Resistance to hepcidin is conferred by hemochromatosis-associated mutations of ferroportin

Hal Drakesmith, Lisa M. Schimanski, Emma Ormerod, Alison T. Merryweather-Clarke, Vip Viprakasit, Jon P. Edwards, Emma Sweetland, Judy M. Bastin, Diana Cowley, Yingyong Chinthammitr, Kathryn J. H. Robson, and Alain R. M. Townsend

Ferroportin (FPN) mediates iron export from cells; FPN mutations are associated with the iron overloading disorder hemochromatosis. Previously, we found that the A77D, V162del, and G490D mutations inhibited FPN activity, but that other disease-associated FPN variants retained full iron export capability. The peptide hormone hepcidin inhibits FPN as part of a homeostatic negative feedback loop. We measured surface expression and func-


tion of wild-type FPN and fully active FPN mutants in the presence of hepcidin. We found that the Y64N and C326Y mutants of FPN are completely resistant to hepcidin inhibition and that N144D and N144H are partially resistant. Hemochromatosisassociated FPN mutations, therefore, either reduce iron export ability or produce an FPN variant that is insensitive to hepcidin. The former mutation type is associated with Kupffer-cell iron deposition and normal transferrin saturation in vivo, whereas patients with the latter category of FPN mutation have high transferrin saturation and tend to deposit iron throughout the liver parenchyma. FPN-linked hemochromatosis may have a variable pathogenesis depending on the causative FPN mutant. (Blood. 2005;106: 1092-1097)

© 2005 by The American Society of Hematology

Hereditary hemochromatosis is an iron overload disease characterized by excessive body iron that causes tissue damage in the liver, pancreas, and heart.In whites hemochromatosis is predominantly associated with 2 mutations in the HFE gene.Non-HFE hemochromatosis is geographically more widespread and results from mutations in other genes involved in iron homeostasis.Numerous mutations in the ferroportin gene have been reported in hemochromatosis patients from diverse origins.3-20 Ferroportin (FPN) transports iron out of cells and is strongly expressed by intestinal enterocytes and liver macrophages (Kupffer cells).21-23 FPN is inhibited by the peptide hormone hepcidin.24,25 Hepcidin levels correlate with iron stores, so that as body iron increases hepcidin is induced,26blocking FPN-mediated iron transfer from the diet by enterocytes and FPN-mediated iron recycling from erythrocytes by macrophages.This negative feedback loop is thought to maintain iron homeostasis.

We previously found that some hemochromatosis-associated FPN mutations (A77D, V162del, and G490D) showed reduced iron export, but other disease-related mutants, Y64N, N144D, N144H, Q248H, and C326Y, maintained full function in vitro.27 We postulated that those functioning FPN mutants might resist negative feedback, and the resulting disturbance in iron homeostasis might lead to hemochromatosis. In this paper we report that some of the hemochromatosis-associated FPN mutations are resistant to inhibition by hepcidin and discuss the implications of this finding for the pathogenesis of hemochromatosis and iron homeostasis in general.

Materials and methods

Expression vectors

pcDNA3.1 constructs encoding wild-type (wt) human and murine FPN c-terminally tagged with c-Myc-poly-histidine were kind gifts from Dr A. McKie (King’s College, London, United Kingdom) and mutated as described.27 A plasmid encoding human CD8 was a kind gift from Dr G. Gao (Oxford, United Kingdom), and a plasmid encoding green fluorescent protein (GFP) was a kind gift from Dr X. Xu (Oxford, United Kingdom).

Two-color flow cytometry

Human embryonic kidney epithelial 293T cells were exposed to DNAeffectene (Qiagen, Valencia, CA) transfection complexes for 8 hours as described27; then hepcidin-25 (the 25-amino acid form of hepcidin; Peptide Institute, Osaka, Japan) was added to half the wells at 0.5 fM. Two days later cells were harvested and incubated with anti–c-Myc–fluorescein isothiocyanate (FITC; Santa Cruz Biotechnology, Santa Cruz, CA) or anti–CD8-FITC (PharMingen, San Diego, CA) and anti–transferrin receptor 1 (TfR1)–biotin (PharMingen); mouse anti–rabbit immunoglobulin (MR12 clone; Dako, Glostrup, Denmark) was used as a negative control. Cells were then incubated with streptavidin-phycoerythrin (Sigma, St Louis, MO) to reveal TfR1 and analyzed using a Becton Dickinson (Mountain View, CA) FACScalibur as described.27 Transfected cells positive for CD8 or c-Myc were gated, and their surface TfR1 expression measured.


293T cells grown on 8-well chamber slides (BD Falcon, Oxford, United Kingdom) were transfected with wt or mutant FPN. Twenty-four hours

From the Weatherall Institute of Molecular Medicine, Oxford, United Kingdom; Medical Research Council Molecular Haematology Unit, Weatherall Institute of Molecular Medicine, Oxford, United Kingdom; Department of Paediatrics, Faculty of Medicine, Siriraj Hospital, Mahidol University, Bangkok, Thailand; and Department of Internal Medicine, Faculty of Medicine, Siriraj Hospital, Mahidol University, Bangkok, Thailand.

H.D., L.M.S., J.P.E., E.S., J.M.B., D.C., and A.R.M.T. supported by the Wellcome Trust Programme Grant no. 060542/2/00.

Submitted February 9, 2005; accepted April 1, 2005. Prepublished online as Blood First Edition Paper, April 14, 2005; DOI 10.1182/blood-2005-02-0561.

H.D. and L.M.S. contributed equally to this work.

Reprints: Hal Drakesmith, Weatherall Institute of Molecular Medicine, Oxford. OX3 9DS, United Kingdom; e-mail: [email protected]

The publication costs of this article were defrayed in part by page charge payment. Therefore, and solely to indicate this fact, this article is hereby marked ‘‘advertisement’’ in accordance with 18 U.S.C. section 1734.

© 2005 by The American Society of Hematology


later, cycloheximide was added to all wells at 100 fg/mL to inhibit protein synthesis and 2 hours later hepcidin-25 was added to half the wells at 0.5 fM. Three hours after adding hepcidin-25, cells were fixed, permeabilized, stained with anti–c-Myc–FITC, and processed for imaging as described.27

59Fe accumulation and 59Fe release

For iron accumulation, 293T cells were incubated with DNA-Effectene complexes for 8 hours, then 40 fg/mL 59Fe-labeled human transferrin (Tf), prepared as described27,28 was added to the cultures, and hepcidin-25 at 0.5 fM was added to half the wells. Forty hours later iron accumulation per million cells was determined as described.28 For iron release, 293T cells were preloaded with 40 fg/mL 59Fe-Tf for 24 hours before being transfected with GFP, wt FPN, or C326Y FPN for 15 hours. Cells were then harvested and 59Fe per million cells was determined before reculturing the cells in serum-free medium (Pro293a-CDM; BioWhittaker, Walkersville, MD) with or without hepcidin-25 at 0.5 fM. The percentage 59Fe export at various time points was calculated as 59Fe in the supernatant at each time point divided by cellular 59Fe at time 0 multiplied by 100.

Ferritin ELISA

Total cellular ferritin was measured from cell lysates using ferritin enzyme-linked immunosorbent assay (ELISA) kits (Laguna Scientific, Laguna Niguel, CA) as described.27 Cells were transfected in the presence of 1 mg/mL human holo-Tf (Sigma) with or without hepcidin-25 at 0.5 fM. After culturing for 3 days, cells were lysed and the protein content of lysates was measured using the Bradford assay (Bio-Rad, Hercules, CA), and normalized by diluting with lysis buffer as necessary. Then, 20 fL doubling dilutions were used per well in the ferritin ELISA and compared against provided ferritin standards.


Hepcidin reduces surface expression of wt FPN but not of FPN mutants

Hepcidin causes internalization of FPN and so reduction of surface expression.24 We wondered if hemochromatosis-associated FPN mutants might resist hepcidin-mediated internalization. To test this we transiently transfected 293T cells with constructs encoding c-terminally c-Myc–tagged wt human FPN, wt murine FPN, and the human FPN variants Y64N, N144D, N144H, Q248H, and C326Y, with or without added hepcidin-25. After 2 days, cells were analyzed for surface expression of the c-Myc tag by flow cytometry (Figure 1A-C). Figure 1A shows a reduction in surface c-Myc expression mediated by hepcidin-25 in cells expressing wt human

Figure 1. Down-regulation of surface wt FPN-c-Myc but not of mutant FPN-c-Myc by hepcidin-25. (A-B) 293T cells were transiently transfected with either c-Myc–tagged wt FPN (A) or c-Myc–tagged C326Y FPN (B) for 2 days with or without 0.5 fM hepcidin-25 (Hep) added. Cells were then stained for surface expression of c-Myc and analyzed by flow cytometry. In the case of wt FPN, hepcidin-25 caused a reduction of detectable cell-surface c-Myc (green line versus red line in panel A), but no reduction of C326Y-c-Myc tag by hepcidin-25 was observed (B). The blue-filled histogram represents the fluorescence of cells stained with an isotype control antibody (anti–CD8-FITC). (C) Quantitation of down-regulation of FPN and FPN mutants by hepcidin-25. Cells were transfected with c-Myc–tagged FPN and FPN mutants with or without added hepcidin-25 and stained for surface c-Myc then analyzed as described in panels A and B. The MFI of the different populations was calculated using CellQuest (BD) software and is displayed as a percentage of the MFI of wt human FPN without added hepcidin-25. Hepcidin-25 reduced surface wt human and murine FPN and Q248H surface expression by at least a half; surface C326Y and Y64N was not affected by hepcidin-25; and N144D and N144H were partially down-regulated. (D) Cells were transfected with c-Myc–tagged FPN and FPN mutants for 24 hours, protein synthesis was inhibited with cycloheximide for 2 hours, and then 0.5 fM hepcidin-25 was added to half the wells for 3 further hours. Cells were then stained for c-Myc expression (green) and cell nuclei were stained by DAPI (blue). Without added hepcidin all FPN variants were localized to plasma membranes (first and third columns from left). In the presence of hepcidin, wt and Q248H FPN were internalized into discrete vesicles, whereas C326Y and Y64N FPN protein remained at the cell surface and both internalized and surface N144D and N144H were observed (second and fourth columns). These results are representative of 3 experiments.

FPN (compare green histogram to red), consistent with the internalization of murine FPN reported by Nemeth et al.24 In contrast hepcidin-25 had no effect on the surface expression of the c-Myc–tagged FPN variant C326Y (Figure 1B). Figure 1C shows the effect of hepcidin-25 on all FPN mutants analyzed, displayed as the percentage surface expression relative to wt human FPN levels in the absence of hepcidin-25. Surface wt human and mouse FPN expression was reduced by over a half by hepcidin-25, C326Y and Y64N were resistant to hepcidin-mediated down-regulation, N144D and N144H were partially resistant, and Q248H was as susceptible to down-regulation as wt FPN. In agreement with Nemeth et al, we found that a preparation of hepcidin-20, the 20-amino acid form of hepcidin, did not reduce surface expression of wt FPN (data not shown).24 We then visualized FPN redistribution by hepcidin-25 using immunofluorescence microscopy. 293T cells transfected with wt human FPN and FPN variants for 24 hours were incubated with cycloheximide (to stop de novo protein synthesis) with or without added hepcidin-25. Cells were then stained for FPN expression using anti–c-Myc antibody (Figure 1D green) and cell nuclei were counterstained using DAPI (4,6 diamidino-2-phenylindole; Figure 1D blue). For all FPN variants, without hepcidin-25 added FPN protein was localized to the plasma membranes. Hepcidin-25 caused internalization of wt FPN into discrete vesicles as previously reported.24 C326Y and Y64N FPN resisted internalization by hepcidin-25 and remained at the cell surface, whereas Q248H was internalized in the same way as wt FPN. The N144 mutants had an intermediate phenotype, with both cell surface and internalized protein apparent.

Hepcidin inhibits the FPN-mediated increase in surface TfR-1 and reduction in ferritin, but FPN mutants are not inhibited

Next we evaluated the effect of hepcidin-25 on the function of FPN and disease-associated FPN variants. FPN expression causes cellular iron deficiency and a reduction in the labile iron pool,21 leading to reduced ferritin and increased surface expression of TfR1. We expressed wt FPN and FPN variants in 293T cells with or without added hepcidin-25 and measured surface TfR on transfected cells using 2-color flow cytometry. As a control, we used cells transfected with CD8, a molecule with no known function in iron transport; hepcidin-25 had no effect on TfR expression by untransfected cells or CD8 transfected 293T cells (data not shown). Figure 2A shows that wt human FPN expression increases surface TfR compared with control CD8-expressing cells (compare red line to filled gray histogram) and that hepcidin-25 inhibits this FPN-mediated TfR increase (green line is similar to filled gray histogram). The Y64N FPN variant similarly increases surface TfR relative to control cells (Figure 2B, red line compared with filled gray histogram), but this increase in TfR is not affected by hepcidin-25 (green line is similar to red line). The effect of hepcidin-25 on all FPN variants is shown in Figure 2C. The mean fluorescence intensity (MFI) of TfR on cells transfected with FPN variants (with or without added hepcidin-25) minus the MFI of TfR on control CD8-transfected cells is given. The wt human and mouse FPN increase TfR levels above those of control cells, but hepcidin-25 blocks this increase, whereas hepcidin-25 did not hinder the increase of TfR mediated by C326Y and Y64N FPN. N144D and N144H are partially susceptible to hepcidin-25 inhibition, whereas Q248H is blocked by hepcidin-25 to the same degree as wt FPN. Levels of the intracellular iron storage protein ferritin are also reduced by FPN expression. We found that the reduction in ferritin caused by FPN was inhibited by hepcidin-25, but the C326Y-mediated ferritin reduction was unaffected by hepcidin-25

Figure 2. Hepcidin-25 inhibits TfR up-regulation and ferritin reduction caused by wt FPN but not by mutant FPN. (A-B) 293T cells were transiently transfected with either c-Myc–tagged wt FPN (A) or c-Myc–tagged Y64N FPN (B) for 2 days with or without 0.5 fM hepcidin-25 added. Cells were then stained simultaneously for surface expression of c-Myc and TfR and analyzed by flow cytometry. Transfected cells (c-Myc+ cells) were gated on and their TfR expression is displayed relative to the TfR expressed by control CD8-transfected cells. The wt FPN expression caused an increase in TfR expression compared with control cells (compare red line with gray histogram in panel A) consistent with FPN causing iron deficiency; coculture with hepcidin-25 reverses the effect of wt FPN (green line is similar to gray filled histogram in panel A). In contrast the up-regulation of TfR by Y64N (compare red line with gray filled histogram in panel B) is not counteracted by coculture with hepcidin-25 (green line is similar to red line in panel B). The blue-filled histogram represents the fluorescence of cells stained with an isotype control antibody (anti–rabbit IgG). (C) Quantitation of inhibition of FPN and FPN mutant-mediated up-regulation of TfR by hepcidin-25. Cells were transfected with c-Myc–tagged FPN and FPN mutants with or without added hepcidin-25 and stained for surface c-Myc and TfR then analyzed as described in panels A and B. The MFI of the different populations was calculated using CellQuest software and is displayed with the MFI of the TfR expressed by control CD8-transfected cells subtracted. The increase of TfR expression induced by wt human, wt murine, and Q248H FPN is counteracted by hepcidin-25, whereas the TfR increase mediated by C326Y and Y64N FPN was resistant to hepcidin-25 inhibition, and the raised TfR due to N144D and N144H expression was partially reduced by hepcidin-25. (D) 293T cells were transfected with wt FPN or C326Y FPN in the presence of 1 mg/mL human holo-Tf to increase background ferritin levels, and with or without added hepcidin-25. Cells were transfected with CD8 as a control. After 2 days cells were analyzed for ferritin levels by ELISA. Cells were lysed in NP40 at 107cells/mL, doubling dilutions were made, and 20 fL transferred to ELISA plate in triplicate. Graph shows mean total ferritin in nanograms per 107 cells (± 95% CI). Cells transfected with wt FPN have around 40 ng ferritin/107cells, a 3-fold reduction compared with control cells transfected with CD8. Coculture with hepcidin-25 completely reverses the effect of wt FPN, but hepcidin-25 has no effect on the reduction of ferritin mediated by C326Y FPN. These results are representative of 3 experiments. Horizontal bars indicate mean values.

Figure 3. Effects of hepcidin on FPN and mutant FPN-mediated changes in iron accumulation and iron release. (A-B) Effect of hepcidin-25 on iron accumulation by FPN and FPN mutant-expressing cells. Cells were transfected with FPN and FPN mutants and cultured with 40 fg/mL 59Fe-Tf with or without 0.5 fM hepcidin-25 added for 2 days, and then cellular 59Fe accumulation per million cells was determined. Hepcidin did not alter 59Fe accumulation by control CD8-transfected cells. Expression of FPN and all FPN variants reduced iron accumulation, consistent with enhanced iron export by transfected cells. Hepcidin-25 reversed the effect of wt and Q248H FPN but did not inhibit C326Y or Y64N FPN and only marginally increased iron accumulation by cells expressing N144D and N144H FPN. Each point represents the iron accumulation by one aliquot of a million cells. Red bar shows mean 59Fe accumulation (± 95% CI). *Significance compared with CD8 control (P < .001 by Student t test). (C) Hepcidin-25 inhibits iron release from cells expressing wt FPN but not C326Y FPN. 293T cells were preloaded with 59Fe, then transfected for 15 hours, washed, and recultured in serum-free medium and the percentage 59Fe released (of starting) was measured over 32 hours. Hepcidin does not affect “background” release from control 293T cells transfected with GFP (or CD8, not shown). Data shown are representative of 2 or more experiments for each mutant.

(Figure 2D). Thus, cellular iron deficiency, caused by FPN and leading to increases in TfR1 and lowering of ferritin, is inhibited by hepcidin. Hemochromatosis-associated mutants of FPN also cause cellular iron deficiency but are not restrained by hepcidin.

Hepcidin inhibits FPN-mediated changes in cellular iron accumulation and iron release, but FPN mutants are not inhibited

Next, we directly measured the effect of hepcidin-25 on iron accumulation by cells. 293T cells were transfected with FPN variants and cultured for 2 days with 40 fg/mL 59Fe-labeled human with or without added hepcidin-25 (Figure 3A-B). 59Fe accumulation by control CD8-transfected cells was unaffected by hepcidin

25. The wt human FPN expression caused a marked decrease in iron accumulation that was largely reversed in the presence of hepcidin-25, and this same effect was observed with cells expressing Q248H FPN. In contrast the reduction in 59Fe accumulation by cells expressing Y64N or C326Y was resistant to hepcidin-25, and hepcidin-25 only marginally counteracted the lower 59Fe accumulation displayed by cells expressing N144D and N144H. Finally, we directly measured 59Fe release from cells transfected with wt FPN or C326Y FPN with or without added hepcidin. Figure 3C shows that wt and C326Y FPN increased iron release compared with control GFP-transfected cells, and that hepcidin inhibited the 59Fe efflux mediated by wt FPN but not C326Y FPN. We conclude from the data shown in Figures 1-3 that wt FPN is internalized and functionally restrained by hepcidin-25 but that the hemochromatosisassociated FPN mutations, Y64N, N144D, N144H, and C326Y, confer total or partial resistance to hepcidin inhibition.


In our earlier investigation we found that A77D, V162del, and G490D FPN mutants lost iron export function, whereas the other FPN mutants that are the subject of this report maintained efflux ability.27 We postulated that this second set of mutants could cause hemochromatosis if they resisted a natural inhibitor of FPN that was involved in iron homeostasis. We proposed 2 possible candidate inhibitors, HFE or hepcidin.29 HFE reduces iron export from


cell types that naturally express but in our hands HFE does not inhibit FPN under the same experimental conditions as for Figure 3C (data not shown); thus the role of HFE remains enigmatic.

Hepcidin was recently reported to induce FPN internalization and degradation.24 Our results are consistent with these findings, and we show that both murine and human wt FPN are equally subject to human hepcidin-25 inhibition. We found that Q248H FPN was as susceptible to hepcidin as wt FPN; although Q248H has been found in some iron-loaded individuals, it is present at high frequency in some African populations and can occur in homozygosity.10,11,15 Q248H may be a polymorphism with a mild effect on FPN function that we could not detect, possibly leading to disease in the presence of modifying factors.

We found that the hemochromatosis-associated FPN mutants Y64N, N144D, N144H, and C326Y, which export iron as well as wt FPN, had abolished or reduced sensitivity to inhibition by hepcidin. In vivo, an FPN protein that cannot be turned off by hepcidin could lead to higher dietary iron uptake and more iron recycling from red cells by macrophages, resulting in high serum Tf saturation. We previously showed that the A77D, V162del, and G490D FPN mutants had lost iron export ability in vitro.27 Patients with these mutations may have reduced iron export from their macrophages leading to Kupffer-cell iron loading without high Tf saturation; characteristics (along with high serum ferritin) of the “ferroportin disease.”31

To investigate any potential relationship between FPN mutant activity in vitro and in vivo disease phenotype, we searched the literature describing clinical features of hemochromatosis patients with “loss-of-function” or “hepcidin-resistant” FPN mutations. We plotted age versus Tf saturation (Figure 4A) and age versus serum ferritin (Figure 4B) from the values in the published studies. Figure 4A shows that patients with the FPN mutations that we have shown to be fully functional but completely hepcidin resistant (Y64N and C326Y) have markedly high Tf saturation. A second mutation at C326, C326S, was recently reported in family members with high Tf saturation before the age of 20.17 Although we have not tested C326S, it is at least possible that like C326Y, this FPN variant is also resistant to hepcidin. Patients with the FPN variants that have lost iron export function in vitro, V162del, G490D, and A77D, have generally normal Tf saturation, although Tf saturation rises with the age of individuals with A77D. Patients with mutations at N144 (that in vitro have active export ability but only partial sensitivity to hepcidin) have an intermediate phenotype, having

Figure 4. Age versus Tf saturation and age versus serum ferritin in patients with FPN-linked hemochromatosis. Values for Tf saturation (A) and serum ferritin (B) were obtained for hemochromatosis patients with the FPN mutants indicated from the specified references. The in vitro behavior of the different FPN mutants is also shown. *Data for C326Y obtained by V.V., A.T.M-C., Y.C., and K.J.H.R. †We have not tested the in vitro function of C326S or N144T.

either high Tf saturation or Tf saturation in the normal range. Thus, Figure 4A shows that our in vitro functional studies categorizing FPN mutants as either loss-of-function or hepcidin resistant have an in vivo correlate with Tf saturation in patients with hemochromatosis. The distinction is not so clear when serum ferritin is plotted against age (Figure 4B). All individuals with the exception of 2 Y64N and 3 C326S patients have raised serum ferritin levels. Serum ferritin levels increase with age for all mutations but may have a higher “start point” for the loss-of-function mutations A77D, V162del, and G490D.

The loss-of-function FPN mutations are clearly associated with predominantly macrophage (Kupffer cell) iron loading in the liver in vivo.5-8,12,18 The pattern of iron deposition in the livers of patients harboring FPN mutations that we have described as hepcidin resistant is more variable. Heavy iron deposition in both hepatocytes and Kupffer cells was reported in individuals with Y64N FPN,13 whereas iron deposition is predominantly in hepatocytes in C326Y patients and also C326S patients.17 There is variation in deposition of iron in patients with mutations at N144 (that confers partial resistance to hepcidin), with iron in either hepatocytes or with a reticuloendothelial distribution.9,14,19

Thus, overall, FPN mutations that have lost iron export capacity in vitro are associated generally with normal Tf saturation (with the exception of older patients with A77D), Kupffer-cell iron loading, and high serum ferritin even at a young age. In contrast, mutations conferring total hepcidin resistance in vitro are linked to markedly high Tf saturation, a pattern of liver iron deposition that includes


and may be predominantly in hepatocytes, and occasionally lower serum ferritin at least early in disease. However, there is variation among family members with the same mutations, perhaps most clearly apparent in patients with mutations at N144 (intermediate phenotype in vitro), which suggests that other factors likely exist that modify the clinical picture.

A final point of interest is that 2 individuals carrying the loss-of-function V162del mutation were recently found to have high levels of hepcidin.32 Iron overload caused by loss-of-function FPN mutations (80 g iron was removed from one V162del patient8) has been proposed to result from iron locked in macrophages being withheld from the bone marrow. The erythron then sends compensatory signals to the intestine to up-regulate iron absorption. The high hepcidin levels found in the V162del patients raises the possibility that this putative bone marrow-to-intestine signal could be hepcidin independent.

In summary, we have found that some hemochromatosisassociated mutations of FPN confer resistance to inhibition by hepcidin in vitro. These mutations are linked to a clinical phenotype that differs from those patients harboring loss-of-function FPN mutations most notably in terms of higher Tf saturation. Hepcidin-resistant FPN may be associated with a greater flow of iron through the erythrocyte iron recycling pathway as well as with increased intestinal iron absorption. Patients harboring hepcidinresistant FPN alleles may in consequence be expected to mobilize iron on phlebotomy more readily than those individuals with loss-of-function FPN mutants.

  1. Pietrangelo A. Hereditary hemochromatosis: a new look at an old disease. N Engl J Med. 2004; 350:2383-2397.
  2. Feder JN, Gnirke A, Thomas W, et al. A novel MHC class I-like gene is mutated in patients with hereditary haemochromatosis. Nat Genet. 1996; 13:399-408.
  3. Robson KJ, Merryweather-Clarke AT, Cadet E, et al. Recent advances in understanding haemochromatosis: a transition state. J Med Genet. 2004;41:721-730.
  4. Njajou OT, Vaessen N, Joosse M, et al. A mutation in SLC11A3 is associated with autosomal dominant hemochromatosis. Nat Genet. 2001;28: 213-214.
  5. Montosi G, Donovan A, Totaro A, et al. Autosomal-dominant hemochromatosis is associated

with a mutation in the ferroportin (SLC11A3) gene. J Clin Invest. 2001;108:619-623.

  1. Devalia V, Carter K, Walker AP, et al. Autosomal dominant reticuloendothelial iron overload associated with a 3-base pair deletion in the ferroportin 1 gene (SLC11A3). Blood. 2002;100:695-697.
  2. Roetto A, Merryweather-Clarke AT, Daraio F, et al. A valine deletion of ferroportin 1: a common mutation in hemochromastosis type 4. Blood. 2002; 100:733-734.
  3. Wallace DF, Pedersen P, Dixon JL, et al. Novel mutation in ferroportin1 is associated with autosomal dominant hemochromatosis. Blood. 2002; 100:692-694.
  4. Arden KE, Wallace DF, Dixon JL, et al. A novel mutation in ferroportin1 is associated with haemochromatosis in a Solomon Islands patient. Gut. 2003;52:1215-1217.
  1. Barton JC, Acton RT, Rivers CA, et al. Genotypic and phenotypic heterogeneity of African Americans with primary iron overload. Blood Cells Mol Dis. 2003;31:310-319.
  2. Gordeuk VR, Caleffi A, Corradini E, et al. Iron overload in Africans and African-Americans and a common mutation in the SCL40A1 (ferroportin 1) gene. Blood Cells Mol Dis. 2003;31:299-304.
  3. Jouanolle AM, Douabin-Gicquel V, Halimi C, et al. Novel mutation in ferroportin 1 gene is associated with autosomal dominant iron overload. J Hepatol. 2003;39:286-289.
  4. Rivard SR, Lanzara C, Grimard D, et al. Autosomal dominant reticuloendothelial iron overload (HFE type 4) due to a new missense mutation in the FERROPORTIN 1 gene (SLC11A3) in a large French-Canadian family. Haematologica. 2003; 88:824-826.
  1. Wallace DF, Clark RM, Harley HA, Subramaniam VN. Autosomal dominant iron overload due to a novel mutation of ferroportin1 associated with parenchymal iron loading and cirrhosis. J Hepatol. 2004;40:710-713.
  2. Beutler E, Barton JC, Felitti VJ, et al. Ferroportin 1 (SCL40A1) variant associated with iron overload in African-Americans. Blood Cells Mol Dis. 2003;31:305-309.
  3. Pietrangelo A, Montosi G, Totaro A, et al. Hereditary hemochromatosis in adults without pathogenic mutations in the hemochromatosis gene. N Engl J Med. 1999;341:725-732.
  4. Sham RL, Phatak PD, West C, Lee P, Andrews C, Beutler E. Autosomal dominant hereditary hemochromatosis associated with a novel ferroportin mutation and unique clinical features. Blood Cells Mol Dis. 2005;34:157-161.
    1. Cazzola M, Cremonesi L, Papaioannou M, et al. Genetic hyperferritinaemia and reticuloendothelial iron overload associated with a three base pair deletion in the coding region of the ferroportin gene (SLC11A3). Br J Haematol. 2002;119:539
    2. 546.
  5. Njajou OT, de Jong G, Berghuis B, et al. Dominant hemochromatosis due to N144H mutation of SLC11A3: clinical and biological characteristics. Blood Cells Mol Dis. 2002;29:439-443.
  1. Njajou OT, Vaessen N, Oostra B, Heutink P, Van Duijn CM. The hemochromatosis N144H mutation of SLC11A3 gene in patients with type 2 diabetes. Mol Genet Metab. 2002;75:290-291.
  2. Abboud S, Haile DJ. A novel mammalian iron-regulated protein involved in intracellular iron metabolism. J Biol Chem. 2000;275:19906-19912.
  3. Donovan A, Brownlie A, Zhou Y, et al. Positional cloning of zebrafish ferroportin1 identifies a conserved vertebrate iron exporter. Nature. 2000; 403:776-781.
  4. McKie AT, Marciani P, Rolfs A, et al. A novel duodenal iron-regulated transporter, IREG1, implicated in the basolateral transfer of iron to the circulation. Mol Cell. 2000;5:299-309.
  5. Nemeth E, Tuttle MS, Powelson J, et al. Hepcidin regulates iron efflux by binding to ferroportin and inducing its internalization. Science. 2004;306: 2051-2053.
  6. Knutson MD, Oukka M, Koss LM, Aydemir F, Wessling-Resnick M. Iron release from macro-phages after erythrophagocytosis is up-regulated by ferroportin 1 overexpression and down-regulated by hepcidin. Proc Natl Acad Sci U S A. 2005;102:1324-1328.
  7. Courselaud B, Pigeon C, Inoue Y, et al. C/EBPalpha regulates hepatic transcription of hepcidin,

an antimicrobial peptide and regulator of iron metabolism. Cross-talk between C/EBP pathway and iron metabolism. J Biol Chem. 2002;277: 41163-41170.

  1. Schimanski LM, Drakesmith H, Merryweather-Clarke AT, et al. In vitro functional analysis of human ferroportin (FPN) and hemochromatosisassociated FPN mutations. Blood. 2005;105: 4096-4102.
  2. Drakesmith H, Sweetland E, Schimanski L, et al. The hemochromatosis protein HFE inhibits iron export from macrophages. Proc Natl Acad Sci U S A. 2002;99:15602-15607. Epub 12002 Nov 15612.
  3. Townsend A, Drakesmith H. Role of HFE in iron metabolism, hereditary haemochromatosis, anaemia of chronic disease, and secondary iron overload. Lancet. 2002;359:786-790.
  4. Davies PS, Enns CA. Expression of the hereditary hemochromatosis protein HFE increases ferritin levels by inhibiting iron export in HT29 cells. J Biol Chem. 2004;279:25085-25092.
  5. Pietrangelo A. The ferroportin disease. Blood Cells Mol Dis. 2004;32:131-138.
  6. Papanikolaou G, Tzilianos M, Christakis JI, et al. Hepcidin in iron overload disorders. Blood. 2005; 105:4103-4105.