. 66, no. 3, pp. 208–213, 2004.
View at: Publisher Site | Google Scholar
L. Karageorgos, D. A. Brooks, A. Pollard et al., “Mutational analysis of 105 mucopolysaccharidosis type VI patients,” Human Mutation, vol. 28, no. 9, pp. 897–903, 2007.
View at: Publisher Site | Google Scholar
E. Fidzianska, T. Abramowicz, and B. Czartoryska, “Assignment of the gene for human arylsulfatase B, ARSB, to chromosome region 5p $11 \to 5$ qter,” Cytogenetics and Cell Genetics, vol. 38, no. 2, pp. 150–151, 1984.
View at: Google Scholar
D. Auclair, J. J. Hopwood, D. A. Brooks, J. F. Lemontt, and A. C. Crawley, “Replacement therapy in Mucopolysaccharidosis type VI: advantages of early onset of therapy,” Molecular Genetics and Metabolism, vol. 78, no. 3, pp. 163–174, 2003.
View at: Publisher Site | Google Scholar
D. Auclair, J. Finnie, J. White et al., “Repeated intrathecal injections of recombinant human 4-sulphatase remove dural storage in mature mucopolysaccharidosis VI cats primed with a short-course tolerisation regimen,” Molecular Genetics and Metabolism, vol. 99, no. 2, pp. 132–141, 2010.
View at: Publisher Site | Google Scholar
D. Auclair, J. J. Hopwood, J. F. Lemontt, L. Chen, and S. Byers, “Long-term intra-articular administration of recombinant human N-acetylgalactosamine-4-sulfatase in feline mucopolysaccharidosis VI,” Molecular Genetics and Metabolism, vol. 91, no. 4, pp. 352–361, 2007.
View at: Publisher Site | Google Scholar
P. Harmatz, R. Giugliani, I. V. D. Schwartz et al., “Long-term follow-up of endurance and safety outcomes during enzyme replacement therapy for mucopolysaccharidosis VI: final results of three clinical studies of recombinant human N-acetylgalactosamine 4-sulfatase,” Molecular Genetics and Metabolism, vol. 94, no. 4, pp. 469–475, 2008.
View at: Publisher Site | Google Scholar
S. Byers, M. Rothe, J. Lalic, R. Koldej, and D. S. Anson, “Lentiviral-mediated correction of MPS VI cells and gene transfer to joint tissues,” Molecular Genetics and Metabolism, vol. 97, no. 2, pp. 102–108, 2009.
View at: Publisher Site | Google Scholar
G. Cotugno, P. Annunziata, A. Tessitore et al., “Long-term amelioration of feline mucopolysaccharidosis VI after AAV-mediated liver gene transfer,” Molecular Therapy, vol. 19, pp. 461–469, 2011.
View at: Publisher Site | Google Scholar
J. M. Shipley, M. Klinkenberg, B. M. Wu, D. R. Bachinsky, J. H. Grubb, and W. S. Sly, “Mutational analysis of a patient with mucopolysaccharidosis type VII, and identification of pseudogenes,” American Journal of Human Genetics, vol. 52, no. 3, pp. 517–526, 1993.
View at: Google Scholar
W. S. Sly, B. A. Quinton, W. H. McAlister, and D. L. Rimoin, “Beta glucuronidase deficiency: report of clinical, radiologic, and biochemical features of a new mucopolysaccharidosis,” The Journal of Pediatrics, vol. 82, no. 2, pp. 249–257, 1973.
View at: Google Scholar
R. D. Miller, J. W. Hoffmann, P. P. Powell et al., “Cloning and characterization of the human β-glucuronidase gene,” Genomics, vol. 7, no. 2, pp. 280–283, 1990.
View at: Publisher Site | Google Scholar
F. Speleman, R. Vervoort, N. Van Roy, I. Liebaers, W. S. Sly, and W. Lissens, “Localization by fluorescence in situ hybridization of the human functional β-glucuronidase gene (GUSB) to 7q11.21 → q11.22 and two pseudogenes to 5p13 and 5q13,” Cytogenetics and Cell Genetics, vol. 72, no. 1, pp. 53–55, 1996.
View at: Google Scholar
J. M. Shipley, M. Klinkenberg, B. M. Wu, D. R. Bachinsky, J. H. Grubb, and W. S. Sly, “Mutational analysis of a patient with mucopolysaccharidosis type VII, and identification of pseudogenes,” American Journal of Human Genetics, vol. 52, no. 3, pp. 517–526, 1993.
View at: Google Scholar
S. Tomatsu, A. M. Montano, V. C. Dung, J. H. Grubb, and W. S. Sly, “Mutations and polymorphisms in GUSB gene in mucopolysaccharidosis VII (sly syndrome),” Human Mutation, vol. 30, no. 4, pp. 511–519, 2009.
View at: Publisher Site | Google Scholar
B. M. Wu, S. Tomatsu, S. Fukuda, K. Sukegawa, T. Orii, and W. S. Sly, “Overexpression rescues the mutant phenotype of L176F mutation causing β- glucuronidase deficiency mucopolysaccharidosis in two Mennonite siblings,” Journal of Biological Chemistry, vol. 269, no. 38, pp. 23681–23688, 1994.
View at: Google Scholar
R. Vervoort, M. R. Islam, W. S. Sly et al., “Molecular analysis of patients with β-glucuronidase deficiency presenting as hydrops fetalis or as early mucopolysaccharidosis VII,” American Journal of Human Genetics, vol. 58, no. 3, pp. 457–471, 1996.
View at: Google Scholar
I. Schwartz, L. R. Silva, S. Leistner et al., “Mucopolysaccharidosis VII: clinical, biochemical and molecular investigation of a Brazilian family,” Clinical Genetics, vol. 64, no. 2, pp. 172–175, 2003.
View at: Publisher Site | Google Scholar
M. E. Haskins, G. D. Aguirre, P. F. Jezyk, E. H. Schuchman, R. J. Desnick, and D. F. Patterson, “Mucopolysaccharidosis type VII (Sly syndrome): beta-glucuronidase-deficient mucopolysaccharidosis in the dog,” American Journal of Pathology, vol. 138, no. 6, pp. 1553–1555, 1991.
View at: Google Scholar
D. C. S. Dombrowski, K. P. Carmichael, P. Wang, T. M. O'Malley, M. E. Haskins, and U. Giger, “Mucopolysaccharidosis type VII in a German shepherd dog,” Journal of the American Veterinary Medical Association, vol. 224, no. 4, pp. 553–532, 2004.
View at: Publisher Site | Google Scholar
A. Bosch, E. Perret, N. Desmaris, and J. M. Heard, “Long-term and significant correction of brain lesions in adult mucopolysaccharidosis type VII mice using recombinant AAV vectors,” Molecular Therapy, vol. 1, no. 1, pp. 63–70, 2000.
View at: Publisher Site | Google Scholar
A. Bosch, E. Perret, N. Desmaris, D. Trono, and J. M. Heard, “Reversal of pathology in the entire brain of mucopolysaccharidosis type VII mice after lentivirus-mediated gene transfer,” Human Gene Therapy, vol. 11, no. 8, pp. 1139–1150, 2000.
View at: Publisher Site | Google Scholar
Y. Yamada, K. Kato, K. Sukegawa et al., “Treatment of MPS VII (Sly disease) by allogeneic BMT in a female with homozygous A619V mutation,” Bone Marrow Transplantation, vol. 21, no. 6, pp. 629–634, 1998.
View at: Google Scholar
L. C. Ginsburg, D. T. DiFerrante, C. T. Caskey, and N. M. DiFerrante, “Glucosamine-6-SO₄ sulfatase deficiency: a new mucopolysaccharidosis,” Clinical Research, vol. 25, p. 471A, 1977.
View at: Google Scholar
L. C. Ginsberg, P. V. Donnelly, and D. T. Di Ferrante, “N-acetylglucosamine-6-sulfate sulfatase in man: deficiency of the enzyme in a new mucopolysaccharidosis,” Pediatric Research, vol. 12, no. 7, pp. 805–809, 1978.
View at: Google Scholar
N. Di Ferrante, “N-acetylglucosamine-6-sulfate sulfatase deficiency reconsidered,” Science, vol. 210, no. 4468, p. 448, 1980.
View at: Google Scholar
M. R. Natowicz, M. P. Short, Y. Wang et al., “Brief report: clinical and biochemical manifestations of hyaluronidase deficiency,” New England Journal of Medicine, vol. 335, no. 14, pp. 1029–1033, 1996.
View at: Publisher Site | Google Scholar
B. Triggs-Raine, T. J. Salo, H. Zhang, B. A. Wicklow, and M. R. Natowicz, “Mutations in HYAL1, a member of a tandemly distributed multigene family encoding disparate hyaluronidase activities, cause a newly described lysosomal disorder, mucopolysaccharidosis IX,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 11, pp. 6296–6300, 1999.
View at: Publisher Site | Google Scholar
A. B. Csoka, G. I. Frost, and R. Stern, “The six hyaluronidase-like genes in the human and mouse genomes,” Matrix Biology, vol. 20, no. 8, pp. 499–508, 2001.
View at: Publisher Site | Google Scholar
L. Jadin, X. Wu, H. Ding et al., “Skeletal and hematological anomalies in HYAL2-deficient mice: a second type of mucopolysaccharidosis IX?” FASEB Journal, vol. 22, no. 12, pp. 4316–4326, 2008.
View at: Publisher Site | Google Scholar
W. Krivit, “Allogeneic stem cell transplantation for the treatment of lysosomal and peroxisomal metabolic diseases,” Springer Seminars in Immunopathology, vol. 26, no. 1-2, pp. 119–132, 2004.
View at: Publisher Site | Google Scholar
R. Lachmann, “Treatments for lysosomal storage disorders,” Biochemical Society Transactions, vol. 38, no. 6, pp. 1465–1468, 2010.
View at: Publisher Site | Google Scholar
P. I. Dickson and A. H. Chen, “Intrathecal enzyme replacement therapy for mucopolysaccharidosis I: translating success in animal models to patients,” Current Pharmaceutical Biotechnology, vol. 12, no. 6, pp. 946–955, 2011.
View at: Publisher Site | Google Scholar
A. Friso, R. Tomanin, M. Salvalaio, and M. Scarpa, “Genistein reduces glycosaminoglycan levels in a mouse model of mucopolysaccharidosis type II,” British Journal of Pharmacology, vol. 159, no. 5, pp. 1082–1091, 2010.
View at: Publisher Site | Google Scholar
A. L. K. Roberts, B. J. Thomas, A. S. Wilkinson, J. M. Fletcher, and S. Byers, “Inhibition of glycosaminoglycan synthesis using rhodamine B in a mouse model of mucopolysaccharidosis type IIIA,” Pediatric Research, vol. 60, no. 3, pp. 309–314, 2006.
View at: Publisher Site | Google Scholar
A. L. K. Roberts, M. H. Rees, S. Klebe, J. M. Fletcher, and S. Byers, “Improvement in behaviour after substrate deprivation therapy with rhodamine B in a mouse model of MPS IIIA,” Molecular Genetics and Metabolism, vol. 92, no. 1-2, pp. 115–121, 2007.
View at: Publisher Site | Google Scholar
K. J. Langford-Smith, J. Mercer, J. Petty et al., “Heparin cofactor II-thrombin complex and dermatan sulphate: chondroitin sulphate ratio are biomarkers of short- and long-term treatment effects in mucopolysaccharide diseases,” Journal of Inherited Metabolic Disease, vol. 34, no. 2, pp. 499–508, 2011.
View at: Publisher Site | Google Scholar
C. M. Simonaro, M. D'Angelo, M. E. Haskins, and E. H. Schuchman, “Joint and bone disease in mucopolysaccharidoses VI and VII: identification of new therapeutic targets and BioMarkers using animal models,” Pediatric Research, vol. 57, no. 5 I, pp. 701–707, 2005.
View at: Publisher Site | Google Scholar
M. Fuller, J. N. Tucker, D. L. Lang et al., “Screening patients referred to a metabolic clinic for lysosomal storage disorders,” Journal of Medical Genetics, vol. 48, no. 6, pp. 422–425, 2011.
View at: Publisher Site | Google Scholar
M. Spada, S. Pagliardini, M. Yasuda et al., “High incidence of later-onset Fabry disease revealed by newborn screening,” American Journal of Human Genetics, vol. 79, no. 1, pp. 31–40, 2006.
View at: Publisher Site | Google Scholar
H. Y. Lin, K. W. Chong, J. H. Hsu et al., “High incidence of the cardiac variant of fabry disease revealed by newborn screening in the Taiwan Chinese population,” Circulation, vol. 2, no. 5, pp. 450–456, 2009.
View at: Publisher Site | Google Scholar
Y. H. Chien, S. C. Chiang, X. K. Zhang et al., “Early detection of pompe disease by newborn screening is feasible: results from the Taiwan screening program,” Pediatrics, vol. 122, no. 1, pp. e39–e45, 2008.
View at: Publisher Site | Google Scholar
P. K. Duffner, M. Caggana, J. J. Orsini et al., “Newborn screening for Krabbe disease: the New York state model,” Pediatric Neurology, vol. 40, no. 4, pp. 245–252, 2009.
View at: Publisher Site | Google Scholar

Copyright

Copyright © 2012 Maria Francisca Coutinho et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

PDF Download Citation

Download other formats

Order printed copies

Views

29014

Downloads

5683

Citations