You are currently viewing a new version of our website. To view the old version click .
MDPIMDPI
Search all articles
Genes
Download PDF
  • Review
  • Open Access

5 March 2020

Inherited Renal Tubulopathies—Challenges and Controversies

and
1
UCL-Centre for Nephrology, Royal Free Campus, University College London, Rowland Hill Street, London NW3 2PF, UK
2
Rare & Inherited Disease Laboratory, London North Genomic Laboratory Hub, Great Ormond Street Hospital for Children National Health Service Foundation Trust, Levels 4-6 Barclay House 37, Queen Square, London WC1N 3BH, UK
*
Author to whom correspondence should be addressed.
Genes2020, 11(3), 277;https://doi.org/10.3390/genes11030277
This article belongs to the Special Issue Genetics of Tubulopathies
Version Notes
Order Reprints

Abstract

Electrolyte homeostasis is maintained by the kidney through a complex transport function mostly performed by specialized proteins distributed along the renal tubules. Pathogenic variants in the genes encoding these proteins impair this function and have consequences on the whole organism. Establishing a genetic diagnosis in patients with renal tubular dysfunction is a challenging task given the genetic and phenotypic heterogeneity, functional characteristics of the genes involved and the number of yet unknown causes. Part of these difficulties can be overcome by gathering large patient cohorts and applying high-throughput sequencing techniques combined with experimental work to prove functional impact. This approach has led to the identification of a number of genes but also generated controversies about proper interpretation of variants. In this article, we will highlight these challenges and controversies.

1. Introduction

Mutations in genes that encode transporter proteins in the renal tubule alter kidney capacity to maintain homeostasis and cause diseases recognized under the generic name of inherited tubulopathies. Hereditary tubulopathies constitute a heterogeneous group of rare diseases with a global prevalence that is still difficult to estimate. Although by combining genetic and functional studies, we have reached a better understanding of the mechanisms of these disorders, and the genetic cause for a significant number of affected patients is still unknown. This may derive from the variable clinical picture, overlapping phenotypes, insufficient exploration of the genome, mostly of non-coding areas, or incomplete knowledge about the genes governing renal tubular function.
Next-generation sequencing (NGS) has become increasingly accessible for both research and clinical practice and brought new challenges into the interpretation process [1,2,3]. Some of the challenges associated with it are derived from the technology itself (a higher number of variants in genes other than the gene of interest, incidental discoveries eliciting ethical issues, hard to sequence genomic regions) [1,4]. Other challenges are related to the limited information available to interpret the variants. Genetic heterogeneity, pleiotropy, variable penetrance, and expressivity, overlapping phenotypes, at least during the early stages, may influence interpretation. Bartter and Gitelman syndromes represent the best examples in this respect [5,6,7]. Occasionally, acquired disorders can mimic genetic tubulopathies (for example, a Gitelman-like syndrome as a rare consequence of Sjögren syndrome) and thus initiate a diagnostic odyssey for the patient. In this article, we aim to highlight the most frequent and recent challenges and controversies raised by the genetic diagnosis of inherited tubulopathies.

2. Exploring the Genetic Causes of Tubulopathies

The evolution of genetic technologies has facilitated the discovery of a large number of disease genes, initially starting with the identification of a candidate gene based on its linkage with certain markers transmitted with the disease in affected families (positional cloning). Sanger sequencing was introduced in 1977 [8] and has supported gene discovery and diagnosis for more than four decades. Human genes vary in length from several hundreds to a few million base pairs [9], which makes Sanger sequencing a very inefficient method for mutation detection in large genes or sets of genes. It is still used in clinical practice to validate results obtained through faster, high-throughput methods. Next-generation sequencing of whole or targeted exomes or even whole genomes circumvented issues like the partial overlap of certain phenotypes and the genetic heterogeneity [10,11,12]. This progress was accompanied by the discovery of a subset of variants that can be difficult to interpret with current knowledge [13,14,15]. To safeguard the accuracy of genetic diagnosis, guidelines for variant interpretation have been developed and published by the American College of Medical Genetics [16]. These recommendations proved to be very useful in clinical context, when variants in validated genes are investigated. An initial evaluation of how different labs apply these criteria showed substantial disagreement [17], but following subsequent discussions led to an improved consistency [18,19]. However, when new genes or new inheritance patterns are discovered, these guidelines are insufficient. Experimental evidence has shown that the physicochemical nature of an amino acid change, conservation through multiple species, and the rarity of the variant are not always indicative of pathogenicity [20,21,22]. Once large-scale sequencing became available and the results collected into large populational datasets like Exome Aggregation Consortium (ExAc) [23] and Genome Aggregation Database (gnomAD) [24], some of the variants previously considered to be causal for a rare disease have been re-classified as uncertain significance or non-pathogenic [21,25] after being found in large numbers in the control population.

3. Animal Models Do Not Always Reflect Human Disease

One aspect impeding a better understanding of the changes of renal physiology induced by mutations in genes responsible for tubular transport is the inconsistent reproduction of the phenotype in animal models [26]. For example, the mouse expressing GATM (Glycine Amidinotransferase) mutants causing AD renal Fanconi syndrome did not show any aminoaciduria or glucosuria [27]. This is also dependent on the type of genetic modification: (a) knock-out mouse reproducing the effect of a loss-of-function variant is the most used model; (b) knock-in mouse obtained by editing the gene to include the precise pathogenic variant identified in patients. A knock-in experiment introducing the missense WNK4 (WNK Lysine Deficient Protein Kinase 4) mutation p.(Q562E) identified the pathogenic mechanism resulting in pseudohypoaldosteronism type II in humans and a similar phenotype in mice [28]. In the case of SLC34A1 (Solute Carrier Family 34 Member 1), two mouse models of Slc34a1 deficiency either due to genetic deletion or to the spontaneous occurrence of the compound heterozygous mutations at p.(L499V) and p.(V528M) show no Fanconi syndrome [29,30]. However, a mouse bearing two Slc34a1 missense mutations presented electrolytic abnormalities due to a trafficking defect [30,31]. OCRL (Inositol Polyphosphate-5-Phosphatase) KO mice did not exhibit Lowe syndrome/Dent disease unless Inpp5b (Inositol Polyphosphate-5-Phosphatase B) was deleted in the proximal tubule as well. This is due to the specific redundancy of Ocrl and Inpp5b in mice which required a deletion of either both genes or replacement of Inpp5b with the human gene to obtain similar phenotype to the one observed in Lowe patients [32]. The zebrafish model has impaired endocytosis, but normal cilia function [33]. SLC26A1 (Solute Carrier Family 26 Member 1) is an anion exchanger with expression in a limited number of tissues (liver, gut, and kidney). The KO mice exhibit hyposulfatemia, hypersulfaturia, calcium oxalate urolithiasis, and nephrocalcinosis [34]. In addition, they have an increased sensitivity to acetaminophen, which is a significant aspect for pharmacogenetics studies in humans [34]. The differences between humans and mice or other animal models challenge our capacity to document the functional effects of genetic variants.

4. Large-Scale Sequencing Projects Have Variable Diagnostic Yields

Two large multicentre studies identified a mutation in 70% of the children [7] and about 26% in adults [6] with clinically diagnosed tubulopathies. Another study found a genetic diagnosis in 7% of 235 Pakistani patients diagnosed with nephrolithiasis [35]. Braun et al. found a monogenic cause of nephrolithiasis (NL) or nephrocalcinosis in close to 17% [36] of the patients, in which the recessive mutations were more frequent than the autosomal dominant. This proportion is similar to another study that included both children and adults with NL [37]. Smaller scale projects were dedicated to distal renal tubular acidosis (dRTA) [38], Dent disease [39,40], and Gitelman syndrome [41] providing genetic confirmation of the diagnosis in variable proportions. The high number of cases with an unresolved genetic diagnosis can be explained by the complex nature of tubulopathies, with both genetic and environmental factors contributing to the disease, as well as the limited knowledge about the contribution of other genes, the small number of patients with some very rare conditions and phenotype variability. The number of studied genes differed in each case. An internationally reviewed resource, PanelApp, attempts to gather expert knowledge to support inclusion of new genes and a permanent review of known genes as part of gene panels for molecular diagnosis [42]. The tubulopathy panel contains 57 genes of which 38 are validated with high confidence (https://panelapp.genomicsengland.co.uk/panels/292/; accessed 27/02/2020) according to the number of cases, functional studies supporting causality and other supporting evidence. Two genes, HNF4A (Hepatocyte Nuclear Factor 4 Alpha) and SLC2A2 (Solute Carrier Family 2 Member 2) causing renal Fanconi syndrome 4 and Fanconi-Bickel syndrome, respectively, are not yet classified due to the reduced number of cases published so far. The panel can be exported and used for selecting genes to be analyzed.

5. Genetic and Phenotypic Heterogeneity Complicate Genetic Analysis

Genetic heterogeneity and variations in phenotype are probably the biggest challenges in the genetic diagnosis of renal tubulopathies, and this is illustrated by Table 1 containing the genes associated with inherited tubulopathies and the corresponding phenotypes described for each gene.
Table 1. Genes associated with inherited tubulopathies.
Fanconi renotubular syndrome (FRTS) is one of the best examples of genetic heterogeneity and phenotype variation. The renal Fanconi syndrome may be inherited or secondary to nephrotoxic substances, autoimmune diseases, or cancer [43]. Four entities have been clustered so far under the name of renal Fanconi syndrome, three autosomal dominant and one autosomal recessive [44,45]. The renal phenotype is the result of impaired reabsorption in the proximal tubule, resulting in loss of water, phosphate, glucose, bicarbonate (HCO3-), uric acid, aminoacids, and low molecular weight proteins [43]. The patients present with polyuria and polydipsia, impaired growth, rickets and osteopenia; in time, they may develop renal insufficiency [43,46]. Three forms (FRTS1, FRTS3, and FRTS4) are validated and follow an autosomal dominant (AD) inheritance pattern while the fourth (FRTS2), which is autosomal recessive, is still debated due to the limited number of cases and insufficient experimental evidence. In addition, a number of other multisystemic, metabolic inherited disorders may associate with renal Fanconi syndrome: cystinosis, galactosemia, hereditary fructose intolerance, tyrosinemia, Wilson disease, and mitochondrial diseases, reviewed in [43,47]. This heterogeneity adds to the fact that sometimes the full clinical picture develops in time, thus delaying appropriate management and increasing the risk of renal failure [48]. Therefore, the early diagnosis is a challenge for the clinician and requires a broad molecular investigation.
FRTS1 was initially linked to a different location at 15q15.3 by Lichter-Konecki et al. [50], but the gene could be identified only after re-analysis of the data extending the region to include the flanking markers and thus the GATM gene [27]. The mutations impair mitochondrial clearance by generating long polymers that prevent mitochondrial fission and degradation [27] in the renal proximal tubules. GATM encodes for L-arginine:glycine amidino-transferase, an enzyme whose gene product was originally isolated from pig kidney mitochondria [51]. Interestingly, biallelic nonsense mutations had been described as the cause for cerebral creatine deficiency syndrome 3 (OMIM# 612718) with autosomal recessive inheritance [52,53] and without any documented renal phenotype.
FRTS3 is caused by monoallelic mutations in the EHHADH gene (enoyl-CoA hydratase/3-hydroxyacyl CoA dehydrogenase), an enzyme involved in peroxisomal oxidation of fatty acids [49]. The phenotype had been described in 1955 by Luder at al. [54] and Tolaymat et al. [55] and it is reviewed in [47].
FRTS4 [56] has been identified by Hamilton et al.; in patients displaying both features of mature onset diabetes of young (MODY) and proximal renal tubulopathy associating nephrocalcinosis, hypercalciuria and hypermagnesemia, hypocalcemia, and renal impairment. The neonates with this condition have hyperinsulinism and increased birth weight.
More controversies surround the association between mutations in SLC34A1 and autosomal recessive FRTS, type 2 [45]. A biallelic in-frame duplication of 21 bp found in two children from a consanguineous family leads to complete loss of function due to a defective membrane localisation of the mutated protein [45]. No further cases have been published and thus OMIM considered this gene-phenotype association as provisional, in concordance with PanelApp [42], which maintains this association in the “Red” zone. SLC34A1 encodes for the NaPiIIa transporter which contributes by about 70–80% of the apical influx of sodium and phosphate, thus being the major effector of phosphate reabsorption in the kidney [57]. Phosphate is mostly reabsorbed in the proximal tubule, and there is no known secretion along the tubule. Reduced systemic phosphate determines adaptive changes with suppression of FGF23 (Fibroblast Growth Factor 23), increased 1-alpha hydroxylation of vitamin D, and suppressed PTH, mobilisation of calcium and phosphate from bones and increased calcium deposits in kidneys (nephrocalcinosis). Mutations in SLC34A1 are also causal for AR infantile hypercalcemia [58,59,60], with many cases reported in the literature. Conversely, it was proposed by some [35,61,62,63] and contested by others [64,65,66] that monoallelic mutations in the same gene determine AD hypophosphatemia and nephrocalcinosis, particularly in association with environmental factors. A dominant negative effect of heterozygous NaPiIIa mutations could not be demonstrated and phosphate transport has been mildly affected in some of the experiments [64,66]. In all cases, the proposed disease mechanism is a classical loss-of-function, with mostly point mutations (missense, splicing, nonsense, frameshift) identified. Two mutations, p.(I456N) and p.(R512C), were shown to impair trafficking to the membrane [63]. SLC34A1 deficiency seems to have a higher impact at earlier ages, while in adulthood the phenotype becomes milder [57]. SLC34A1 mutations have been found in five cases of infantile hypercalcemia of a total of 410 children with tubulopathies underlining the rarity of this condition [7]. A similar study focusing on 1033 adult patients identified only two patients with renal hypophosphatemia and heterozygous variants in SLC34A1 [6]. It is accepted that SlC34A1 is characterised by an increased number of single allele non-synonymous variants in the general population, with increased predisposition to developing kidney stones [67,68] and chronic kidney disease [69,70].
SLC34A3 (Solute Carrier Family 34 Member 3) is another member of the SLC34 gene family expressed in the proximal tubule which contributes less to phosphate reabsorption and has been associated with AR hypophosphatemic rickets with hypercalciuria (HHRH) [71,72]. In this case, both recessive and dominant inheritance are largely accepted, following the discovery that heterozygotes have been seen in a number of cases with hypercalciuria and kidney stones but without bone disease and with inconsistent hypophosphatemia [73]. One of the mutations, p.(Ser192Leu), is more frequent among Europeans and associated with a less severe renal and osseous phenotype in homozygous form [74] and with increased predisposition to renal calcification (NL/NC) when heterozygous [68,75]. Experimental studies demonstrated a reduced phosphate transport function of the mutant channel in different cellular systems (Xenopus oocytes and Human embryonic kidney cells, HEK293) and the high frequency in gnomAD database (99 alleles out of a total of 214,524; 88 of 91,194 alleles in Europeans) interpreted in the context of a milder phenotype [74]. Similar experiments were not able to support any evidence of functional impairment in monoallelic cases [74]. Both transporter proteins may adjust their cell surface expression in accordance with hormonal factors and phosphate intake [76]. Missense mutations can prevent proper localisation of the protein at the membrane [77]. Carriers of some SLC34A3 mutations may present with hypercalciuria [71], but a functional study of two carriers in a family of a HHRH patient showed no biochemical abnormality [77]. In fact, both SLC34A1 and SLC34A3 are known to harbor a large number of monoallelic variants, as shown by control populational databases [57].
Another gene involved in phosphate reabsorption is SLC20A2 (Solute Carrier Family 20 Member 2), but, unlike the SLC34A1 and SLC34A3, it is expressed ubiquitously and the associated phenotype involves brain calcifications but no renal features [78]. XPR1 is a gene presumed to be expressed in the basolateral membrane, where it might export phosphate into the blood stream [79]. There is no renal disease associated with mutations in this gene, despite the kidney being one of the organs with higher expression; instead, several missense mutations have been reported to cause a form of basal ganglia calcification [80]. Although no pathogenic variants associated with a renal phenotype have been identified in humans, the mouse in which Xpr1 gene had been conditionally inactivated exhibited a clear picture of renal tubular dysfunction [81]. A better understanding of these genes and more detailed experimental studies may shed light on the intricate physiology of the proximal tubule.

6. Mutations outside the Known Pattern for the Condition

Variation in some genes like SLC5A2, AQP2, KLHL3, SLC4A1, or SLC2A9 may follow either an autosomal recessive or autosomal dominant pattern, with one of these being the rule while the other is occasionally seen. The disease mechanism might differ between AD and AR even for those cases where the phenotype is similar [82]. This is not unique to tubulopathies and raises a challenge for the clinical interpretation of new variants that are not yet experimentally proven to be pathogenic. Experiments with either heterozygous, homozygous, or compound heterozygous knock-in models may orient the interpretation, and the new genome-editing technologies and organoid models are expected to clarify many of the questions we still have today [83]. In most cases, the disease mechanism is of loss-of-function in both AD and AR cases but also gain-of-function is seen in some of the AD conditions [82]. Thus, autosomal dominant SLC5A2 is caused by a reduced transport function, to about 70% of the wild-type level [84]. Variants in KLHL3 cause Pseudohypoaldosteronism type IID in either monoallelic (AD) or biallelic (AR) combinations. The difference is that the variants causing AD disease are clustered at intra- or intermolecular interaction sites, impeding functional interactions [85]. AD NDI-causing AQP2 mutations are located towards the C-terminal end and exert a dominant-negative effect [86]. The same clustering and disease mechanism is seen in SLC4A1 [87], while a loss-of-function mechanism has been found for SLC2A9 [88].
Deep intronic mutations may escape detection, unless suspected and investigated separately or within a more general, whole-genome approach. They have been cited in SLC34A3 [89,90], or SLC12A3 [91,92]. Since targeted panel sequencing is the commonest approach, these rare cases might be missed unless supplementary tests are performed. Regularly, the introns are considered the less conserved parts of a gene, where most variations may accumulate without significant consequences, unless they change one of the critical regions, the canonical donor and acceptor sites or the branch site. However, occasionally, some of these variants disrupt regulatory regions or other genes, introduce a new, ectopic splice site, resulting in an insertion of a new sequence (pseudo-exon) that can be in-frame or shift the reading frame and ultimately lead to insertion of a premature stop codon [93]. Deep intronic mutations are reported in more than 77 disease-associated genes [93]. The SLC5A2 gene encodes for the major sodium-glucose cotransporter in the kidney [94]. Monoallelic and biallelic mutations are responsible for isolated renal glycosuria [95,96,97]. Besides several missense and truncating mutations, an intronic variant consisting of a deletion of 20 nucleotides between −10 and −31, presumably affecting the branching site, has been published [98]. As whole genome sequencing becomes more cost-efficient and broadly used, it is expected that the number of reported mutations in this category will increase.
Occasionally, a tubulopathy gene may be affected as part of a contiguous gene deletion and lead to a syndromic presentation. An example is a deletion comprising SLC34A1 and NSD1 determining the association of severe hypophosphatemia to Sotos syndrome [99]. Therefore, once any sign of renal tubular impairment is seen in a patient, it is worth exploring potential additional causes as this can be critical for disease management and genetic counselling in the family.
A recent international survey identified 6 out of 36 patients with no clear causative variant in any of the known dRTA genes as being heterozygous for the variant ATP6V1B1: c.1181G>T, p.(Arg394Gln). Since the second pathogenic variant has not been identified in these cases [100] as well as others [7,101], it has been suggested that this mutation might be an example of autosomal dominant inheritance, but this still needs experimental proof.
A heterozygous mutation (c.265G>A; p.(A89T)) added glycosuria to the phenotype of an otherwise unrelated disease, juvenile cataract with microcornea, caused by monoallelic SLC16A12 mutations. Because SLC16A12 was found to be also expressed in the kidney, the association had been initially reported as a new syndrome [102,103]. Further segregation studies demonstrated that glucosuria was a separate phenotype [104]. Thus, a broader genetic investigation in the case of an unusual presentation of a disorder is more appropriate to clarify the diagnosis and guide management and family counselling as the occurrence of two independent genetic disorders, however exceptional, must not be disregarded.

7. Digenic Inheritance

Mutations in more than one gene may exceptionally be associated with an unusual phenotype [105]. With replacement of single gene sequencing by whole exome or whole genome sequencing, it is likely that many more such cases will surface where pathogenic variants are found in two or more genes, suggesting the so-called digenic or oligogenic inheritance. One question that might be asked in such situations is whether this is a true digenic effect [106] or the second gene bears a mutation only by chance. In diseases with variable phenotype like renal tubulopathies, this is more difficult to assess. It is known that some genes are more tolerant to non-synonymous variation [107]. A number of renal transporters can be included in this category: SLC34A1 is already a famous example, acknowledged by many publications and the allelic frequency in populational databases.
According to the cases reported so far in tubulopathies and in other conditions, several situations can be recognized: (1) two genes causing similar phenotypes are mutated simultaneously according to the recognised individual pattern and generate a more severe or variable phenotype [108]; (2) two genes from the same pathway and with known functional and/or physical overlap suffer from inactivating mutations with a different phenotype [109]; and (3) variants in two or more genes, inconsistent with the pattern of inheritance characteristic for the disease [110,111].
Bartter and Gitelman syndromes are the commonest renal tubulopathies [5,112]. Clinical and biochemical characteristics are detailed here [5]. There are five main forms of Bartter syndrome, each with an independent genetic cause and a subset of characteristic biochemical features [5]. Clinical presentation is not always suggestive and may not be similar in all affected members in a family. Expert consensus guidelines [112] have been drawn up to guide efficient genetic testing in GS patients. One interesting and challenging aspect is the number of digenic inheritance reports following the initial case of Bartter syndrome and deafness caused by inactivating biallelic mutations in both CLCNKA and CLCNKB [109,113]. The patient presented with a similar phenotype to Bartter syndrome 4A, known to be caused by mutations in BSND [114]. More recently, next-generation sequencing results suggested more cases of digenic inheritance in Bartter and Gitelman syndromes, one of which involves monoallelic variants in CLCNKB and SLC12A3 genes [111]. There is no demonstrated dominant negative effect of a heterozygous CLCNKB or SLC12A3 mutation and no experiment has proven that in heterozygous state these variants would have any effect at all on protein stability, trafficking, or transport function. Carrier relatives of patients with either CLCNKB or SLC12A3 associated Gitelman syndrome are healthy. The two chloride channels, CLCNKA and CLCNKB, are known to interact and to be co-expressed in certain parts of the nephron and internal ear. They both require BSND for stability and membrane localisation [115]. In the ascending loop of Henle, CLCNKA is less expressed, which means that inactivating mutations in CLCNKB result in salt loss and impaired mineral homeostasis as a result of reduced chloride export from the renal tubule cells [116,117]. Through inactivating mutations of both genes, there is a severe loss of saline transport associated with hearing loss due to defective formation of endolymph [113]. This phenotype is similar to that generated by mutations in BSND, thus illustrating the interdependence of the three genes [114]. Interestingly, only homozygous inactivating mutations in each of the two chloride channels, CLCNKA and CLCNKB, have been associated with deafness, perfectly overlapping with the definition of true digenic effects. Digenic inheritance requires a demonstrable interaction between the two genes, a clear consistence across a larger pedigree or multiple pedigrees [105], which could be proven for Bartter syndrome 4B but would be less convincing in other cases. Exome and genome sequencing result in a larger number of potentially damaging variants, which make them more demanding in terms of analysis and interpretation. Similar results have been reported in dRTA [118].
A patient with Dent 2 disease was found to have mutations in both CLCN5 and OCRL genes, and an intermediary phenotype between DD and LS [108], while another case with OCRL and INPP5B variants presented with a Chiari I malformation [119].
Given the number of non-synonymous mutation in the genes encoding for transporter proteins, it is very likely that pathogenic mutations can be present independently in more than one gene thus requiring a thorough experimental, genetic, and physiological investigation before supporting a non-canonical inheritance pattern. Interestingly, some of the genes associated with Mendelian diseases are also the site of relatively rare variants that confer increased susceptibility to common forms of renal diseases (nephrolithiasis, chronic kidney disease) [120,121,122].
While the occurrence of damaging variants in two or more genes in one individual is not impossible, we can suggest that these cases must be validated experimentally before being used to manage and counsel patients and families.

8. Conclusions

Next-generation sequencing has the potential to speed up gene discovery and thus improve management of patients with inherited tubulopathies through a more precise molecular diagnosis. One effect of the technology can be generation of a large list of variants of unknown significance that can lead to overinterpretation and false diagnostic association, unless stringent criteria are applied to classify and interpret them.

Author Contributions

D.I. drafted the manuscript; E.A. supervised and amended the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by the European Union, FP7 (grant agreement 2012-305608 “European Consortium for High-Throughput Research in Rare Kidney Diseases (EURenOmics)” and by the British Kidney Patient Association.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Biesecker, L.G.; Green, R.C. Diagnostic clinical genome and exome sequencing. N. Engl. J. Med. 2014, 370, 2418–2425. [Google Scholar] [CrossRef] [PubMed]
  2. Goldstein, D.B.; Allen, A.; Keebler, J.; Margulies, E.H.; Petrou, S.; Petrovski, S.; Sunyaev, S. Sequencing studies in human genetics: Design and interpretation. Nat. Rev. Genet. 2013, 14, 460–470. [Google Scholar] [CrossRef] [PubMed]
  3. Groopman, E.E.; Gharavi, A.G. Expanding opportunities and emerging challenges: Broadening the scope of genetic testing in nephrology. Kidney Int. 2019, 95, 743–746. [Google Scholar] [CrossRef] [PubMed]
  4. Yu, J.H.; Appelbaum, P.S.; Brothers, K.B.; Joffe, S.; Kauffman, T.L.; Koenig, B.A.; Prince, A.E.; Scollon, S.; Wolf, S.M.; Bernhardt, B.A.; et al. Consent for clinical genome sequencing: Considerations from the Clinical Sequencing Exploratory Research Consortium. PerMed 2019, 16, 325–333. [Google Scholar] [CrossRef] [PubMed]
  5. Walsh, P.R.; Tse, Y.; Ashton, E.; Iancu, D.; Jenkins, L.; Bienias, M.; Kleta, R.; Hoff, W.V.; Bockenhauer, D. Clinical and diagnostic features of Bartter and Gitelman syndromes. Clin. Kidney J. 2017, 11, 302–309. [Google Scholar] [CrossRef] [PubMed]
  6. Hureaux, M.; Ashton, E.; Dahan, K.; Houillier, P.; Blanchard, A.; Cormier, C.; Koumakis, E.; Iancu, D.; Belge, H.; Hilbert, P.; et al. High-throughput sequencing contributes to the diagnosis of tubulopathies and familial hypercalcemia hypocalciuria in adults. Kidney Int. 2019, 96, 1408–1416. [Google Scholar] [CrossRef]
  7. Ashton, E.J.; Legrand, A.; Benoit, V.; Roncelin, I.; Venisse, A.; Zennaro, M.-C.; Jeunemaitre, X.; Iancu, D.; Hoff, W.G.v.; Walsh, S.B.; et al. Simultaneous sequencing of 37 genes identified causative mutations in the majority of children with renal tubulopathies. Kidney Int. 2018, 93, 961–967. [Google Scholar] [CrossRef]
  8. Sanger, F.; Nicklen, S.; Coulson, A.R. DNA sequencing with chain-terminating inhibitors. Proc. Natl. Acad. Sci. USA 1977, 74, 5463–5467. [Google Scholar] [CrossRef]
  9. Grishkevich, V.; Yanai, I. Gene length and expression level shape genomic novelties. Genome Res. 2014, 24, 1497–1503. [Google Scholar] [CrossRef]
  10. Groopman, E.E.; Rasouly, H.M.; Gharavi, A.G. Genomic medicine for kidney disease. Nat. Rev. Nephrol. 2018, 14, 83–104. [Google Scholar] [CrossRef]
  11. Daga, A.; Majmundar, A.J.; Braun, D.A.; Gee, H.Y.; Lawson, J.A.; Shril, S.; Jobst-Schwan, T.; Vivante, A.; Schapiro, D.; Tan, W.; et al. Whole exome sequencing frequently detects a monogenic cause in early onset nephrolithiasis and nephrocalcinosis. Kidney Int. 2018, 93, 204–213. [Google Scholar] [CrossRef] [PubMed]
  12. LaDuca, H.; Farwell, K.D.; Vuong, H.; Lu, H.M.; Mu, W.; Shahmirzadi, L.; Tang, S.; Chen, J.; Bhide, S.; Chao, E.C. Exome sequencing covers >98% of mutations identified on targeted next generation sequencing panels. PLoS ONE 2017, 12, e0170843. [Google Scholar] [CrossRef]
  13. McPherson, J.D. Next-generation gap. Nat. Methods 2009, 6, S2–S5. [Google Scholar] [CrossRef]
  14. Lyon, G.J.; Wang, K. Identifying disease mutations in genomic medicine settings: Current challenges and how to accelerate progress. Genome Med. 2012, 4, 58. [Google Scholar] [CrossRef]
  15. Quintáns, B.; Ordóñez-Ugalde, A.; Cacheiro, P.; Carracedo, A.; Sobrido, M. Medical genomics: The intricate path from genetic variant identification to clinical interpretation. Appl. Transl. Genom. 2014, 3, 60–67. [Google Scholar] [CrossRef] [PubMed]
  16. Richards, S.; Aziz, N.; Bale, S.; Bick, D.; Das, S.; Gastier-Foster, J.; Grody, W.W.; Hegde, M.; Lyon, E.; Spector, E. Standards and guidelines for the interpretation of sequence variants: A joint consensus recommendation of the American College of Medical Genetics and Genomics and the Association for Molecular Pathology. Genet. Med. 2015, 17, 405. [Google Scholar] [CrossRef] [PubMed]
  17. Amendola, L.M.; Jarvik, G.P.; Leo, M.C.; McLaughlin, H.M.; Akkari, Y.; Amaral, M.D.; Berg, J.S.; Biswas, S.; Bowling, K.M.; Conlin, L.K. Performance of ACMG-AMP variant-interpretation guidelines among nine laboratories in the Clinical Sequencing Exploratory Research Consortium. Am. J. Hum. Genet. 2016, 98, 1067–1076. [Google Scholar] [CrossRef] [PubMed]
  18. Strande, N.T.; Brnich, S.E.; Roman, T.S.; Berg, J.S. Navigating the nuances of clinical sequence variant interpretation in Mendelian disease. Genet. Med. 2018, 20, 918–926. [Google Scholar] [CrossRef]
  19. Harrison, S.M.; Dolinsky, J.S.; Johnson, A.E.K.; Pesaran, T.; Azzariti, D.R.; Bale, S.; Chao, E.C.; Das, S.; Vincent, L.; Rehm, H.L. Clinical laboratories collaborate to resolve differences in variant interpretations submitted to ClinVar. Genet. Med. 2017, 19, 1096–1104. [Google Scholar] [CrossRef] [PubMed]
  20. Kim, Y.E.; Ki, C.S.; Jang, M.A. Challenges and Considerations in Sequence Variant Interpretation for Mendelian Disorders. Ann. Lab. Med. 2019, 39, 421–429. [Google Scholar] [CrossRef]
  21. Tarailo-Graovac, M.; Zhu, J.Y.A.; Matthews, A.; van Karnebeek, C.D.M.; Wasserman, W.W. Assessment of the ExAC data set for the presence of individuals with pathogenic genotypes implicated in severe Mendelian pediatric disorders. Genet. Med. 2017, 19, 1300–1308. [Google Scholar] [CrossRef] [PubMed]
  22. Whiffin, N.; Minikel, E.; Walsh, R.; O’Donnell-Luria, A.H.; Karczewski, K.; Ing, A.Y.; Barton, P.J.R.; Funke, B.; Cook, S.A.; MacArthur, D.; et al. Using high-resolution variant frequencies to empower clinical genome interpretation. Genet. Med. 2017, 19, 1151–1158. [Google Scholar] [CrossRef] [PubMed]
  23. Lek, M.; Karczewski, K.J.; Minikel, E.V.; Samocha, K.E.; Banks, E.; Fennell, T.; O’Donnell-Luria, A.H.; Ware, J.S.; Hill, A.J.; Cummingset, B.B.; et al. Analysis of protein-coding genetic variation in 60,706 humans. Nature 2016, 536, 285. [Google Scholar] [CrossRef] [PubMed]
  24. Karczewski, K.J.; Francioli, L.C.; Tiao, G.; Cummings, B.B.; Alföldi, J.; Wang, Q.; Collins, R.L.; Laricchia, K.M.; Ganna, A.; Birnbaum, D.P.; et al. Variation across 141,456 human exomes and genomes reveals the spectrum of loss-of-function intolerance across human protein-coding genes. bioRxiv 2019, 531210. [Google Scholar] [CrossRef]
  25. Walsh, R.; Thomson, K.L.; Ware, J.S.; Funke, B.H.; Woodley, J.; McGuire, K.J.; Mazzarotto, F.; Blair, E.; Seller, A.; Taylor, J.C.; et al. Reassessment of Mendelian gene pathogenicity using 7855 cardiomyopathy cases and 60,706 reference samples. Genet. Med. 2017, 19, 192–203. [Google Scholar] [CrossRef]
  26. Wagner, C.A.; Biber, J.; Murer, H. Of men and mice: Who is in control of renal phosphate reabsorption? J. Am. Soc. Nephrol. 2008, 19, 1625–1626. [Google Scholar] [CrossRef]
  27. Reichold, M.; Klootwijk, E.D.; Reinders, J.; Otto, E.A.; Milani, M.; Broeker, C.; Laing, C.; Wiesner, J.; Devi, S.; Zhou, W.; et al. Glycine Amidinotransferase (GATM), Renal Fanconi Syndrome, and Kidney Failure. J. Am. Soc. Nephrol. 2018, 29, 1849–1858. [Google Scholar] [CrossRef]
  28. López-Cayuqueo, K.I.; Chavez-Canales, M.; Pillot, A.; Houillier, P.; Jayat, M.; Baraka-Vidot, J.; Trepiccione, F.; Baudrie, V.; Büsst, C.; Soukaseum, C.; et al. A mouse model of pseudohypoaldosteronism type II reveals a novel mechanism of renal tubular acidosis. Kidney Int. 2018, 94, 514–523. [Google Scholar] [CrossRef]
  29. Beck, L.; Karaplis, A.C.; Amizuka, N.; Hewson, A.S.; Ozawa, H.; Tenenhouse, H.S. Targeted inactivation of Npt2 in mice leads to severe renal phosphate wasting, hypercalciuria, and skeletal abnormalities. Proc. Natl. Acad. Sci. USA 1998, 95, 5372–5377. [Google Scholar] [CrossRef]
  30. Iwaki, T.; Sandoval-Cooper, M.J.; Tenenhouse, H.S.; Castellino, F.J. A missense mutation in the sodium phosphate co-transporter Slc34a1 impairs phosphate homeostasis. J. Am. Soc. Nephrol. 2008, 19, 1753–1762. [Google Scholar] [CrossRef]
  31. Chau, H.; El-Maadawy, S.; McKee, M.D.; Tenenhouse, H.S. Renal calcification in mice homozygous for the disrupted type IIa Na/Pi cotransporter gene Npt2. J. Bone Miner Res. 2003, 18, 644–657. [Google Scholar] [CrossRef] [PubMed]
  32. Inoue, K.; Balkin, D.M.; Liu, L.; Nandez, R.; Wu, Y.; Tian, X.; Wang, T.; Nussbaum, R.; de Camilli, P.; Ishibe, S. Kidney Tubular Ablation of Ocrl/Inpp5b Phenocopies Lowe Syndrome Tubulopathy. J. Am. Soc. Nephrol. 2017, 28, 1399–1407. [Google Scholar] [CrossRef] [PubMed]
  33. Oltrabella, F.; Pietka, G.; Ramirez, I.B.; Mironov, A.; Starborg, T.; Drummond, I.A.; Hinchliffe, K.A.; Lowe, M. The Lowe syndrome protein OCRL1 is required for endocytosis in the zebrafish pronephric tubule. PLoS Genet. 2015, 11, e1005058. [Google Scholar] [CrossRef] [PubMed]
  34. Dawson, P.A.; Russell, C.S.; Lee, S.; McLeay, S.C.; van Dongen, J.M.; Cowley, D.M.; Clarke, L.A.; Markovich, D. Urolithiasis and hepatotoxicity are linked to the anion transporter Sat1 in mice. J. Clin. Investig. 2010, 120, 706–712. [Google Scholar] [CrossRef]
  35. Amar, A.; Majmundar, A.J.; Ullah, I.; Afzal, A.; Braun, D.A.; Shril, S.; Daga, A.; Jobst-Schwan, T.; Ahmad, M.; Sayeret, J.A.; et al. Gene panel sequencing identifies a likely monogenic cause in 7% of 235 Pakistani families with nephrolithiasis. Hum. Genet. 2019, 138, 211–219. [Google Scholar] [CrossRef]
  36. Braun, D.A.; Lawson, J.A.; Gee, H.Y.; Halbritter, J.; Shril, S.; Tan, W.; Stein, D.; Wassner, A.J.; Ferguson, M.A.; Gucev, Z. Prevalence of monogenic causes in pediatric patients with nephrolithiasis or nephrocalcinosis. Clin. J. Am. Soc. Nephrol. 2016, 11, 664–672. [Google Scholar] [CrossRef]
  37. Halbritter, J.; Baum, M.; Hynes, A.M.; Rice, S.J.; Thwaites, D.T.; Gucev, Z.S.; Fisher, B.; Spaneas, L.; Porath, J.D.; Braun, D.A.; et al. Fourteen monogenic genes account for 15% of nephrolithiasis/nephrocalcinosis. J. Am. Soc. Nephrol. 2015, 26, 543–551. [Google Scholar] [CrossRef]
  38. Besouw, M.T.P.; Bienias, M.; Walsh, P.; Kleta, R.; Hoff, W.G.V.; Ashton, E.; Jenkins, L.; Bockenhauer, D. Clinical and molecular aspects of distal renal tubular acidosis in children. Pediatric Nephrol. 2017, 32, 987–996. [Google Scholar] [CrossRef]
  39. Blanchard, A.; Curis, E.; Guyon-Roger, T.; Kahila, D.; Treard, C.; Baudouin, V.; Bérard, E.; Champion, G.; Cochat, P.; Dubourg, J.; et al. Observations of a large Dent disease cohort. Kidney Int. 2016, 90, 430–439. [Google Scholar] [CrossRef]
  40. Sekine, T.; Komoda, F.; Miura, K.; Takita, J.; Shimadzu, M.; Matsuyama, T.; Ashida, A.; Igarashi, T. Japanese Dent disease has a wider clinical spectrum than Dent disease in Europe/USA: Genetic and clinical studies of 86 unrelated patients with low-molecular-weight proteinuria. Nephrol. Dial. Transpl. 2014, 29, 376–384. [Google Scholar] [CrossRef]
  41. Ma, J.; Ren, H.; Lin, L.; Zhang, C.; Wang, Z.; Xie, J.; Shen, P.; Zhang, W.; Wang, W.; Chen, X.; et al. Genetic Features of Chinese Patients with Gitelman Syndrome: Sixteen Novel SLC12A3 Mutations Identified in a New Cohort. Am. J. Nephrol. 2016, 44, 113–121. [Google Scholar] [CrossRef] [PubMed]
  42. Martin, A.R.; Williams, E.; Foulger, R.E.; Leigh, S.; Daugherty, L.C.; Niblock, O.; Leong, I.U.S.; Smith, K.R.; Gerasimenko, O.; Haraldsdottir, E.; et al. PanelApp crowdsources expert knowledge to establish consensus diagnostic gene panels. Nat. Genet. 2019, 51, 1560–1565. [Google Scholar] [CrossRef] [PubMed]
  43. Wijst, J.V.D.; Belge, H.; Bindels, R.J.M.; Devuyst, O. Learning Physiology from Inherited Kidney Disorders. Physiol. Rev. 2019, 99, 1575–1653. [Google Scholar] [CrossRef] [PubMed]
  44. Klootwijk, E.D.; Reichold, M.; Unwin, R.J.; Kleta, R.; Warth, R.; Bockenhauer, D. Renal Fanconi syndrome: Taking a proximal look at the nephron. Nephrol. Dial. Transpl. 2015, 30, 1456–1460. [Google Scholar] [CrossRef] [PubMed]
  45. Magen, D.; Berger, L.; Coady, M.J.; Ilivitzki, A.; Militianu, D.; Tieder, M.; Selig, S.; Lapointe, J.Y.; Zelikovic, I.; Skorecki, K. A loss-of-function mutation in NaPi-IIa and renal Fanconi’s syndrome. N. Engl. J. Med. 2010, 362, 1102–1109. [Google Scholar] [CrossRef]
  46. Bokenkamp, A.; Ludwig, M. Disorders of the renal proximal tubule. Nephron Physiol. 2011, 118, 1–6. [Google Scholar] [CrossRef]
  47. Klootwijk, E.; Dufek, S.; Issler, N.; Bockenhauer, D.; Kleta, R. Pathophysiology, current treatments and future targets in hereditary forms of renal Fanconi syndrome. Expert Opin. Orphan Drugs 2017, 5, 45–54. [Google Scholar] [CrossRef][Green Version]
  48. Connaughton, D.M.; Kennedy, C.; Shril, S.; Mann, N.; Murray, S.L.; Williams, P.A.; Conlon, E.; Nakayama, M.; van der Ven, A.T.; Ityel, H.; et al. Monogenic causes of chronic kidney disease in adults. Kidney Int. 2019, 95, 914–928. [Google Scholar] [CrossRef]
  49. Klootwijk, E.D.; Reichold, M.; Helip-Wooley, A.; Tolaymat, A.; Broeker, C.; Robinette, S.L.; Reinders, J.; Peindl, D.; Renner, K.; Eberhart, K.; et al. Mistargeting of peroxisomal EHHADH and inherited renal Fanconi’s syndrome. N. Engl. J. Med. 2014, 370, 129–138. [Google Scholar] [CrossRef]
  50. Lichter-Konecki, U.; Broman, K.W.; Blau, E.B.; Konecki, D.S. Genetic and physical mapping of the locus for autosomal dominant renal Fanconi syndrome, on chromosome 15q15.3. Am. J. Hum. Genet. 2001, 68, 264–268. [Google Scholar] [CrossRef]
  51. Humm, A.; Huber, R.; Mann, K. The amino acid sequences of human and pig L-arginine:glycine amidinotransferase. FEBS Lett. 1994, 339, 101–107. [Google Scholar] [CrossRef]
  52. Bianchi, M.C.; Tosetti, M.; Fornai, F.; Alessandri, M.G.; Cipriani, P.; de Vito, G.; Canapicchi, R. Reversible brain creatine deficiency in two sisters with normal blood creatine level. Ann. Neurol. 2000, 47, 511–513. [Google Scholar] [CrossRef]
  53. Item, C.B.; Stockler-Ipsiroglu, S.; Stromberger, C.; Muhl, A.; Alessandri, M.G.; Bianchi, M.C.; Tosetti, M.; Fornai, F.; Cioni, G. Arginine:glycine amidinotransferase deficiency: The third inborn error of creatine metabolism in humans. Am. J. Hum. Genet. 2001, 69, 1127–1133. [Google Scholar] [CrossRef] [PubMed]
  54. Luder, J.; Sheldon, W. A familial tubular absorption defect of glucose and amino-acids. Arch. Dis. Child. 1955, 30, 160. [Google Scholar] [CrossRef] [PubMed]
  55. Tolaymat, A.; Sakarcan, A.; Neiberger, R. Idiopathic Fanconi syndrome in a family. Part I. Clinical aspects. J. Am. Soc. Nephrol. 1992, 2, 1310–1317. [Google Scholar] [PubMed]
  56. Hamilton, A.J.; Bingham, C.; McDonald, T.J.; Cook, P.R.; Caswell, R.C.; Weedon, M.N.; Oram, R.A.; Shields, B.M.; Shepherd, M.; Inward, C.D.; et al. The HNF4A R76W mutation causes atypical dominant Fanconi syndrome in addition to a β cell phenotype. J. Med. Genet. 2014, 51, 165–169. [Google Scholar] [CrossRef]
  57. Wagner, C.A.; Rubio-Aliaga, I.; Hernando, N. Renal phosphate handling and inherited disorders of phosphate reabsorption: An update. Pediatr. Nephrol. 2019, 34, 549–559. [Google Scholar] [CrossRef]
  58. Pronicka, E.; Ciara, E.; Halat, P.; Janiec, A.; Wojcik, M.; Rowinska, E.; Rokicki, D.; Pludowski, P.; Wojciechowska, E.; Wierzbicka, A.; et al. Biallelic mutations in CYP24A1 or SLC34A1 as a cause of infantile idiopathic hypercalcemia (IIH) with vitamin D hypersensitivity: Molecular study of 11 historical IIH cases. J. Appl. Genet. 2017, 58, 349–353. [Google Scholar] [CrossRef]
  59. Schlingmann, K.P.; Ruminska, J.; Kaufmann, M.; Dursun, I.; Patti, M.; Kranz, B.; Pronicka, E.; Ciara, E.; Akcay, T.; Bulus, D.; et al. Autosomal-Recessive Mutations in SLC34A1 Encoding Sodium-Phosphate Cotransporter 2A Cause Idiopathic Infantile Hypercalcemia. J. Am. Soc. Nephrol. 2016, 27, 604–614. [Google Scholar] [CrossRef]
  60. De Paolis, E.; Scaglione, G.L.; de Bonis, M.; Minucci, A.; Capoluongo, E. CYP24A1 and SLC34A1 genetic defects associated with idiopathic infantile hypercalcemia: From genotype to phenotype. Clin. Chem. Lab. Med. 2019, 57, 1650–1667. [Google Scholar] [CrossRef]
  61. Chen, X.; Xie, Y.; Wan, S.; Xu, J.; Cai, B.; Zhang, Y.; Yu, X. A novel heterozygous mutation c.680A>G (p. N227S) in SLC34A1 gene leading to autosomal dominant hypophosphatemia: A case report. Medicine 2019, 98, e15617. [Google Scholar] [CrossRef] [PubMed]
  62. Prié, D.; Huart, V.; Bakouh, N.; Planelles, G.; Dellis, O.; Gérard, B.; Hulin, P.; Benqué-Blanchet, F.; Silve, C.; Grandchamp, B.; et al. Nephrolithiasis and osteoporosis associated with hypophosphatemia caused by mutations in the type 2a sodium-phosphate cotransporter. N. Engl. J. Med. 2002, 347, 983–991. [Google Scholar]
  63. Fearn, A.; Allison, B.; Rice, S.J.; Edwards, N.; Halbritter, J.; Bourgeois, S.; Pastor-Arroyo, E.M.; Hildebrandt, F.; Tasic, V.; Wagner, C.A.; et al. Clinical, biochemical, and pathophysiological analysis of SLC34A1 mutations. Physiol. Rep. 2018, 6, e13715. [Google Scholar] [CrossRef] [PubMed]
  64. Lederer, E.; Wagner, C.A. Clinical aspects of the phosphate transporters NaPi-IIa and NaPi-IIb: Mutations and disease associations. PFLUG Arch. 2019, 471, 137–148. [Google Scholar] [CrossRef] [PubMed]
  65. Lapointe, J.Y.; Tessier, J.; Paquette, Y.; Wallendorff, B.; Coady, M.J.; Pichette, V.; Bonnardeaux, A. NPT2a gene variation in calcium nephrolithiasis with renal phosphate leak. Kidney Int. 2006, 69, 2261–2267. [Google Scholar] [CrossRef]
  66. Virkki, L.V.; Forster, I.C.; Hernando, N.; Biber, J.; Murer, H. Functional characterization of two naturally occurring mutations in the human sodium-phosphate cotransporter type IIa. J. Bone Min. Res. 2003, 18, 2135–2141. [Google Scholar] [CrossRef]
  67. Arcidiacono, T.; Mingione, A.; Macrina, L.; Pivari, F.; Soldati, L.; Vezzoli, G. Idiopathic calcium nephrolithiasis: A review of pathogenic mechanisms in the light of genetic studies. Am. J. Nephrol. 2014, 40, 499–506. [Google Scholar] [CrossRef]
  68. Oddsson, A.; Sulem, P.; Helgason, H.; Edvardsson, V.O.; Thorleifsson, G.; Sveinbjornsson, G.; Haraldsdottir, E.; Eyjolfsson, G.I.; Sigurdardottir, O.; Olafsson, I.; et al. Common and rare variants associated with kidney stones and biochemical traits. Nat. Commun. 2015, 6, 7975. [Google Scholar] [CrossRef]
  69. Kottgen, A.; Pattaro, C.; Boger, C.A.; Fuchsberger, C.; Olden, M.; Glazer, N.L.; Parsa, A.; Gao, X.; Yang, Q.; Smith, A.V.; et al. New loci associated with kidney function and chronic kidney disease. Nat. Genet. 2010, 42, 376–384. [Google Scholar] [CrossRef]
  70. Sveinbjornsson, G.; Mikaelsdottir, E.; Palsson, R.; Indridason, O.S.; Holm, H.; Jonasdottir, A.; Helgason, A.; Sigurdsson, S.; Jonasdottir, A.; Sigurdsson, A.; et al. Rare mutations associating with serum creatinine and chronic kidney disease. Hum. Mol. Genet. 2014, 23, 6935–6943. [Google Scholar] [CrossRef]
  71. Bergwitz, C.; Roslin, N.M.; Tieder, M.; Loredo-Osti, J.C.; Bastepe, M.; Abu-Zahra, H.; Frappier, D.; Burkett, K.; Carpenter, T.O.; Anderson, D.; et al. SLC34A3 mutations in patients with hereditary hypophosphatemic rickets with hypercalciuria predict a key role for the sodium-phosphate cotransporter NaPi-IIc in maintaining phosphate homeostasis. Am. J. Hum. Genet. 2006, 78, 179–192. [Google Scholar] [CrossRef] [PubMed]
  72. Lorenz-Depiereux, B.; Benet-Pages, A.; Eckstein, G.; Tenenbaum-Rakover, Y.; Wagenstaller, J.; Tiosano, D.; Gershoni-Baruch, R.; Albers, N.; Lichtner, P.; Schnabel, D.; et al. Hereditary hypophosphatemic rickets with hypercalciuria is caused by mutations in the sodium-phosphate cotransporter gene SLC34A3. Am. J. Hum. Genet. 2006, 78, 193–201. [Google Scholar] [CrossRef] [PubMed]
  73. Sayer, J.A. Progress in Understanding the Genetics of Calcium-Containing Nephrolithiasis. J. Am. Soc. Nephrol. 2017, 28, 748–759. [Google Scholar] [CrossRef] [PubMed]
  74. Schönauer, R.; Petzold, F.; Lucinescu, W.; Seidel, A.; Müller, L.; Neuber, S.; Bergmann, C.; Sayer, J.A.; Werner, A.; Halbritter, J. Evaluating pathogenicity of SLC34A3-Ser192Leu, a frequent European missense variant in disorders of renal phosphate wasting. Urolithiasis 2019, 47, 511–519. [Google Scholar] [CrossRef]
  75. Forster, I.C. The molecular mechanism of SLC34 proteins: Insights from two decades of transport assays and structure-function studies. Pflügers Archiv Eur. J. Physiol. 2019, 471, 15–42. [Google Scholar] [CrossRef]
  76. Wagner, C.A.; Hernando, N.; Forster, I.C.; Biber, J. The SLC34 family of sodium-dependent phosphate transporters. PFLUG Arch. 2014, 466, 139–153. [Google Scholar] [CrossRef]
  77. Jaureguiberry, G.; Carpenter, T.O.; Forman, S.; Juppner, H.; Bergwitz, C. A novel missense mutation in SLC34A3 that causes hereditary hypophosphatemic rickets with hypercalciuria in humans identifies threonine 137 as an important determinant of sodium-phosphate cotransport in NaPi-IIc. Am. J. Physiol. Renal Physiol. 2008, 295, F371–F379. [Google Scholar] [CrossRef]
  78. Guo, X.X.; Su, H.Z.; Zou, X.H.; Lai, L.L.; Lu, Y.Q.; Wang, C.; Li, Y.L.; Hong, J.M.; Zhao, M.; Lin, K.X.; et al. Identification of SLC20A2 deletions in patients with primary familial brain calcification. Clin. Genet. 2019, 96, 53–60. [Google Scholar] [CrossRef]
  79. Giovannini, D.; Touhami, J.; Charnet, P.; Sitbon, M.; Battini, J.-L. Inorganic Phosphate Export by the Retrovirus Receptor XPR1 in Metazoans. Cell Rep. 2013, 3, 1866–1873. [Google Scholar] [CrossRef]
  80. Legati, A.; Giovannini, D.; Nicolas, G.; Lopez-Sanchez, U.; Quintans, B.; Oliveira, J.R.; Sears, R.L.; Ramos, E.M.; Spiteri, E.; Sobrido, M.J.; et al. Mutations in XPR1 cause primary familial brain calcification associated with altered phosphate export. Nat. Genet. 2015, 47, 579–581. [Google Scholar] [CrossRef]
  81. Ansermet, C.; Moor, M.B.; Centeno, G.; Auberson, M.; Hu, D.Z.; Baron, R.; Nikolaeva, S.; Haenzi, B.; Katanaeva, N.; Gautschi, I.; et al. Renal Fanconi Syndrome and Hypophosphatemic Rickets in the Absence of Xenotropic and Polytropic Retroviral Receptor in the Nephron. J. Am. Soc. Nephrol. 2017, 28, 1073–1078. [Google Scholar] [CrossRef] [PubMed]
  82. Guo, Y.; Wei, X.; Das, J.; Grimson, A.; Lipkin, S.M.; Clark, A.G.; Yu, H. Dissecting disease inheritance modes in a three-dimensional protein network challenges the “guilt-by-association” principle. Am. J. Hum. Genet. 2013, 93, 78–89. [Google Scholar] [CrossRef] [PubMed]
  83. Islam, M.; Nishinakamura, R. How to rebuild the kidney: Recent advances in kidney organoids. J. Biochem. 2019, 166, 7–12. [Google Scholar] [CrossRef] [PubMed]
  84. Yu, L.; Lv, J.C.; Zhou, X.J.; Zhu, L.; Hou, P.; Zhang, H. Abnormal expression and dysfunction of novel SGLT2 mutations identified in familial renal glucosuria patients. Hum. Genet. 2011, 129, 335–344. [Google Scholar] [CrossRef]
  85. Boyden, L.M.; Choi, M.; Choate, K.A.; Nelson-Williams, C.J.; Farhi, A.; Toka, H.R.; Tikhonova, I.R.; Bjornson, R.; Mane, S.M.; Colussi, G.; et al. Mutations in kelch-like 3 and cullin 3 cause hypertension and electrolyte abnormalities. Nature 2012, 482, 98–102. [Google Scholar] [CrossRef]
  86. Calvanese, L.; D’Auria, G.; Vangone, A.; Falcigno, L.; Oliva, R. Structural basis for mutations of human aquaporins associated to genetic diseases. Int. J. Mol. Sci. 2018, 19, 1577. [Google Scholar] [CrossRef]
  87. Quilty, J.A.; Cordat, E.; Reithmeier, R.A. Impaired trafficking of human kidney anion exchanger (kAE1) caused by hetero-oligomer formation with a truncated mutant associated with distal renal tubular acidosis. Biochem. J. 2002, 368, 895–903. [Google Scholar] [CrossRef]
  88. Matsuo, H.; Chiba, T.; Nagamori, S.; Nakayama, A.; Domoto, H.; Phetdee, K.; Wiriyasermkul, P.; Kikuchi, Y.; Oda, T.; Nishiyama, J.; et al. Mutations in glucose transporter 9 gene SLC2A9 cause renal hypouricemia. Am. J. Hum. Genet. 2008, 83, 744–751. [Google Scholar] [CrossRef]
  89. Hasani-Ranjbar, S.; Amoli, M.M.; Ebrahim-Habibi, A.; Dehghan, E.; Soltani, A.; Amiri, P.; Larijani, B. SLC34A3 intronic deletion in a new kindred with hereditary hypophosphatemic rickets with hypercalciuria. J. Clin. Res. Pediatr. Endocrinol. 2012, 4, 89–93. [Google Scholar] [CrossRef]
  90. Ichikawa, S.; Sorenson, A.H.; Imel, E.A.; Friedman, N.E.; Gertner, J.M.; Econs, M.J. Intronic Deletions in the SLC34A3 Gene Cause Hereditary Hypophosphatemic Rickets with Hypercalciuria. J. Clin. Endocrinol. Metab. 2006, 91, 4022–4027. [Google Scholar] [CrossRef]
  91. Nozu, K.; Iijima, K.; Nozu, Y.; Ikegami, E.; Imai, T.; Fu, X.J.; Kaito, H.; Nakanishi, K.; Yoshikawa, N.; Matsuo, M. A deep intronic mutation in the SLC12A3 gene leads to Gitelman syndrome. Pediatr. Res. 2009, 66, 590–593. [Google Scholar] [CrossRef] [PubMed]
  92. Lo, Y.-F.; Nozu, K.; Iijima, K.; Morishita, T.; Huang, C.-C.; Yang, S.-S.; Sytwu, H.-K.; Fang, Y.-W.; Tseng, M.-H.; Lin, S.-H. Recurrent deep intronic mutations in the SLC12A3 gene responsible for Gitelman’s syndrome. Clin. J. Am. Soc. Nephrol. CJASN 2011, 6, 630–639. [Google Scholar] [CrossRef] [PubMed]
  93. Vaz-Drago, R.; Custódio, N.; Carmo-Fonseca, M. Deep intronic mutations and human disease. Hum. Genet. 2017, 136, 1093–1111. [Google Scholar] [CrossRef]
  94. Wells, R.G.; Pajor, A.M.; Kanai, Y.; Turk, E.; Wright, E.M.; Hediger, M.A. Cloning of a human kidney cDNA with similarity to the sodium-glucose cotransporter. Am. J. Physiol. 1992, 263, F459–F465. [Google Scholar] [CrossRef] [PubMed]
  95. Calado, J.; Soto, K.; Clemente, C.; Correia, P.; Rueff, J. Novel compound heterozygous mutations in SLC5A2 are responsible for autosomal recessive renal glucosuria. Hum. Genet. 2004, 114, 314–316. [Google Scholar] [CrossRef] [PubMed]
  96. Van den Heuvel, L.P.; Assink, K.; Willemsen, M.; Monnens, L. Autosomal recessive renal glucosuria attributable to a mutation in the sodium glucose cotransporter (SGLT2). Hum. Genet. 2002, 111, 544–547. [Google Scholar] [CrossRef] [PubMed]
  97. Ottosson-Laakso, E.; Tuomi, T.; Forsén, B.; Gullström, M.; Groop, P.-H.; Groop, L.; Vikman, P. Influence of Familial Renal Glycosuria Due to Mutations in the SLC5A2 Gene on Changes in Glucose Tolerance over Time. PLoS ONE 2016, 11, e0146114. [Google Scholar] [CrossRef]
  98. Zhao, X.; Cui, L.; Lang, Y.; Liu, T.; Lu, J.; Wang, C.; Tuffery-Giraud, S.; Bottillo, I.; Wang, X.; Shao, L. A recurrent deletion in the SLC5A2 gene including the intron 7 branch site responsible for familial renal glucosuria. Sci. Rep. 2016, 6, 33920. [Google Scholar] [CrossRef]
  99. Levtchenko, E.; Schoeber, J.; Jaeken, J. Genetic disorders of renal phosphate transport. N. Engl. J. Med. 2010, 363, 1774. [Google Scholar]
  100. Lopez-Garcia, S.C.; Emma, F.; Walsh, S.B.; Fila, M.; Hooman, N.; Zaniew, M.; Bertholet-Thomas, A.; Colussi, G.; Burgmaier, K.; Levtchenko, E.; et al. Treatment and long-term outcome in primary distal renal tubular acidosis. Nephrol. Dial. Transpl. 2019, 34, 981–991. [Google Scholar] [CrossRef]
  101. Carboni, I.; Andreucci, E.; Caruso, M.R.; Ciccone, R.; Zuffardi, O.; Genuardi, M.; Pela, I.; Giglio, S. Medullary sponge kidney associated with primary distal renal tubular acidosis and mutations of the H + -ATPase genes. Nephrol. Dial. Transpl. 2009, 24, 2734–2738. [Google Scholar] [CrossRef] [PubMed]
  102. Kloeckener-Gruissem, B.; Vandekerckhove, K.; Nürnberg, G.; Neidhardt, J.; Zeitz, C.; Nürnberg, P.; Schipper, I.; Berger, W. Mutation of solute carrier SLC16A12 associates with a syndrome combining juvenile cataract with microcornea and renal glucosuria. Am. J. Hum. Genet. 2008, 82, 772–779. [Google Scholar] [CrossRef] [PubMed]
  103. Vandekerckhove, K.; Lange, A.P.; Herzog, D.; Schipper, I. Juvenile cataract associated with microcornea and glucosuria: A new syndrome. Klin Monbl Augenheilkd 2007, 224, 344–346. [Google Scholar] [CrossRef] [PubMed]
  104. Dhayat, N.; Simonin, A.; Anderegg, M.; Pathare, G.; Luscher, B.P.; Deisl, C.; Albano, G.; Mordasini, D.; Hediger, M.A.; Surbek, D.V.; et al. Mutation in the Monocarboxylate Transporter 12 Gene Affects Guanidinoacetate Excretion but Does Not Cause Glucosuria. J. Am. Soc. Nephrol. 2016, 27, 1426–1436. [Google Scholar] [CrossRef]
  105. Schäffer, A.A. Digenic inheritance in medical genetics. J. Med. Genet. 2013, 50, 641–652. [Google Scholar] [CrossRef] [PubMed]
  106. Gazzo, A.; Raimondi, D.; Daneels, D.; Moreau, Y.; Smits, G.; van Dooren, S.; Lenaerts, T. Understanding mutational effects in digenic diseases. Nucleic Acids Res. 2017, 45, e140. [Google Scholar] [CrossRef]
  107. Yates, C.M.; Sternberg, M.J. Proteins and domains vary in their tolerance of non-synonymous single nucleotide polymorphisms (nsSNPs). J. Mol. Biol. 2013, 425, 1274–1286. [Google Scholar] [CrossRef]
  108. Addis, M.; Meloni, C.; Tosetto, E.; Ceol, M.; Cristofaro, R.; Melis, M.A.; Vercelloni, P.; del Prete, D.; Marra, G.; Anglani, F. An atypical Dent’s disease phenotype caused by co-inheritance of mutations at CLCN5 and OCRL genes. Eur. J. Hum. Genet. 2013, 21, 687–690. [Google Scholar] [CrossRef]
  109. Nozu, K.; Inagaki, T.; Fu, X.J.; Nozu, Y.; Kaito, H.; Kanda, K.; Sekine, T.; Igarashi, T.; Nakanishi, K.; Yoshikawa, N.; et al. Molecular analysis of digenic inheritance in Bartter syndrome with sensorineural deafness. J. Med. Genet. 2008, 45, 182–186. [Google Scholar] [CrossRef]
  110. Sile, S.; Velez, D.R.; Gillani, N.B.; Alexander, C.A.; George, A.L., Jr.; Williams, S.M. Haplotype diversity in four genes (CLCNKA, CLCNKB, BSND, NEDD4L) involved in renal salt reabsorption. Hum. Hered. 2007, 65, 33–46. [Google Scholar] [CrossRef]
  111. Kong, Y.; Xu, K.; Yuan, K.; Zhu, J.; Gu, W.; Liang, L.; Wang, C. Digenetic inheritance of SLC12A3 and CLCNKB genes in a Chinese girl with Gitelman syndrome. BMC Pediatr. 2019, 19, 114. [Google Scholar] [CrossRef] [PubMed]
  112. Blanchard, A.; Bockenhauer, D.; Bolignano, D.; Calò, L.A.; Cosyns, E.; Devuyst, O.; Ellison, D.H.; Frankl, F.E.K.; Knoers, N.V.A.M.; Konrad, M.; et al. Gitelman syndrome: Consensus and guidance from a Kidney Disease: Improving Global Outcomes (KDIGO) Controversies Conference. Kidney Int. 2017, 91, 24–33. [Google Scholar] [CrossRef] [PubMed]
  113. Schlingmann, K.P.; Konrad, M.; Jeck, N.; Waldegger, P.; Reinalter, S.C.; Holder, M.; Seyberth, H.W.; Waldegger, S. Salt wasting and deafness resulting from mutations in two chloride channels. N. Engl. J. Med. 2004, 350, 1314–1319. [Google Scholar] [CrossRef] [PubMed]
  114. Scholl, U.; Hebeisen, S.; Janssen, A.G.; Muller-Newen, G.; Alekov, A.; Fahlke, C. Barttin modulates trafficking and function of ClC-K channels. Proc. Natl. Acad. Sci. USA 2006, 103, 11411–11416. [Google Scholar] [CrossRef] [PubMed]
  115. Wojciechowski, D.; Thiemann, S.; Schaal, C.; Rahtz, A.; de la Roche, J.; Begemann, B.; Becher, T.; Fischer, M. Activation of renal ClC-K chloride channels depends on an intact N terminus of their accessory subunit barttin. J. Biol. Chem. 2018, 293, 8626–8637. [Google Scholar] [CrossRef] [PubMed]
  116. Konrad, M.; Vollmer, M.; Lemmink, H.H.; van den Heuvel, L.P.; Jeck, N.; Vargas-Poussou, R.; Lakings, A.; Ruf, R.; Deschenes, G.; Antignac, C.; et al. Mutations in the chloride channel gene CLCNKB as a cause of classic Bartter syndrome. J. Am. Soc. Nephrol. 2000, 11, 1449–1459. [Google Scholar] [PubMed]
  117. Simon, D.B.; Bindra, R.S.; Mansfield, T.A.; Nelson-Williams, C.; Mendonca, E.; Stone, R.; Schurman, S. Mutations in the chloride channel gene, CLCNKB, cause Bartter’s syndrome type III. Nat. Genet. 1997, 17, 171–178. [Google Scholar] [CrossRef]
  118. Nagara, M.; Papagregoriou, G.; Abdallah, R.B.; Landoulsi, Z.; Bouyacoub, Y.; Elouej, S.; Kefi, R.; Pippucci, T.; Voskarides, K.; Bashamboo, A. Distal renal tubular acidosis in a Libyan patient: Evidence for digenic inheritance. Eur. J. Med. Genet. 2018, 61, 1–7. [Google Scholar] [CrossRef]
  119. Duran, D.; Jin, S.C.; DeSpenza, T.; Nelson-Williams, C.; Cogal, A.G.; Abrash, E.W.; Harris, P.C.; Lieske, J.C.; Shimshak, S.J.E.; Mane, S.; et al. Digenic mutations of human OCRL paralogs in Dent’s disease type 2 associated with Chiari I malformation. Hum. Genome Var. 2016, 3, 16042. [Google Scholar] [CrossRef]
  120. Tanikawa, C.; Kamatani, Y.; Terao, C.; Usami, M.; Takahashi, A.; Momozawa, Y.; Suzuki, K.; Ogishima, S.; Shimizu, A.; Satoh, M.; et al. Novel Risk Loci Identified in a Genome-Wide Association Study of Urolithiasis in a Japanese Population. J. Am. Soc. Nephrol. 2019, 30, 855–864. [Google Scholar] [CrossRef]
  121. Palsson, R.; Indridason, O.S.; Edvardsson, V.O.; Oddsson, A. Genetics of common complex kidney stone disease: Insights from genome-wide association studies. Urolithiasis 2019, 47, 11–21. [Google Scholar] [CrossRef] [PubMed]
  122. Arcidiacono, T.; Simonini, M.; Lanzani, C.; Citterio, L.; Salvi, E.; Barlassina, C.; Spotti, D.; Cusi, D.; Manunta, P.; Vezzoli, G. Claudin-14 Gene Polymorphisms and Urine Calcium Excretion. Clin. J. Am. Soc. Nephrol. 2018, 13, 1542–1549. [Google Scholar] [CrossRef] [PubMed]

Article Metrics

Citations

Article Access Statistics

Journal Statistics
Multiple requests from the same IP address are counted as one view.
Download PDF
Identification of Structural Variation in Chimpanzees Using Optical Mapping and Nanopore Sequencing
Previous
Seascape Genetics and the Spatial Ecology of Juvenile Green Turtles
Next