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Generation of dyskeratosis congenita-like hematopoietic stem cells through the stable inhibition of DKC1

Abstract

Dyskeratosis congenita (DC) is a rare telomere biology disorder, which results in different clinical manifestations, including severe bone marrow failure. To date, the only curative treatment for the bone marrow failure in DC patients is allogeneic hematopoietic stem cell transplantation. However, due to the toxicity associated to this treatment, improved therapies are recommended for DC patients. Here, we aimed at generating DC-like human hematopoietic stem cells in which the efficacy of innovative therapies could be investigated. Because X-linked DC is the most frequent form of the disease and is associated with an impaired expression of DKC1, we have generated DC-like hematopoietic stem cells based on the stable knock-down of DKC1 in human CD34+ cells with lentiviral vectors encoding for DKC1 short hairpin RNAs. At a molecular level, DKC1-interfered CD34+ cells showed a decreased expression of TERC, as well as a diminished telomerase activity and increased DNA damage, cell senescence, and apoptosis. Moreover, DKC1-interfered human CD34+ cells showed defective clonogenic ability and were incapable of repopulating the hematopoiesis of immunodeficient NSG mice. The development of DC-like hematopoietic stem cells will facilitate the understanding of the molecular and cellular basis of this inherited bone marrow failure syndrome and will serve as a platform to evaluate the efficacy of new hematopoietic therapies for DC.

Introduction

Telomeres are repetitive nucleotide sequences localized at the end of the eukaryotic chromosomes, which play an essential role in the chromosome replication and stability. Telomeric DNA consists of tandemly repeated TTAGGG sequences [1, 2] which become shortened as a consequence of the division of somatic cells, leading to a situation called “end replication problem”. The loss of telomeric repeats is counteracted by the telomerase complex [3]. Telomerase is a specialized ribonucleoprotein reverse transcriptase mainly composed of TERT (with reverse transcriptase activity), TERC (the RNA template) and dyskerin, which stabilizes telomerase complex [4,5,6]. Although telomerase expression is low or absent in most somatic cells, telomerase remains active in somatic stem cells to maintain their telomere length [7]. A decreased telomerase activity results in an abnormal telomere biology, leading to telomere biology disorders (TBD), such as aplastic anemia, pulmonary fibrosis, coats plus syndrome, or dyskeratosis congenita (DC) [2, 8].

Clinically, DC patients are characterized by the mucocutaneous triad (nail dystrophy, oral leukoplakia, and abnormal skin pigmentation). Nevertheless, bone marrow failure (BMF) is the main cause of early mortality of these patients (80% of the cases) as also occurs in other congenic BMF syndromes [7]. So far, 14 DC associated genes have been discovered, all of them involved in the telomere maintenance: DKC1, TERT, TERC, TINF2, TCAB1, NOP10, NHP2, CTC1, RTEL1, TPP1, PARN, POT1, NAF1, and STN1 [9,10,11,12]. According to the inheritance of the disease, three DC variants have been reported: X-linked recessive, autosomal dominant, and autosomal recessive. The X-linked variant of DC (X-DC) is mainly caused by point mutations in DKC1, which encodes for the dyskerin nucleolar protein [13]. Interestingly, the knock-out of Dkc1 has been reported to be embryonic lethal in mice [14]. This observation and the fact that only hypomorphic DKC1 mutations have been reported in X-DC patients [15, 16] reveals the critical relevance of DKC1 in the cell biology.

To date, the only curative treatment for BMF in DC patients is the allogeneic hematopoietic stem cell transplantation (alloHSCT) from healthy donors. Apart from the low availability of HLA-matched donors, the outcome of DC patients undergoing alloHSCT is very poor, mainly due to the toxicity of conditioning regimens and the development of graft versus host disease [17]. Thus, new therapies such as gene therapy without cytotoxic conditioning, as recently reported in Fanconi anemia (FA) [18], would be highly beneficial for DC patients.

Taking into account that periodic BM aspirations are not part of the routine follow-up of DC patients, difficulties in the access of HSCs constitute an important limitation in the development of new therapies for DC patients. Furthermore, the animal models of telomeropathies developed to date do not mimic the characteristic BMF of DC patients [19]. Considering that DKC1 is one the most frequently mutated genes in DC [9], the purpose of this study was the generation of DC-like human HSCs based on the interference of DKC1 in human HSCs which would serve as a platform for the development of new hematopoietic therapies for DC patients.

Materials and methods

Detailed methods are shown as supplementary data

Results

Molecular implications of DKC1 inhibition in human hematopoietic stem and progenitor cells

Previous studies revealed that the knock-out of Dkc1 is embryonic lethal [14] and that only hypomorphic mutations have been found in X-DC patients [15, 16]. In this study, we aimed at generating X-DC-like hematopoietic stem and progenitor cells (HSPCs) based on the downregulation of DKC1 with short hairpin RNA (shRNA) lentiviral vectors (LVs). shRNA-LVs carried a puromycin resistance gene to facilitate the selection of transduced HSPCs (see the “Materials and methods” section).

The efficacy of seven different shRNA-LVs (Suppl. Table 1) to downregulate the expression of DKC1 was screened in healthy donor CD34+ cells (Suppl. Fig. 1A). In subsequent experiments, we showed that three of these shRNA-LVs, iDKC1, iDKC4, and iDKC7 significantly decreased DKC1 mRNA levels to 34–47% compared to levels determined in cells transduced with the scrambled shRNA LV (Fig. 1a and Suppl. Table 2A). Vector copy numbers (VCN) determined in these cells showed the presence of 1–8 copies per cell in all groups (Suppl. Fig. 1B), revealing that inhibitory effects upon DKC1 were related to the interfering proviruses.

Fig. 1
figure1

Molecular implications associated with the inhibition of DKC1 in human hematopoietic stem and progenitor cells. Cord blood CD34+ cells were transduced with specific anti shRNA-LVs and maintained in liquid cultures for 5–8 days (see details in the “Materials and methods” section). a Decreased expression of DKC1 gene after CD34+ cell transduction with specific shRNA-LVs (7 independent experiments were conducted; n = 7). DKC1 expression levels in cells transduced with DKC1 shRNA LVs represent relative values of those obtained in cells transduced with the scrambled shRNA LV. Raw data are shown in Suppl. Table 2. b Decreased expression of TERC after CD34+ cell transduction with specific shRNA-LVs (n = 7). Raw data are shown in Suppl. Table 2. c Representative analysis of a telomeric repeat amplification protocol (TRAP). Internal control is marked by the black arrow, negative control was performed with buffer (NC) and non-transduced cells were used as control. d Analysis of the telomerase activity after transduction with shRNA LVs (n = 3). Data are expressed as mean ± SEM. Asterisks indicate significant differences determined by Student’s t test (*p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001)

To investigate the molecular implications resulting from the inhibition of DKC1, we first evaluated the expression of TERC in CD34+ cells transduced with scrambled and DKC1-shRNA LVs. As shown in Fig. 1b and Suppl. Table 2B, TERC mRNA levels in cells transduced with iDKC1-, iDKC4-, or iDKC7-LVs were respectively decreased to 27.7% ± 10.8%, 49.1% ± 18.6%, and 19.8% ± 11.5%, compared to levels determined in the control group. In subsequent analyses, changes in the telomerase functionality of DKC1-interfered CD34+ cells were quantified. To this end, we measured telomerase activity of DKC1-interfered and control CD34+ cells by the TRAP assay. These results showed marked decreases in the telomerase activity of CD34+ cells that had been transduced with iDKC1-, iDKC4-, or iDKC7-LVs, which showed values of 42.8% ± 19%, 61.5% ± 3.6%, and 43.7% ± 15.6%, respectively, of values determined in the control group (Fig. 1c and d).

In the following experiments, we investigated the implication of DKC1 interference in the DNA damage determined in CD34+ cells. Analyses of γH2AX foci in the nucleus of cells transduced with iDKC1-, iDKC4-, or iDKC7-LVs revealed that only 19% of cells transduced with the scrambled shRNA LV showed more than 10 γH2AX foci per cell. However, an important increase in the proportion of CD34+ cells with γH2AX foci was observed in cells transduced with either the iDKC1- (76%), iDKC4- (42%), or the iDKC7- (61%) LVs (Fig. 2a). In next studies, we determined the expression of phosphorylated p53 and p21 (CDKN1A) in CD34+ cells transduced with the different constructs. As shown in Fig. 2b, phosphorylated p53 expression was higher in CD34+ cells transduced with the DKC1-shRNA LVs. When the expression of p21 was tested, iDKC1- and iDKC4-LVs enhanced its levels (2.7 ± 0.7 and 2.4 ± 0.26 fold, respectively) compared to the control group, though this was not observed in iDKC7-transduced cells (Fig. 2c and Suppl. Table 2C). Levels of caspase 3 and Annexin V+ cells were also increased in CD34+ cells transduced with either type of DKC1-shRNA LVs, although levels did not reach statistical significance (Fig. 2b and d and Suppl. Fig. 2). Taken together these results suggest the induction of DNA damage, cell senescence, and apoptosis of DKC1-interfered HSPCs (Fig. 2).

Fig. 2
figure2

DNA damage and apoptosis associated with the inhibition of DKC1 in human hematopoietic stem and progenitor cells. Cord blood CD34+ cells were transduced with specific anti-shRNA-LVs and maintained in liquid cultures for 10 days (see details in “Materials and methods” section). a Analysis of DNA damage in CD34+ cells transduced with specific shRNA LVs. Cells with more than 10 γH2AX foci per cell are shown (n = 3). b Representative Western blot (WB) assays for phosphorylated p53 (upper WB) and fragmented caspase 3 (lower WB) expression using β-actin as control. Quantification appears in italics below the images as the ratio of expression in relation with the control protein. c Increased expression of p21 after transduction of CD34+ cells with specific shRNA-LVs (n = 6). Raw data are shown in Suppl. Table 2. d Fold increase of apoptotic cells (Annexin V+) in comparison with the scrambled control condition (n = 3). Data are expressed as mean ± SEM. Asterisks indicate significant differences determined by Student’s t test (*p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001)

The interfered expression of DKC1 impairs the in vitro growth and ablates the in vivo repopulating ability of human HSPC

To determine whether the knockdown of DKC1 affects the functionality of human HSPCs, DKC1-interfered CD34+ cells were in vitro cultured for 10 days (see the “Materials and methods” section) to evaluate implications in cell growth. In these studies, the portion of CD34+ cells at the end of the culture period was similar among the different experimental groups (Suppl. Fig. 3). While transduced cells with the scrambled shRNA-LV showed a marked cell expansion during this period (117 ± 87.31 fold compared to initial cell numbers), levels of expansion observed in iDKC1- and iDKC4-transduced CD34+ cells were only 13 ± 6.99 and 15.3 ± 2.42 fold compared to input cell numbers (Fig. 3a). These values represent a significant decrease to 20 ± 8% and 10 ± 4%, respectively, of cell expansions corresponding to the control group (CD34+ cells transduced with the scrambled shRNA LV) (Fig. 3b). As happened with p21 levels (Fig. 2c), defects in cell proliferation were not observed with iDKC7-transduced cells (Fig. 3b). In additional studies, we evaluated changes in the telomere length in DKC1-interfered cells, although no differences were observed among the different experimental groups (Suppl. Fig. 4). This suggests that much longer incubation periods would be required to observe a significant telomere shortening, although defects in the ability of DKC1-interfered cells to grow in culture limited the possibility of evaluating changes in the telomere length long-term after DKC1-interference.

Fig. 3
figure3

Analysis of the in vitro growth properties and in vivo repopulating ability of DKC1-interfered CD34+ cells. a Analysis of the cell expansion analyzed 2 weeks after ex vivo incubation of transduced cells in liquid culture (n = 5). b Relative cell expansion in comparison with cells transduced with the scrambled shRNA-LV (n = 6). c Analysis of the clonogenic potential of CD34+ cells transduced with DKC1-shRNA LVs and scrambled shRNA-LVs (n = 8). d Analysis of the repopulation potential of CD34+ cells transduced with scrambled shRNA-LV (orange dots) or DKC1-shRNA LVs (blue dots). The proportion of human CD45+ cells in the BM of recipient mice was analyzed at 1–3 months post-transplantation (mpt). Data are expressed as mean ± SEM. Asterisks indicate significant differences determined by Student’s t test (*p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001)

When the clonogenic potential of DKC1-interfered cells was assessed, a significant reduction in the number of colonies generated by CD34+ cells transduced with any of the three anti-DKC1 LVs was observed (Fig. 3c and Suppl. Fig. 5). Again, reductions were more significant in cells transduced with the iDKC1- and iDKC4-LVs, which reduced the clonogenic potential to 20% ± 4% and 52% ± 5%, respectively, compared to the control group.

Based on the results obtained in cells transduced with iDKC1-LV, in a final set of experiments, we assessed the repopulation potential of CD34+ cells transduced with this LV, and with a control LV (scrambled shRNA-LV). To this aim, 8 × 105 transduced cells, which contained an average number of 30,000 transduced CD34+ cells (Suppl. Fig. 3), were transplanted into NSG mice. As shown in Fig. 3d, CD34+ cells transduced with the control LV showed an evident in vivo repopulating ability (see orange dots in Fig. 3d). In these animals, the presence of human hematopoietic progenitors (CD34+), as well as of myeloid (CD33+) and lymphoid cells (CD19+) were observed (Suppl. Fig. 6), confirming the multi-lineage repopulation ability of human HSPCs transduced with the scrambled shRNA LVs. In sharp contrast with these observations, 7 out of the 8 recipients that were transplanted with iDKC1-transduced CD34+ cells failed to repopulate recipient NSG mice (see light blue dots in Fig. 3d). Interestingly, when VCNs were tested in the BM of mice engrafted with cells of the control group, the presence of integrated LV copies was observed in all cases (0.3 to 1 VCNs/cell; Suppl. Fig. 7). However, no copies of the iDKC1 provirus were detected in BM cells from the animal engrafted with cells transduced with the DKC1-shRNA LV (Suppl. Fig. 7). This reveals that this specific recipient was repopulated with cells that have survived the puromycin selection, although did not integrate in their genome the iDKC1-interfering provirus. As expected, the presence of the DKC1-shRNA provirus was neither observed in the non-engrafted NSG recipients (Suppl. Fig. 7), since no human hematopoietic cells were observed in these recipients (Fig. 3d).

Based on the hematopoietic studies conducted in these experiments, we conclude that the inhibited expression of DKC1 impairs the in vitro growth properties and the in vivo repopulating ability of human HSPCs.

Discussion

The absence of good models which mimic HSC defects characteristic of DC patients [20] constitute an important limitation in the development of therapies for the treatment of BMF of these patients [21]. In this study, we show that three different DKC1-shRNAs inhibited DKC1 expression to levels below 50%, similar to observations in X-DC patients, all of them with hypomorphic mutations in DKC1 [22, 23]. Consistent with data from these patients [22,23,24,25], DKC1 inhibition in healthy HSPCs was associated with a significant reduction in the expression of TERC and of telomerase activity. As also observed in cells from DC patients, DKC1 interference with iDKC1- and iDKC4-LVs induced markers of DNA damage, cell senescence, and apoptosis, such as the generation of nuclear γH2AX foci and upregulation of caspase 3, p21, and phosphorylated p53.

Consistent with observations showing that BM from DC patients contain reduced numbers of HSPCs [26], DKC1 interference with iDKC1- and iDKC4-LVs markedly reduced the cell expansion, as well as the clonogenic and in vivo repopulating potential of CD34+ cells. The fact that, in contrast to iDKC1- and iDKC4-, iDKC7-LV did not increase levels of p21 nor affected the cell growth of CD34+ cells suggests the different functional implications associated with the interference of different domains of DKC1.

Remarkably, defects in the in vitro and in vivo growth of human HSPCs were evident immediately after DKC1 interference, despite no changes in the telomere length of these cells were observed. This observation indicates that the inhibited proliferation and repopulation ability of DC-like HSPCs, and most probably of HSCs from X-DC patients, are not necessarily a consequence of the reduced telomere length. Thus, we propose that the generation of DNA damage and induction of cell senescence and apoptotic responses would account for these relevant phenotypic defects of DC HSPCs. Although the inability of DKC1-interfered HSCs to engraft in immunodeficient mice would limit studies of the behavior of these cells in vivo, this model will be an invaluable tool to evaluate the efficacy of ex vivo therapies, such as hematopoietic gene therapy, to restore the repopulating properties of HSCs defective in DKC1. Moreover, the repopulation defects observed in our study in DC-like HSPCs would suggest that the restored function of dyskerin through gene therapy strategies might confer a proliferation advantage in DC HSPCs, as we have already demonstrated in FA patients treated by hematopoietic gene therapy [27].

Aiming at restoring the function of X-DC cells, discrepant results have been observed after the ectopic expression of dyskerin [22, 28, 29]. The use of codon optimized sequences of DKC1 (not recognized by DKC1-shRNAs) or the use of functionally active DKC1-derived sequences, such as those encoding for GSE24.2 and GSE4 peptides [29,30,31], might compensate the molecular and cellular defects of DC HSCs. As proposed for FA [27], the correction of HSCs in early stages of the disease of DC would be also relevant to complement the function of affected genes before telomeres are significantly reduced. Whether or not gene complementation in DC HSPCs with shortened telomeres would facilitate their elongation is currently unknown and will require extensive studies in this and other DC models.

Conclusion

The generation of DC-like HSPCs constitutes a new platform for studying the molecular basis of the BMF in DC and also for screening the efficacy and safety of hematopoietic therapies for DC patients, including gene therapy and drugs capable of protecting or restoring the function of DC HSPCs.

Availability of data and materials

The authors confirm that the data supporting the findings of this study are available from the corresponding author on reasonable request.

Abbreviations

AlloHSCT:

Allogeneic hematopoietic stem cell transplantation

BM:

Bone marrow

BMF:

Bone marrow failure

DC:

Dyskeratosis congenita

FA:

Fanconi anemia

HSC:

Hematopoietic stem cell

HSPC:

Hematopoietic stem and progenitor cell

LV:

Lentiviral vector

shRNA:

Short hairpin RNA

TBD:

Telomere biology disorder

TERC:

Telomerase RNA component

TERT:

Telomerase reverse transcriptase

TRAP:

Telomeric repeat amplification protocol

VCN:

Vector copy number

WB:

Western blot

X-DC:

X-linked dyskeratosis congenita

References

  1. 1.

    Meyne J, Ratliff RL, Moyzis RK. Conservation of the human telomere sequence (TTAGGG) n among vertebrates. Proc Natl Acad Sci U S A. 1989;86(18):7049–53 PubMed PMID: 2780561. Pubmed Central PMCID: PMC297991.

    CAS  Article  Google Scholar 

  2. 2.

    Savage SA. Human telomeres and telomere biology disorders. Prog Mol Biol Transl Sci. 2014;125:41–66 PubMed PMID: 24993697.

    CAS  Article  Google Scholar 

  3. 3.

    Jones M, Bisht K, Savage SA, Nandakumar J, Keegan CE, Maillard I. The shelterin complex and hematopoiesis. J Clin Invest. 2016;126(5):1621–9 PubMed PMID: 27135879. Pubmed Central PMCID: PMC4855927.

    Article  Google Scholar 

  4. 4.

    Greider CW, Blackburn EH. Identification of a specific telomere terminal transferase activity in Tetrahymena extracts. Cell. 1985;43(2 Pt 1):405–13 PubMed PMID: 3907856.

    CAS  Article  Google Scholar 

  5. 5.

    Blackburn EH. Telomeres and telomerase: their mechanisms of action and the effects of altering their functions. FEBS Lett. 2005;579(4):859–62 PubMed PMID: 15680963.

    CAS  Article  Google Scholar 

  6. 6.

    Cohen SB, Graham ME, Lovrecz GO, Bache N, Robinson PJ, Reddel RR. Protein composition of catalytically active human telomerase from immortal cells. Science. 2007;315(5820):1850–3 PubMed PMID: 17395830.

    CAS  Article  Google Scholar 

  7. 7.

    Kirwan M, Dokal I. Dyskeratosis congenita: a genetic disorder of many faces. Clin Genet. 2008;73(2):103–12 PubMed PMID: 18005359.

    CAS  Article  Google Scholar 

  8. 8.

    Townsley DM, Dumitriu B, Young NS. Bone marrow failure and the telomeropathies. Blood. 2014;124(18):2775–83 PubMed PMID: 25237198. Pubmed Central PMCID: PMC4215309.

    CAS  Article  Google Scholar 

  9. 9.

    Dokal I, Vulliamy T, Mason P, Bessler M. Clinical utility gene card for: dyskeratosis congenita - update 2015. Eur J Hum Genet. 2015;23(4) PubMed PMID: 25182133. Pubmed Central PMCID: PMC4667501.

  10. 10.

    Perdigones N, Perin JC, Schiano I, Nicholas P, Biegel JA, Mason PJ, et al. Clonal hematopoiesis in patients with dyskeratosis congenita. Am J Hematol. 2016;91(12):1227–33 PubMed PMID: 27622320. Pubmed Central PMCID: PMC5118079.

    CAS  Article  Google Scholar 

  11. 11.

    Perona R, Iarriccio L, Pintado-Berninches L, Rodriguez-Centeno J, Manguan-Garcia C, Garcia E, et al. Molecular diagnosis and precision therapeutic approaches for telomere biology disorders. In: Larramendy ML, editor. Telomere - A Complex End of a Chromosome. Rijeka: InTech; 2016. p. Ch. 05.

    Google Scholar 

  12. 12.

    Savage SA, Dufour C. Classical inherited bone marrow failure syndromes with high risk for myelodysplastic syndrome and acute myelogenous leukemia. Semin Hematol. 2017;54(2):105–14 PubMed PMID: 28637614.

    Article  Google Scholar 

  13. 13.

    Dokal I, Vulliamy T. Inherited bone marrow failure syndromes. Haematologica. 2010;95(8):1236–40 PubMed PMID: 20675743. Pubmed Central PMCID: PMC2913069.

    CAS  Article  Google Scholar 

  14. 14.

    He J, Navarrete S, Jasinski M, Vulliamy T, Dokal I, Bessler M, et al. Targeted disruption of Dkc1, the gene mutated in X-linked dyskeratosis congenita, causes embryonic lethality in mice. Oncogene. 2002;21(50):7740–4 PubMed PMID: 12400016.

    CAS  Article  Google Scholar 

  15. 15.

    Calado RT, Regal JA, Hills M, Yewdell WT, Dalmazzo LF, Zago MA, et al. Constitutional hypomorphic telomerase mutations in patients with acute myeloid leukemia. Proc Natl Acad Sci U S A. 2009;106(4):1187–92 PubMed PMID: 19147845. Pubmed Central PMCID: PMC2627806.

    CAS  Article  Google Scholar 

  16. 16.

    Fernandez Garcia MS, Teruya-Feldstein J. The diagnosis and treatment of dyskeratosis congenita: a review. J Blood Med. 2014;5:157–67 PubMed PMID: 25170286. Pubmed Central PMCID: PMC4145822.

    PubMed  PubMed Central  Google Scholar 

  17. 17.

    Barbaro P, Vedi A. Survival after hematopoietic stem cell transplant in patients with dyskeratosis congenita: systematic review of the literature. Biol Blood Marrow Transplant. 2016;22(7):1152–8 PubMed PMID: 26968789.

    Article  Google Scholar 

  18. 18.

    Rio P, Navarro S, Wang W, Sanchez-Dominguez R, Pujol RM, Segovia JC, et al. Successful engraftment of gene-corrected hematopoietic stem cells in non-conditioned patients with Fanconi anemia. Nat Med. 2019;25(9):1396–401 PubMed PMID: 31501599.

    CAS  Article  Google Scholar 

  19. 19.

    Autexier C. POT of gold: modeling dyskeratosis congenita in the mouse. Genes Dev. 2008;22(13):1731–6 PubMed PMID: 18593874. Pubmed Central PMCID: PMC2732423.

    CAS  Article  Google Scholar 

  20. 20.

    Kirwan M, Dokal I. Dyskeratosis congenita, stem cells and telomeres. Biochim Biophys Acta. 2009;1792(4):371–9 PubMed PMID: 19419704.

    CAS  Article  Google Scholar 

  21. 21.

    Hockemeyer D, Palm W, Wang RC, Couto SS, de Lange T. Engineered telomere degradation models dyskeratosis congenita. Genes Dev. 2008;22(13):1773–85.

    CAS  Article  Google Scholar 

  22. 22.

    Mitchell JR, Wood E, Collins K. A telomerase component is defective in the human disease dyskeratosis congenita. Nature. 1999;402:551 12/02/online.

    CAS  Article  Google Scholar 

  23. 23.

    Parry EM, Alder JK, Lee SS, Phillips JA 3rd, Loyd JE, Duggal P, et al. Decreased dyskerin levels as a mechanism of telomere shortening in X-linked dyskeratosis congenita. J Med Genet. 2011;48(5):327–33 PubMed PMID: 21415081. Pubmed Central PMCID: PMC3088476.

    CAS  Article  Google Scholar 

  24. 24.

    Cong YS, Wright WE, Shay JW. Human telomerase and its regulation. Microbiol Mol Biol Rev. 2002;66(3):407–25.

    CAS  Article  Google Scholar 

  25. 25.

    Marrone A, Stevens D, Vulliamy T, Dokal I, Mason PJ. Heterozygous telomerase RNA mutations found in dyskeratosis congenita and aplastic anemia reduce telomerase activity via haploinsufficiency. Blood. 2004;104(13):3936–42.

    CAS  Article  Google Scholar 

  26. 26.

    Frederick D, Goldman GA, Al J, Klingelhutz MH, Cooper SR, Hamilton WS, Schlueter AJ, Lambie K, Connie J. Eaves and Peter M. Lansdorp. Characteristics of primitive hematopoietic cells from patients with Dyskeratosis congenita. Hematopoiesis and Stem Cells. 2008;111(9):4523–31.

    Google Scholar 

  27. 27.

    Rio P, Navarro S, Guenechea G, Sanchez-Dominguez R, Lamana ML, Yanez R, et al. Engraftment and in vivo proliferation advantage of gene-corrected mobilized CD34(+) cells from Fanconi anemia patients. Blood. 2017;130(13):1535–42 PubMed PMID: 28801449.

    CAS  Article  Google Scholar 

  28. 28.

    Bellodi C, McMahon M, Contreras A, Juliano D, Kopmar N, Nakamura T, et al. H/ACA small RNA dysfunctions in disease reveal key roles for noncoding RNA modifications in hematopoietic stem cell differentiation. Cell Rep. 2013;3(5):1493–502.

    CAS  Article  Google Scholar 

  29. 29.

    Machado-Pinilla R, Sanchez-Perez I, Murguia JR, Sastre L, Perona R. A dyskerin motif reactivates telomerase activity in X-linked dyskeratosis congenita and in telomerase-deficient human cells. Blood. 2008;111(5):2606–14 PubMed PMID: 18057229.

    CAS  Article  Google Scholar 

  30. 30.

    Iarriccio L, Manguan-Garcia C, Pintado-Berninches L, Mancheno JM, Molina A, Perona R, et al. GSE4, a small dyskerin- and GSE24.2-related peptide, induces telomerase activity, cell proliferation and reduces DNA damage, oxidative stress and cell senescence in dyskerin mutant cells. PloS one. 2015;10(11):e0142980 PubMed PMID: 26571381. Pubmed Central PMCID: PMC4646510.

    Article  Google Scholar 

  31. 31.

    Manguan-Garcia C, Pintado-Berninches L, Carrillo J, Machado-Pinilla R, Sastre L, Perez-Quilis C, et al. Expression of the genetic suppressor element 24.2 (GSE24.2) decreases DNA damage and oxidative stress in X-linked dyskeratosis congenita cells. PloS one. 2014;9(7):e101424 PubMed PMID: 24987982. Pubmed Central PMCID: 4079255.

    Article  Google Scholar 

Download references

Acknowledgements

The authors would like to thank Miguel A. Martin for the careful maintenance of the animals and Omaira Alberquilla and Dr. Rebeca Sánchez for their technical assistance in flow cytometry. The authors would also like to thank to Dr. Elena G. Arias-Salgado for measurement of telomere length and the Centro de Transfusiones de la Comunidad de Madrid for the cord blood human samples.

Funding

This work was supported by grants from the “Ministerio de Economía, Comercio y Competitividad and Fondo Europeo de Desarrollo Regional (FEDER)” (SAF2015-68073-R) and from the “Ministerio de Ciencia, Innovación y Universidades and Fondo Europeo de Desarrollo Regional (FEDER)” (RTI2018-097125-B-I00) and P17-01401 from “Fondo de Investigaciones Sanitarias, Instituto de Salud Carlos III (FIS-ISCIII)”. The authors also thank the Fundación Botín for promoting translational research at the Hematopoietic Innovative Therapies Division of the CIEMAT. CIBERER is an initiative of the “Instituto de Salud Carlos III” and “FEDER”. CCR was supported by an FPI grant from the Universidad Autónoma de Madrid (UAM).

Author information

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Authors

Contributions

CCR: conception and design, collection and/or assembly of data, data analysis and interpretation, and manuscript writing; HAZ: conception and design, collection and/or assembly of data, and data analysis and interpretation; LPB: collection and/or assembly of data; BFV: collection and/or assembly of data; MLL: collection and/or assembly of data; CMG: collection and/or assembly of data; LS: conception and design, data analysis and interpretation, and manuscript writing; JAB: conception and design, data analysis and interpretation, financial support, and manuscript writing; RP: conception and design, data analysis and interpretation, financial support, manuscript writing, and final approval of manuscript; GG: conception and design, collection and/or assembly of data, data analysis and interpretation, financial support, manuscript writing, and final approval of manuscript.

Corresponding author

Correspondence to Guillermo Guenechea.

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Ethics approval and consent to participate

Human cord blood samples from healthy donors were kindly provided by the Centro de Transfusión de la Comunidad de Madrid under the approval of its IRB and in accordance with the Helsinki Declaration. In all instances, informed consents were previously signed by the donors. All experimental procedures involving mice were conducted at the CIEMAT animal facility (registration number 28079-21 A) and were approved by the Animal Welfare Body of this institution. This project was authorized by the competent authorities of the Comunidad de Madrid, under the registration number PROEX-70/15 fulfilling Spanish and European legislation (Spanish RD 53/2013 and Law 6/2013 in compliance with the European Directive 2010/63/EU about the use and protection of vertebrate mammals used for experimentation and other scientific purposes).

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Supplementary Information

Additional file 1:

Supplementary Table 1. Overview of the information about the shRNA sequences. Supplementary Table 2. Compilation of RT-qPCR data in CD34+ transduced with scrambled and DKC1-shRNA LVs. A) Results of DKC1 expression (n = 7). B) TERC expression data (n = 7). C) Expression of CDKN1A gene (n = 6). Triplicates were performed in every experiment and results are expressed as mean ± SEM

Additional file 2:

Supplementary Figure 1. A) DKC1 expression after transduction with a library of DKC1-specific shRNAs, n=3. Analyses were performed 5-8 days post-transduction. B) Analysis of the vector copy number per cell (VCN/cell) after transduction with shRNA-LVs. Analyses were performed at least after 15 days post-transduction. Supplementary Figure 2. Gating strategy and analysis of Annexin V-based apoptosis assay. Representative dot-plots of flow cytometry analyses in DKC1-interferred CD34+ cells are shown. Supplementary Figure 3. Levels of CD34+ cells after 10 days in culture (n=3). Supplementary Figure 4. Telomere length in human CD34+ samples transduced with DKC1-shRNAs and scrambled-shRNA LVs and cultured for 8 days as described in Materials and Methods section. For comparison, also human peripheral blood cells and fresh CD34+ cells were analyzed (n=1). Supplementary Figure 5. Analysis of the clonogenic potential, discriminating between GM-CFU (A) and E-BFU (B) colonies, of CD34+ cells transduced with DKC1-shRNA LVs and scrambled shRNA-LVs (n=8). Data are expressed as mean ± SEM. Asterisks indicate significant differences determined by Student’s t test (*p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001). Supplementary Figure 6. Gating strategy and analysis of the NSG mice repopulating potential of CD34+ cells transduced with iDKC1 and scrambled-shRNA LVs. Representative dot-plots of flow cytometry analyses performed in the bone marrow samples from two mice transplanted with scrambled-shRNA LVs are shown. Supplementary Figure 7. Analysis of the VCNs in the bone marrow of recipient NSG mice at 3 months post-transplantation. NSG mice were transplanted with scrambled transduced CD34+ cells (orange dots, n=14) or iDKC1 interfered CD34+ cells (blue dots, n=8)

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Carrascoso-Rubio, C., Zittersteijn, H.A., Pintado-Berninches, L. et al. Generation of dyskeratosis congenita-like hematopoietic stem cells through the stable inhibition of DKC1. Stem Cell Res Ther 12, 92 (2021). https://doi.org/10.1186/s13287-021-02145-8

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Keywords

  • Dyskeratosis congenita
  • DKC1 gene
  • Bone marrow failure disorders
  • Hematopoietic stem cells
  • Short hairpin RNA
  • Lentiviral vectors