Research ArticlePhysiology

The mTORC1/4E-BP pathway coordinates hemoglobin production with L-leucine availability

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Sci. Signal.  14 Apr 2015:
Vol. 8, Issue 372, pp. ra34
DOI: 10.1126/scisignal.aaa5903

Red cells need leucine to make hemoglobin

Inhibitors of the protein complex mTORC1 are used in the clinic, but they can cause anemia. Limitation of nutrients, such as amino acids, inhibits mTORC1 activity, which reduces protein synthesis by enhancing the activity of the translation inhibitor protein 4E-BP. The oxygen-carrying protein complex hemoglobin in red blood cells contains globin proteins, which have a particularly high percentage of leucine residues, leading Chung et al. to investigate the role of mTORC1 in hemoglobin production. Deficiency or inhibition of LAT3, an uptake transporter for l-leucine, prevented hemoglobin production in zebrafish and mouse red blood cells. Inadequate l-leucine uptake prevented the translation of globin-encoding transcripts. Thus, red cell function critically depends on leucine availability.


In multicellular organisms, the mechanisms by which diverse cell types acquire distinct amino acids and how cellular function adapts to their availability are fundamental questions in biology. We found that increased neutral essential amino acid (NEAA) uptake was a critical component of erythropoiesis. As red blood cells matured, expression of the amino acid transporter gene Lat3 increased, which increased NEAA import. Inadequate NEAA uptake by pharmacologic inhibition or RNAi-mediated knockdown of LAT3 triggered a specific reduction in hemoglobin production in zebrafish embryos and murine erythroid cells through the mTORC1 (mammalian target of rapamycin complex 1)/4E-BP (eukaryotic translation initiation factor 4E–binding protein) pathway. CRISPR-mediated deletion of members of the 4E-BP family in murine erythroid cells rendered them resistant to mTORC1 and LAT3 inhibition and restored hemoglobin production. These results identify a developmental role for LAT3 in red blood cells and demonstrate that mTORC1 serves as a homeostatic sensor that couples hemoglobin production at the translational level to sufficient uptake of NEAAs, particularly l-leucine.


Amino acids are the fundamental building blocks of all proteins. Clinically, targeting amino acid metabolism is gaining increasing prominence as a treatment modality for several human diseases (14), highlighting the need for a more thorough basic understanding of amino acid metabolism in normal physiology. For most eukaryotes that lack the ability to produce essential amino acids (EAA) de novo, transport mechanisms are required for uptake of EAAs from the extracellular milieu (5). There are several classes of EAA transporters, one of which is the system L (“leucine preferring”) family that consists of four members—LAT1 (SLC7A5), LAT2 (SLC7A6), LAT3 (SLC43A1), and LAT4 (SLC43A2) (68). LAT1 and LAT2 have broader substrate specificity and require the CD98 (SLC3A2) cotransporter for function, whereas LAT3 and LAT4 are monomeric facilitative uniporters with greater affinity for the transport of branched, neutral essential amino acids (NEAAs), particularly l-leucine (6, 7, 9, 10). To date, the vast majority of work has focused on unravelling LAT1 function (7, 1114), and little is known regarding the roles of other LAT-family proteins in normal development (6).

Eukaryotic cells adapt to insufficient EAA uptake by altering their cellular metabolism (5). One such mechanism, which was first identified in yeast and later in mammals, involves the activation of the kinase GCN2 (general control nonderepressible 2) by uncharged tRNAs (transfer RNAs) under severe amino acid deprivation (1517). Active GCN2 inhibits eIF2α (eukaryotic initiation factor 2α) by phosphorylating Ser51, thereby decreasing global translation initiation (1820). Paradoxically, phosphorylated eIF2α also triggers the translation of a subset of mRNAs including Atf4 (15, 16, 21, 22), which encodes a transcription factor that induces the expression of genes involved in amino acid metabolism to increase amino acid availability (19, 23). The serine/threonine kinase mTORC1 (mammalian target of rapamycin complex 1) constitutes a second pathway that is responsive to amino acid stress, particularly l-leucine deficiency (2426). Under nutrient-rich conditions, mTORC1 is active and phosphorylates various downstream proteins that mediate anabolic metabolism including activation of protein translation (2429). When nutrient pools, particularly l-leucine, become depleted, mTORC1 activity diminishes, triggering cellular catabolism (3, 2426). Although mTORC1 activity can be modulated by l-leucine–loaded leucyl-tRNA synthetase (30, 31), it is also sensitive to changes in the intracellular l-leucine pool (24, 25). This indicates that a hierarchy exists in amino acid stress responses such that mTORC1 responds to variations in amino acid pools, particularly l-leucine, whereas GCN2 is only engaged under general severe starvation conditions.

Efforts to decipher mTORC1 translation control have relied on pharmacologic and genetic loss-of-function approaches (27, 28, 32). However, such pronounced deficiencies in mTORC1 activity are unlikely to be encountered physiologically and does not accurately reflect feedback regulation of maintaining nutrient homeostasis. This is an essential consideration in understanding the physiologic role of mTORC1 signaling that may have a substantial impact on biological output (33). For example, phosphorylation of eIF2α inhibits the translation of most proteins (1820), but particularly that of globin transcripts in erythroid cells (34). This is largely due to feedback regulation of heme availability that signals to intricately balance α/β-globin protein translation to heme biosynthesis (34) and the vast number of globin proteins that comprise 97% of the erythroid proteome (35).

In humans, mutations in the translation machinery are associated with about 50% of Diamond-Blackfan anemias (DBAs), whereas the remaining anemias have unknown causes (3638). Modulation of the mTORC1 pathway has been reported to alleviate DBA symptoms in model organisms (39). Together, these results underscore not only the importance of translational regulation in erythropoiesis but also the need to better understand the dynamics of nutrient homeostasis. This knowledge can substantially affect human health by uncovering potentially new causes of disease as well as improved treatment options. Here, we show that red blood cell development requires increased NEAA uptake, and mTORC1 coordinates hemoglobin production with the availability of NEAAs, particularly that of l-leucine.


Erythropoiesis involves increased NEAA uptake through LAT3

As erythrocytes mature, their transcriptional profiles undergo changes that reflect an altered metabolic state, including the induction of iron and heme metabolism genes, as well as those involved in amino acid recycling (4043). The maintenance of amino acid homeostasis plays a critical role in erythropoiesis (42), highlighting how red blood cell development serves as an excellent framework for understanding the metabolic regulation of amino acid signaling during normal physiology. Using RNAseq (44, 45), we found that the expression of mRNAs encoding system L amino acid transporters, Lat1 (also known as Slc7a5) and Lat3 (also known as Slc43a1), was substantially increased in maturing red blood cells in a manner similar to mRNAs for other erythroid solute transporters such as Glut1 (also known as Slc2a1), Ae1 (also known as Slc4a1), and Mfrn1 (also known as Slc25a37); iron and heme metabolism genes such as Tfrc, Snx3, and Fech; and other erythroid-associated genes such as Hba-a1 (which encodes α-globin) and Hbb-b1 (which encodes β-globin) (Fig. 1A) (45). The transcript abundance of two closely related paralogs (6), Lat2 (also known as Slc7a6) and Lat4 (also known as Slc43a2), or that of the Tuba1a gene (which encodes the cytoskeletal protein β-tubulin) was relatively unchanged throughout erythroid maturation (Fig. 1A). We also did not detect expression of the mRNA encoding CD98 cotransporter requisite for LAT1-dependent transport, indicating that although LAT1 was induced, it was likely not functional. Thus, we focused our subsequent analysis on Lat3.

Fig. 1 Erythropoiesis involves increased NEAA uptake mediated by increased Lat3 expression.

(A) RNAseq gene expression analysis (accession number GSE32110) of fetal liver cells as they mature from R1 to R5 stages, showing induction of Lat3 mRNA with other terminal erythroid transcripts. CD98, the required cotransporter for LAT1 and LAT2, was not detected at any differentiation stage. (B and C) Lat3 mRNA expression was examined in the murine embryo at E14.5 by radiolabeled in situ hybridization (pseudo-colored red) (B) and in differentiating MEL cells by quantitative reverse transcription–polymerase chain reaction (RT-PCR) (C), showing enrichment of Lat3 mRNA in erythropoietic tissues and during erythroid maturation. (D) Lysates from undifferentiated and differentiating MEL cells induced with dimethyl sulfoxide (DMSO) at various days were immunoblotted with anti-LAT3 or anti-GAPDH antibodies. (E to I) The uptake of l-[3H]leucine was monitored over 4 min in the indicated MEL cell populations (E), in differentiating (day 3) control or stably Lat3 shRNA–expressing MEL cells (F to H), or in differentiating (day 3) MEL cells treated with the indicated nonradioactive amino acids (I). For (I), * denotes significant difference from MOCK treatment. (J) GC-MS analysis of maturing MEL cells stably expressing control or Lat3-targeting shRNAs. The percentage of each amino acid was normalized to the corresponding undifferentiated samples. *P < 0.05. Mean ± SEM, n = 3 independent experiments for (C), (E), (F), (H), (I), and (J). n = 2 embryos for (B). n = 2 independent experiments for (D) and (G). FL, fetal liver; IB, immunoblot; Undiff, undifferentiated; Diff, differentiated.

In situ hybridization performed on the developing murine embryo revealed broad expression of Lat3 at embryonic day (E) 8.5 with enrichment in erythropoietic blood islands of the yolk sac as well as the neural epithelium (fig. S1A) and high expression in the fetal liver, the site of definitive erythropoiesis, at E14.5 (Fig. 1B). The Lat3 expression pattern mirrors that of heme metabolism genes (46, 47). LAT3 transcript abundance was also increased in human CD34+ cells induced to differentiate along the erythroid lineage (fig. S1B). We also examined changes in Lat3 expression in differentiating Friend murine erythroleukemia (MEL) cells, which are committed erythroid cells that are used to study red blood cell maturation (48). Consistent with our observations in the murine embryo, the abundance of the mRNA and protein increased in terminally differentiating MEL cells (Fig. 1, C and D). Further analysis of chromatin immunoprecipitation–sequencing databases for the erythroid master transcription factors GATA1 and KLF1 revealed the presence of GATA1 (49) and KLF1 (50, 51) binding sites within intron 1 and the promoter of the murine Lat3 gene, respectively, suggesting that Lat3 is directly induced by erythroid master transcription factors during erythropoiesis.

Given the increase in Lat3 expression, we tested whether maturing red blood cells exhibited increased uptake of NEAAs. LAT3 most efficiently transports l-leucine compared to other substrates such as l-phenylalanine, l-isoleucine, l-valine, and l-methionine (9). Thus, we performed uptake assays using l-leucine as a representative amino acid. Differentiating MEL cells took up more l-[3H]leucine than did undifferentiated cells, an effect that was restored to basal amounts with 2-aminobicyclo-(1,2,2)-heptane-2-carboxylic acid (BCH) (Fig. 1E), a system L–specific plasma membrane inhibitor (6). BCH also partially blocked l-leucine uptake in differentiating primary murine fetal liver cells (fig. S1C). Stable knockdown of Lat3 expression with short hairpin RNAs (shRNAs) in maturing MEL cells similarly diminished but did not fully abrogate l-[3H]leucine import (Fig. 1, F to H). In contrast, competition assays showed that l-[3H]leucine uptake was markedly decreased by the addition of excess, nonradioactive l-leucine, partially decreased by the addition of other NEAAs, and not affected by d-leucine, l-glutamic acid, or l-glutamine (Fig. 1I), indicating that maturing erythroid cells have higher NEAA import mediated by increased expression of Lat3 but that basal transport relies on other mechanisms or transporters (6). Gas chromatography–mass spectrometry (GC-MS) analysis also demonstrated that intracellular concentrations of l-leucine as well as l-phenylalanine, l-valine, and l-isoleucine—all purported substrates of LAT3 (9)—were decreased in Lat3 shRNA–expressing erythroid cells that were differentiated (Fig. 1J), but not those that were undifferentiated (fig. S1D). However, our analysis of differentiating cells did not find any significant difference in l-methionine concentrations (Fig. 1J), consistent with a previous work showing that l-methionine is a relatively poor substrate, although it can efficiently outcompete LAT3-mediated transport of other NEAAs (9). In addition, undifferentiated, Lat3 shRNA–expressing cells showed no difference in l-[3H]leucine import from controls (fig. S1E). Together, our data indicate that increased LAT3-mediated NEAA import during red blood cell maturation is a component of developmental erythropoiesis.

Hemoglobin production is coupled to NEAA sufficiency

The increase in LAT3-mediated NEAA uptake in maturing erythroid cells prompted us to examine how cells adapt to amino acid stresses in vivo with the zebrafish (Danio rerio) model that has been widely used to study hematopoiesis. Although mammals have only one Lat3 gene, a GenBank BLAST query revealed that zebrafish have two Lat3 paralogs—lat3a (slc43a1a) and lat3b (slc43a1b)—which are likely to have arisen because of genomic duplication during teleost evolution (fig. S2A) (52). In some cases, gene duplication in teleosts has facilitated the study of cell type–specific effects by circumventing early embryonic lethality from global loss-of-function effects (53). In situ hybridization performed on 24 hours postfertilization (hpf) zebrafish embryos indicated that zygotic lat3a transcripts, but not lat3b, can be readily detected at the 20-somite stage in the intermediate cell mass (ICM), which is equivalent to the mammalian primitive erythropoietic blood islands and is characterized by gata-1 expression (Fig. 2A and fig. S2B). lat3a ICM staining was further confirmed by performing in situ hybridization on 24-hpf chordino (dino) (54) or spadetail (spt) (55) mutants, which either have an expanded or absent blood progenitor population, respectively. The lat3a staining pattern paralleled that of gata-1 with increased ICM staining in the dino mutants and no ICM staining in spt mutants (Fig. 2B), indicating that lat3a is the functional ortholog in zebrafish erythropoiesis, whereas lat3b is required for zebrafish nephrogenesis as previously reported (56).

Fig. 2 NEAA insufficiency reduces hemoglobinization of erythroid cells.

(A and B) In situ hybridization using probes specific for lat3a, lat3b, or gata-1 was performed on 24-hpf wild-type (WT) embryos (A) or mutant fish (B). ICM, red arrowheads; somites are positioned dorsal to the ICM at this developmental stage (black arrowhead). An enlarged view of the posterior ICM is provided in the bottom left corner of each panel. Scale bars, 0.2 μm. (C to F) Total RNA was isolated from control or morphant 72-hpf zebrafish embryos, and quantitative PCR analysis was performed (C). Control or morphant embryos from Tg(globin-LCR:eGFP) (D) or Tg(gata-1:eGFP) (E) transgenic lines were analyzed by flow cytometry. Control or morphant WT (F) zebrafish were stained with o-dianisidine to examine hemoglobinization at 72 hpf. Scale bar, 0.2 μm. (G and H) o-Dianisidine staining was performed on BCH-treated MEL cells or control or stably Lat3 shRNA–expressing MEL cells. (I and J) Total RNA was isolated from differentiating fetal liver cells infected with lentiviruses expressing the indicated shRNAs, and quantitative PCR was performed (I). These primary fetal liver cells were stained with o-dianisidine (J). *P < 0.05. Mean ± SEM, n = 3 independent experiments for (C), (D), (E), (G), (H), (I), and (J). Images in (A), (B), and (F) are representative of two independent experiments, each consisting of at least 40 embryos per condition. MO, morpholino.

Because naïve Lat1−/− T cells with inadequate NEAA import fail to differentiate (7), we asked whether limiting NEAA uptake in erythroid cells by inhibiting LAT3 function affected lineage commitment and specification. Using a transgenic zebrafish line that expresses enhanced green fluorescent protein (eGFP) driven by the globin promoter [Tg(globin-LCR:eGFP)], lat3a morphants had a comparable proportion of erythroid cells as control zebrafish embryos at 48 hpf (Fig. 2, C and D). However, at 72 hpf, we noticed a decrease in eGFP-positive erythroid cells in these morphant embryos (Fig. 2D). In contrast, a second transgenic zebrafish line that expresses eGFP driven by the gata-1 promoter [Tg(gata-1:eGFP)] showed a slight increase (that was not statistically significant) in the proportion of Tg(gata-1:eGFP)–positive erythroid cells in lat3a morphants (Fig. 2E), which may represent compensatory erythropoiesis that has previously been documented in models of defective red blood cell development (57, 58). In support of this notion, the proliferation of maturing MEL cells expressing either Lat3 shRNA was higher than that of control cells (fig. S2C). Together, these data suggest that LAT3 inhibition does not adversely affect erythroid specification and that the reduction in erythroid numbers in Tg(globin-LCR:eGFP) transgenic morphants represents a specific decrease in globin protein abundance. We further tested this idea by examining additional erythroid markers by in situ hybridization. Control and lat3a morphants expressed comparable amounts of the early erythroid markers gata-1 (59) and ae1 (60) at 24 and 48 hpf (fig. S2, D and E), respectively. Analysis of thrombocytic, myeloid, and lymphoid populations in lat3a morphants did not reveal a substantial effect on other hematopoietic lineages (fig. S2, F to H), suggesting that NEAA insufficiency did not affect hematopoietic lineage commitment or specification. We used flow cytometric analysis to further examine whether NEAA availability influences differentiation within the erythroid lineage. Primary murine fetal liver cells expressing Lat3 shRNAs showed no significant differences in the proportion of c-KITHigh;TER119Low progenitors or more committed c-KITModerate;TER119High and c-KITLow;TER119High erythroid populations (fig. S2, I to K). In addition, both control and Lat3 shRNA–expressing cells had similar increases in GATA1 protein abundance (fig. S2L), although this result differs slightly from that of a previous study showing a lack of change in GATA1 abundance throughout MEL cell maturation (61), a difference that likely reflects the genetic drift of our MEL cell subclone.

Whereas NEAA insufficiency did not affect red blood cell commitment and specification, the decrease in eGFP-positive cells in Tg(globin-LCR:eGFP) morphants (Fig. 2D) suggested a reduction in globin protein production. We directly tested this idea by performing o-dianisidine staining, which revealed a substantial reduction in red blood cell hemoglobinization in lat3a morphants (Fig. 2F). This effect was specific for lat3a because knockdown of the zebrafish lat1 homolog did not affect hemoglobinization (fig. S2, M and N), although lat1 expression was increased in murine fetal liver cells (Fig. 1A) and in the ICM of 24-hpf zebrafish embryos (fig. S2O). This finding agrees with LAT1’s functional requirement for the CD98 cotransporter, which is not present in erythroid cells (Fig. 1A) (6). Pharmacologic inhibition or RNAi (RNA interference)–mediated knockdown of LAT3 in MEL and primary murine fetal liver cells similarly reduced the proportion of o-dianisidine–positive cells (Figs. 1, F and G, and 2, G to J), indicating that hemoglobin production in red cells requires adequate LAT3-dependent NEAA uptake. These data are also consistent with the expression profile of Lat3 (Fig. 1A) in which maximal Lat3 expression occurs at later stages of erythroid maturation when hemoglobinization becomes most prominent (62).

Nascent globin protein translation depends on NEAA availability

We began to explore the molecular mechanisms and specificity underlying the deficit in hemoglobin production in response to limited NEAA uptake by first examining the abundance of erythroid-specific proteins (ankyrin1 and EPB42) and mitochondrial heme biosynthetic enzymes (ALAS2, PPOX, and FECH) that are critical for erythroid maturation (Fig. 3A) (63, 64). The protein abundance of all markers was similar in control and Lat3 shRNA–expressing maturing erythroid cells (Fig. 3A), as was that of several housekeeping proteins [TUBA1A, glyceraldehyde-3-phosphate dehydrogenase (GAPDH), heat shock 60 kD protein 1 (HSPD1), and cyclooxygenase IV (COX-IV)] (Fig. 3A). Mitochondrial physiology was also unaffected in maturing red blood cells with LAT3 knockdown because we did not detect deficiencies in mitochondrial biogenesis and glycolytic and tricarboxylic acid (TCA) cycle intermediates (fig. S3, A to C). These findings suggest that overall cellular function was largely unaffected by Lat3 knockdown. However, we noticed a substantial reduction in the abundance of α-globin protein (Fig. 3B) despite robust mRNA expression (Fig. 3C and fig. S3D). Unfortunately, we were unable to analyze β-globin protein abundance because of the lack of an immunoblot-applicable antibody. A similar decrease in β-globin protein abundance is likely because an imbalance in the ratio of α and β globin chains is cytotoxic and would lead to a substantial decrease in cell viability (65), which was not observed in either maturing primary murine fetal liver or MEL cells with LAT3 knockdown (fig. S3, E and F). Moreover, although Lat3 shRNA–expressing cells had lower TFRC protein abundance, iron uptake, and heme-bound iron, exogenous non–transferrin-bound iron supplementation did not restore hemoglobinization in these cells, but could do so in an SNX3-silenced MEL clone (fig. S3, G to J), which has a defect in the efficient acquisition of transferrin-bound iron (47). These findings exclude primary iron deficiency as the cause for the decreased hemoglobin production and suggest that NEAA insufficiency leads to a selective decrease in α/β-globin protein translation.

Fig. 3 α/β-Globin protein translation is preferentially reduced under limiting NEAA availability.

(A and B) Undifferentiated (day 0) and maturing (day 3 or 4) control or Lat3 shRNA–expressing MEL cells were lysed and immunoblotted with the indicated antibodies. (C) Total RNA was isolated from undifferentiated (day 0) and differentiating (day 3) control or Lat3 shRNA–expressing cells, and semiquantitative RT-PCR analysis for murine α-globin, β-major-globin, and Hprt was performed. (D) Control or Lat3 shRNA–expressing differentiating MEL cells were metabolically labeled with or without l-AHA. Nascent proteins were visualized by streptavidin–horseradish peroxidase (HRP), and other proteins were detected by immunoblotting. (E and F) Polysome profiling followed by semiquantitative RT-PCR was performed on differentiating control or Lat3 shRNA–expressing MEL cells at day 3 of DMSO differentiation. A representative profile is shown in (E) where the upward arrow represents the start of fraction collection. Densitometry analysis was performed on results from three independent experiments and expressed as a percentage of total RNA (F). The graph shows the means ± SEM. (G) Nonradioactive metabolic labeling was performed on differentiating MEL cells (day 3) treated with BCH. Nascent proteins were visualized using streptavidin-HRP and also immunoblotted with anti–α-globin antibody. n = 2 independent experiments for (A), (B), (D), and (G) and n = 3 for (C).

To test this idea, we performed nonradioactive metabolic labeling experiments with the l-methionine analog l-azidohomoalanine (l-AHA) (37). Metabolic labeling provides the most robust and accurate measurement of changes in protein translation rate (37, 66). We found that Lat3 knockdown substantially compromised nascent α/β-globin protein synthesis without affecting general translation, as evidenced by comparable amounts of higher molecular weight bands and similar steady-state amounts of several housekeeping proteins (Fig. 3D). In support of this notion, complementary polysome profiling revealed that α/β-globin mRNAs, but not those of other genes (Fig. 3, E and F), were shifted to lighter polysome fractions associated with decreased translation initiation in Lat3 shRNA–expressing maturing erythroid cells (20, 66). Given the sheer abundance of α/β-globin transcripts in red blood cells (35), even a selective reduction in α/β-globin translation results in a global decrease in polysome size (Fig. 3E), an effect that has previously been reported (67). Together, our results are consistent with a selective decrease in the translation α/β-globin proteins caused by diminished translation initiation that is associated with lighter polysomes and not elongation or termination, which would similarly result in slower translation but paradoxically with higher-density polysomes (66, 6872). To further establish the causal relationship between α/β-globin protein translation and subsequent change in steady-state amounts, we performed metabolic labeling experiments on already differentiated MEL cells. Short-term treatment with BCH to acutely inhibit LAT3 function significantly reduced nascent α/β-globin protein synthesis before exerting a noticeable effect on steady-state α-globin protein abundance (Fig. 3G). Thus, a specific deficit in globin protein translation occurs a priori and causes diminished red blood cell hemoglobinization under conditions of NEAA insufficiency.

mTORC1 senses sufficient uptake of NEAAs, particularly l-leucine, in maturing erythroid cells

Although LAT3 can transport l-leucine, l-phenylalanine, l-valine, and l-isoleucine, we wondered if a particular amino acid was more important for red cell hemoglobinization and tested this by administering esterified derivatives of these amino acids individually to BCH-treated MEL cells. Esterified amino acids are lipid-permeable and, once inside the cell, are converted to usable proteinogenic amino acids by endogenous esterases (73). o-Dianisidine staining revealed that esterified l-leucine had the most pronounced effect at restoring hemoglobin production (Fig. 4A). In addition, metabolic labeling experiments showed that esterified l-leucine most effectively increased the rate of α/β-globin protein translation in BCH-treated MEL cells (Fig. 4, B and C). This suggests that although LAT3 transports multiple NEAAs, hemoglobin production in maturing erythroid cells is particularly sensitive to l-leucine availability.

Fig. 4 mTORC1 senses sufficient NEAA uptake, particularly l-leucine, in maturing erythroid cells.

(A) BCH-treated MEL cells were administered with or without various amino acid esters starting at day 0 and were o-dianisidine–stained for hemoglobinization at day 4 of differentiation. (B and C) Nonradioactive metabolic labeling was performed on day 3 differentiated MEL cells treated with the indicated combinations of BCH and esterified amino acids (B). Relative protein abundance was quantified by densitometry from three independent experiments and normalized to the total amount of α-globin protein (C). (D) Day 3 differentiating control or Lat3 shRNA–expressing cell lysates were immunoblotted with the indicated antibodies. (E) Lysates isolated from control or lat3a MO2–injected zebrafish embryos were immunoblotted with the indicated antibodies. (F to I) MEL cells were treated with torin 1 (F and G) or rapamycin (H and I) and analyzed by o-dianisidine staining (F and H) or Western blotting (G and I). (J and K) Zebrafish embryos were treated with the indicated compounds and stained with o-dianisidine (J) or lysed and analyzed by Western blotting (K). Scale bar, 0.2 μm. (L) Nonradioactive metabolic labeling was performed on day 3 differentiating MEL cells treated with the indicated combinations of torin 1 and esterified amino acids. *P < 0.05. Mean ± SEM, n = 3 independent experiments for (A), (C), (F), and (H); n = 2 independent experiments for (D), (E), (G), (I), (K), and (L). Images in (J) are representative of two independent experiments with at least 40 embryos per treatment.

The responsiveness to l-leucine content and the preferential reduction in α/β-globin protein translation suggest that this is a coordinated adaptive mechanism that enables maturing erythroid cells to cope with amino acid insufficiency. mTORC1 is a kinase that is sensitive to amino acid availability, particularly that of l-leucine (2426). Thus, we next asked whether mTORC1 coordinates hemoglobin production with NEAA availability in maturing erythroid cells by examining whether mTORC1 activity was affected by LAT3 inhibition. Phosphorylation of Thr37/46 in 4E-BP1 (eukaryotic translation initiation factor 4E–binding protein 1) and Thr389 in S6K1 (S6 kinase 1)—two well-characterized mTORC1 targets—as well as phosphorylation of Ser240/244 in S6 was decreased in differentiating Lat3-knockdown MEL cells (Fig. 4D). The phosphorylation of S6K1 was not altered in undifferentiated cells (fig. S4A). These findings are consistent with the dispensable role for LAT3 in undifferentiated red blood cells (fig. S1, D and E). Additionally, MEL cells expressing Lat3 shRNAs also had increased autophagy characterized by higher LC3-II amounts (Fig. 4D), another marker of reduced mTORC1 function. Similarly, lat3a zebrafish morphant embryos at both 48 and 72 hpf showed reduced phosphorylation of Thr37/46 in 4E-BP1 and of Thr389 in S6K1 (Fig. 4E). mTORC1 activity was reduced in both undifferentiated and differentiating MEL cells starved of l-leucine, indicating that mTORC1 signaling was intact regardless of erythroid maturation (fig. S4B). In contrast, phosphorylation of Ser51 in eIF2α did not change in MEL cells with Lat3 knockdown (fig. S4C) or in lat3a zebrafish morphants (fig. S4D). These results were consistent with the partial reduction in NEAA uptake induced by LAT3 inhibition, which did not enable uncharged tRNAs to stimulate the kinase activity of GCN2, which required complete amino acid starvation (fig. S4E) (28) or complete l-leucine starvation, which may also reduce hemoglobin production (fig. S4, F and G).

To further examine whether mTORC1 activity regulated hemoglobin production, we treated MEL cells with the pharmacological mTOR inhibitors rapamycin and torin 1. MEL cell maturation occurs over 4 days, and hemoglobinization was reduced by continuous, chronic treatment of MEL cells with torin 1, but not with rapamycin (Fig. 4, F to I). Only an acute, 24-hour rapamycin treatment inhibited hemoglobinization (Fig. 4, H and I). The effect of rapamycin on hemoglobinization correlated with reduced phosphorylation of 4E-BP1, but not of S6K1 (Fig. 4, H and I), which agrees with work showing that S6K1 phosphorylation is more sensitive to rapamycin-mediated mTORC1 inhibition (28, 74). We also confirmed the effects of mTORC1 inhibition in vivo. Treatment with either rapamycin or torin 1 reduced hemoglobinization in zebrafish embryos, with torin 1 having a more pronounced effect (Fig. 4, J and K). Finally, although esterified l-leucine increased α/β-globin protein translation in MEL cells treated short-term with BCH (Fig. 4, B and C), it had no effect on torin 1–treated MEL cells (Fig. 4L), suggesting that mTORC1 activity is downstream of LAT3 and is required for coordinated α/β-globin protein translation in response to l-leucine availability.

α/β-Globin transcripts are direct mTORC1 translational targets

mTORC1 is a critical regulator of protein translation, and its effects are believed to involve both direct and indirect mechanisms (27, 28). Biochemically, direct mechanisms have been defined as translational changes that occur immediately (within 2 hours) after mTORC1 inhibition, whereas indirect mechanisms first involve mTORC1-dependent changes in the abundance of ribosomal subunits and would be engaged after the immediate response (27, 28). Transcripts that are directly regulated by mTORC1 also typically, but not always, have 5′ terminal oligopyrimidine (TOP) or TOP-like mRNA motifs [such as a pyrimidine-rich translational element (PRTE)] (27, 28, 66). Given our results that α/β-globin protein translation was dependent on mTORC1 activity, we asked whether α/β-globin transcripts are direct mTORC1 targets by evaluating these two criteria.

First, by mapping the transcription start sites of human and murine globin mRNAs using data from RefSeq, Ensembl, and UCSC (University of California Santa Cruz) databases, we found that five of the six globin transcripts fit the definitions of a TOP-like motif or PRTE (27, 28) (Fig. 5A). Unfortunately, we were unable to confirm our results using the database of transcription start sites (dbTSS) (28) that contain data from experimentally validated transcription start sites because α/β-globin mRNAs have not yet been annotated in the dbTSS. Nonetheless, all currently available data indicate that α/β-globin transcripts do have 5′ elements typically associated with direct mTORC1 translational regulation (66).

Fig. 5 α/β-Globin transcripts are direct mTORC1 translational targets.

(A) The most frequent transcription start sites (TSS) of murine and human α/β-globin mRNAs were analyzed using data from RefSeq, Ensembl, and UCSC databases for the presence of a 5′ terminal oligopyrimidine tract (TOP)–like motif or a PRTE. (B) Nonradioactive metabolic labeling was performed on differentiating MEL cells (day 3) treated with torin 1. Nascent proteins were visualized using streptavidin-HRP and also immunoblotted with anti–α-globin antibody. n = 2 independent experiments. (C and D) Polysome profiling and semiquantitative PCR were performed on differentiating control or torin 1–treated (2 hours) MEL cells at day 3 of DMSO differentiation. A representative profile is shown in (C) where the upward arrow denotes the start of fraction collection. Densitometry analysis was performed on results from three independent experiments normalized to total mRNA expression (D). The graph shows the means ± SEM.

Examining the sensitivity of α/β-globin protein translation to acute mTORC1 inhibition is the most crucial test of whether they represent direct targets. The enrichment of TOP and TOP-like variants has been derived using this definition (27, 28, 66). Empirical evaluation of acute responsiveness is required, given the potential ambiguity of α/β-globin transcription start sites in the absence of reliable data from dbTSS. Metabolic labeling experiments performed on differentiated MEL cells showed that α/β-globin protein translation was acutely responsive to short-term inhibition of mTORC1 activity by torin 1 (28) before a concomitant change in α-globin protein abundance (Fig. 5B). Polysome profiling experiments also confirmed a shift of α/β-globin mRNAs to lighter polysome and monosome fractions (Fig. 5, C and D). Compared to Lat3 shRNA knockdown (Fig. 3, E and F), the effects of torin 1 treatment are much more pronounced and widespread (such as depletion of Gata-1 from polysomes with torin 1 treatment but not with Lat3 shRNA knockdown), which is consistent with previous data showing that potent and acute mTORC1 inhibition by torin 1 affects the translation initiation of many proteins (28). As previously reported (28), Ybx1 was shifted to lighter polysome fractions, whereas Actb was more refractory to the effects of torin 1 (Fig. 5D). Together, our data establish α/β-globin mRNAs as direct, physiologic translational targets of mTORC1.

Control of hemoglobin production is mediated by 4E-BPs

The molecular mechanisms underlying mTORC1 translational regulation have been of considerable interest (27, 28, 75). Accumulating evidence indicates that 4E-BPs, not S6Ks, are the major regulators downstream of mTORC1 that mediate its direct effects (28). Unphosphorylated 4E-BPs bind to eIF4E, blocking the formation of the eIF4F complex to inhibit translation initiation. To date, three 4E-BP proteins have been identified, but only two have been studied (4E-BP1 and 4E-BP2) with regard to translation initiation (28, 76). We hypothesized that 4E-BPs were critical regulators of red blood cell hemoglobinization for three reasons: (i) α/β-globin transcripts are direct mTORC1 translational targets (Fig. 5); (ii) LAT3 inhibition triggers a depletion of α/β-globins from heavier polysome fractions, an effect that reflects diminished translation initiation (Fig. 3, E to G); and (iii) the effect of pharmacologic mTORC1 inhibition on hemoglobinization correlated with changes in the phosphorylation of 4E-BP1 but not that of S6K1 (Fig. 4, H and I).

We began testing our hypothesis with the 4E-BP mimetic 4EGI-1 and the S6K inhibitor DG2. Hemoglobin production in MEL cells and zebrafish embryos was reduced by 4EGI-1, but not in MEL cells by DG2 (Fig. 6, A and B), although phosphorylation of S6 was markedly reduced (fig. S5A), suggesting that control of hemoglobin production largely relies on 4E-BPs, not S6Ks. We further confirmed this result by deleting 4e-bp1 (Eif4ebp1) and 4e-bp2 (Eif4ebp2) using CRISPR/Cas9 genome editing in MEL cells (fig. S5, B to D). Compound, double-knockout (DKO) MEL cells retained greater hemoglobinization (Fig. 6, C and D) and α/β-globin protein translation (Fig. 6, E to H) compared to wild-type cells when treated with BCH or torin 1. Notably, loss of 4E-BP proteins had a greater effect on attenuating the inhibition of hemoglobinization by torin 1 than by BCH (Fig. 6, C and D). This result is likely because BCH inhibits NEAA uptake, resulting in inadequate NEAA substrate availability, an effect that would not be caused by torin 1 inhibition. Furthermore, administration of esterified l-leucine did not affect the translation rate of α/β-globin proteins in DKO erythroid cells treated with BCH or torin 1 (Fig. 6, I and J). Chloroquine treatment to inhibit autophagy (77) also failed to restore hemoglobin production in BCH-treated MEL cells (fig. S5E) as well as the translation and abundance of globin proteins in wild-type and DKO cells (fig. S5F), suggesting that the reduction in globin protein abundance does not result from autophagic hemoglobin degradation. Together, our data suggest that increased NEAA uptake is an integral aspect of erythropoiesis. mTORC1 serves as a sensor for NEAA sufficiency, particularly l-leucine, and coordinately regulates hemoglobin output at the translational level through the 4E-BPs and is distinct from the previously identified HRI signaling pathway (Fig. 7). We propose that this likely constitutes an adaptive mechanism in red blood cells because globin proteins have an unusually high l-leucine content compared to many other erythroid-enriched and housekeeper proteins (fig. S5G and table S1).

Fig. 6 α/β-Globin protein translation is regulated by 4E-BP proteins.

(A) Differentiating MEL cells at day 4 were stained with o-dianisidine after treatment with 4EGI-1 or DG2. (B) Zebrafish embryos at 72 hpf were treated with the 4E-BP mimetic 4EGI-1 and stained for hemoglobinization with o-dianisidine. Scale bar, 0.2 μm. (C and D) WT or DKO (deficient for both eif4ebp1 and eif4ebp2) MEL cells were differentiated with or without BCH (C) or torin 1 (D) and stained with o-dianisidine. (E to H) Nonradioactive metabolic labeling experiments were performed with l-AHA on WT or DKO cells with short-term BCH (E and F) or torin 1 (G and H) treatment. Proteins were detected by immunoblotting with the indicated antibodies, whereas biotinylated, nascent proteins were detected using a streptavidin-HRP conjugate (E and G). Densitometry analysis was performed on three independent experiments (F and H). Nascent α/β-globin protein synthesis was normalized to α-globin protein expression. (I and J) Nonradioactive metabolic labeling was performed on day 3 differentiated DKO MEL cells treated with the indicated combinations of BCH (I) or torin 1 (J) and esterified amino acids. *P < 0.05. Mean ± SEM, n = 3 independent experiments for (A), (C), (D), (F), and (H). Images in (B) are representative of two independent experiments with at least 40 embryos per treatment. n = 2 independent experiments for (I) and (J).

Fig. 7 mTORC1 coordinates hemoglobin translation with sufficient NEAA uptake, particularly l-leucine, during erythropoiesis.

A schematic depicting our model in which maturing erythroid cells rely on LAT3-mediated NEAA uptake to maintain homeostasis. In the absence of adequate uptake, reduced NEAA content, particularly l-leucine, triggers a reduction in mTORC1/4E-BP signaling and subsequent repression in translation for globin proteins. This mechanism is distinct from the previously identified eIF2α-dependent mechanism that becomes activated with severe amino acid (aa) deprivation (GCN2) or heme availability (HRI).


Why would erythroid cells require such a regulatory mechanism? The unusually high l-leucine content of the globin proteins together with their overall abundance (35) suggests that red blood cells require strategies to coordinate hemoglobin production with the availability of NEAAs, particularly l-leucine. mTORC1 exerts its metabolic effects through several effector pathways (24, 26). In nonerythroid tissues, mTORC1 inhibition reduces TFRC-mediated iron uptake (78). Although this effect may occur in maturing red blood cells (fig. S3, G to I), iron supplementation does not appreciably increase hemoglobinization under NEAA insufficiency (fig. S3J), indicating that a primary iron defect is not a major regulatory mechanism in maturing red blood cells downstream of LAT3. Although mTORC1 inhibition can block mitochondrial biogenesis (79), we did not find reduced mitochondrial function in cells expressing Lat3 shRNAs as suggested by lack of changes in mitochondrial proteins (Fig. 3A), MitoTracker staining (fig. S3A), and glycolytic and TCA cycle intermediates (fig. S3, B and C). Together, these results suggest that α/β-globin protein translational regulation is the principal mechanism that is engaged in erythroid cells to maintain NEAA homeostasis. Translational regulation offers the advantage of a rapid response (20) and is particularly beneficial because maturing erythroid cells become incapable of eliciting transcriptional adaptive responses, such as increased NFE2L1-mediated proteasome degradation (29) after chromatin condensation and enucleation.

The translation of α/β-globin proteins is tightly controlled by heme-regulated eIF2α kinase (HRI), which phosphorylates and inhibits eIF2α when heme is scarce (34). eIF2α is also phosphorylated under severe amino acid–depleted conditions by GCN2 (18), raising the possibility that diminished LAT3-mediated transport could influence hemoglobin production through GCN2-eIF2α signaling. However, we did not find an increase in the phosphorylation of Ser51 in eIF2α in Lat3 knockdown cells or lat3a zebrafish morphants (fig. S4, C and D). LAT3 inhibition likely did not sufficiently deplete intracellular NEAAs for uncharged tRNAs to activate GCN2 (1517). This observation also suggests that mTORC2 activity is unaffected by LAT3 inhibition because Torc2 stimulates Gcn2 activity in response to amino acid starvation in yeast (80). Instead, our data show that the coordinate regulation of α/β-globin protein translation in response to NEAA availability involves the mTORC1/4E-BP signaling mechanism, which is distinct from the eIF2α-dependent pathway (Fig. 7).

Current efforts to identify direct translational targets of mTORC1 have relied on using pharmacologic mTORC1 inhibitors (27, 28, 32). However, these analyses do not account for homeostatic feedback regulation that can influence the duration, magnitude, and specificity of the response (33, 75). Regulation of α/β-globin protein translation by HRI-eIF2α signaling in which specificity is dictated by heme availability exemplifies the importance of these considerations (34, 81) and highlights how upstream signals can substantially affect downstream translational control. In support of this notion, our polysome profiling experiments demonstrated that whereas acute torin 1 treatment markedly blocked translation initiation of multiple proteins (Fig. 5D), Lat3 knockdown had a more selective effect on globin protein translation (Fig. 3F). Genes that had TOP-like sequences that are responsive to torin 1 such as Ybx1 (28) were refractory to LAT3 inhibition (Fig. 3F) but remained responsive to torin 1 (Fig. 5D). Our findings are consistent with the failure of Lat1−/− naïve T cells to activate due to a selective inability to increase Myc protein abundance (7) and in contrast with the much more severe developmental defects that occur with genetic abrogation of mTORC1 (8284).

Tissue specificity also likely plays a crucial role in determining mTORC1 translational targets. For example, although vimentin translation is directly regulated by mTORC1 (27, 28), it is not transcriptionally expressed in maturing erythroid cells (85, 86). Currently, tissue-specific transcription start sites remain poorly annotated, which likely explains why the dbTSS has no data pertaining to α/β-globin mRNAs. The transcriptional programs in different cell types undoubtedly affect translational regulation, and although the use of potent mTORC1 inhibitors has provided considerable insight into mTORC1 translational control, a better understanding of these mechanisms in normal physiology and nutrient homeostasis is needed.

Our work has broad clinical implications. Clinical use of mTOR inhibitors has been associated with pronounced microcytic anemia, leukopenia, and thrombocytopenia in humans (87, 88). Some of these symptoms may be the result of defective hematopoietic stem cell function where mTORC1 activity and proper translational regulation are essential (82, 89, 90). However, our work suggests that these processes are also critical in committed erythroid cells, and the future clinical use of mTORC1 inhibitors with greater efficacy at blocking mTORC1-mediated translation is likely to cause a higher incidence of anemias. Our results also are an example of how a better understanding of amino acid metabolism can have a positive impact on human health by providing an explanation on why modulation of the mTORC1 pathway has been successful in treating human blood disorders. Rapamycin improves thalassemia symptoms in a murine model (91), and our data suggest that this effect is due to inhibition of defective globin translation, thereby correcting the globin chain imbalance and decreasing the formation of toxic aggregates. Conversely, l-leucine administration rescues several defects associated with DBA in animal models, cultured human CD34+ hematopoietic progenitors, and a human DBA patient (39, 9295) and has led to ongoing multicenter clinical trials (in phases 1 and 2) to assess the therapeutic benefits of l-leucine in the treatment of transfusion-dependent DBA patients. Although it is tempting to speculate that defective l-leucine or NEAA metabolism plays an etiological role in the actual development of DBAs or other human diseases arising from aberrant protein translation such as autism and Roberts syndrome cohesinopathies, whether this is truly the case is currently unknown (14, 37). Thus, further work directed at unravelling amino acid metabolism may not only uncover new causes of human disease but also lead to more mainstream use of amino acid supplementation as an effective treatment modality for a broad range of disorders.


Cell culture

DS19 MEL cells were cultured and differentiated with 2% DMSO as previously described (47). Primary fetal liver cells were harvested from E13.5 CD1 embryos. After dissections, livers were washed once with Hanks’ balanced salt solution. Cells were dissociated and maintained in culture medium consisting of StemPro-34 medium and supplement (Gibco), penicillin (100 U/ml), streptomycin (100 μg/ml), 2 mM l-glutamine, and freshly added erythropoietin (0.5 U/ml), stem cell factor (100 ng/ml), and 1 μM dexamethasone.

DS19 MEL cells were treated with 1 μM rapamycin (LC Laboratories) for 24 hours or 4 days and with 100 nM torin 1 (Tocris), 50 μM 4EGI-1 (Millipore), 1 μM DG2 (Millipore), 10 μM chloroquine, or 10 mM BCH (Sigma-Aldrich) for 4 days and then o-dianisidine–stained as described below. Amino acid esters were added to cells at a concentration of 0.8 mM (Sigma-Aldrich for all amino acid esters except for isoleucine ester, which was purchased from VWR).

MEL cells were electroporated with NT9 (control) or two shRNAs targeting Lat3 (shRNA-1 and shRNA-2) and cultured in medium containing puromycin (5 μg/ml) as previously described (47).

Three days after isolation, fetal liver cells were infected with lentiviruses expressing either a control shRNA or shRNA targeting murine Lat3. Two days after infection, cells were switched to differentiation medium consisting of StemPro-34 + supplement, penicillin (100 U/ml), streptomycin (100 μg/ml), 2 mM l-glutamine, and freshly added erythropoietin (5 U/ml), holo-transferrin (1 mg/ml), and insulin (0.4 U/μl) and incubated for another 2 days at 37°C. Cells were then o-dianisidine–stained to determine the extent of hemoglobinization.

Human CD34+ cells from mobilized peripheral blood of healthy donors were obtained from the Center of Excellence in Molecular Hematology at Fred Hutchinson Cancer Research Center, Seattle, WA. After thawing, 106 cells were maintained in stem cell medium [serum-free expansion medium (SFEM) supplemented with Flt3 ligand (100 ng/ml) and human thrombopoietin (10 ng/ml)] for 2 days to recover. The stem cell medium was a gift from B. Ebert (Harvard Medical School, Boston, MA). Cells were then switched to erythroid differentiation medium [SFEM supplemented with 2 mM l-glutamine, penicillin (100 U/ml), streptomycin (100 μg/ml), holo-transferrin (1 mg/ml), 10 μM β-mercaptoethanol, dexamethasone (4 μg/ml), recombinant human stem cell factor (25 ng/ml), and human erythropoietin (0.5 U/ml)]. After 7 days, total RNA was isolated.

Zebrafish experiments

All zebrafish experiments were performed in accordance with the Institutional Animal Care and Use Committee regulations. Injections and in situ hybridizations were performed as previously described (47, 53). Quantification by flow cytometry using fluorescently labeled transgenic zebrafish embryos was performed as previously described (96, 97). MOs were purchased from Gene Tools, LLC.

Zebrafish embryos at the one-cell stage were injected with MOs. The sequence of the MOs targeting the exon 4–intron 4 (MO1) and the exon 5–intron 5 (MO2) boundaries of D. rerio lat3a (see “Bioinformatics and statistical analysis” for accession numbers) were as follows: lat3a MO1, 5′-ATAGATCATGTACTCACCTTCTGGT-3′; lat3a MO2, 5′-CATTTTCTGCTGCTCCTTACCGTTA-3′. The MO targeting zebrafish lat1 (NM_001128358) at the exon 1–intron 1 boundary was 5′-AGGTAACAGTTTACTTACGTATACA-3′. Zebrafish embryos at 19 hpf (20 somites) were chemically dechorionated with Pronase (Roche); treated with DMSO (vehicle), 50 μM rapamycin, 1 μM torin 1, or 10 μM 4EGI-1; and o-dianisidine–stained at 72 hpf (96).

Quantitative and semiquantitative RT-PCR

RT-PCRs were performed as previously described with modifications (47). Total RNA was isolated from cells or 72-hpf zebrafish embryos using the Qiagen RNeasy Plus Mini Kit with on-column deoxyribonuclease (DNase) digestion with the ribonuclease (RNase)–free DNase set (Qiagen) according to the manufacturer’s instructions.

o-Dianisidine and trypan blue staining and cell proliferation

o-Dianisidine staining of MEL cells and zebrafish embryos was performed as described elsewhere (47). Trypan blue staining was performed according to the manufacturer’s instructions (Gibco) on day 4 differentiated control or shRNA-expressing MEL cells. For cell proliferation, control or MEL cells expressing Lat3 shRNAs were counted on days 0 to 4 of DMSO differentiation.

Metabolic labeling

55Fe-transferrin (55FeCl3, specific activity = 54.5 mCi/mol, Perkin Elmer) metabolic labeling was performed as previously described (47, 98). l-[3H]Leucine labeling was performed as described elsewhere with modifications (7). Two million cells were resuspended in 1 ml of leucine-free medium (Crystalgen) supplemented with 10% dialyzed fetal bovine serum (Invitrogen) and l-[3H]leucine (0.5 mCi/ml, specific activity = 106.2 Ci/mmol, Perkin Elmer) and incubated for 4 min at 37°C. Competition assays were performed in the presence of 10 mM BCH or the indicated amino acids (Sigma-Aldrich). Cells were then washed twice with phosphate-buffered saline (PBS) and resuspended in 500 μl of PBS, and radioactivity was measured by liquid scintillation.

Nonradioactive metabolic labeling was performed using the Click-iT Protein Reaction Buffer Kit (Molecular Probes) with Click-iT l-AHA (Molecular Probes) and biotin alkyne (Molecular Probes) according to the manufacturer’s instructions. Nonradioactive metabolic labeling of shRNA-expressing cells was carried out for 4 hours. For experiments involving acute treatment with torin 1, cells were first pretreated for 30 min with 250 nM torin 1, washed with PBS, and subsequently labeled for 1 hour in cysteine/methionine-free medium (Gibco) supplemented with 10% dialyzed fetal bovine serum, 2 mM l-glutamine, 1 mM sodium pyruvate, 50 μM l-AHA, 2% DMSO, and 250 nM torin 1 for an additional 2 hours at 37°C. BCH experiments were similarly performed except that 10 mM BCH pretreatment was for 1 hour. Esterified amino acids were added to the cells at the same time as pretreatment and regular treatment at a concentration of 0.8 mM.

Chloroquine was added to cells at the same time as torin 1 at 1 mM. Labeled lysates were resolved by SDS–polyacrylamide gel electrophoresis and analyzed by chemiluminescence using streptavidin-HRP (ThermoFisher Scientific) and Western blotting.

Lentivirus production and infection

Lentiviruses were produced as previously described with the following changes (99). Human embryonic kidney 293T cells were transfected with plasmids encoding psPax2, vesicular stomatitis virus glycoprotein, and various shRNAs using the ProFection Calcium Phosphate Kit (Promega) according to the manufacturer’s instructions. One day after transfection, medium was changed to low-serum medium (5%) and incubated at 37°C for another 2 days. Cell culture medium supernatant was collected and centrifuged at 24,000 rpm for 2 hours. The viral pellet was resuspended in 200 μl of Dulbecco’s modified Eagle’s medium. To infect cells, 50 μl of virus was added to the cells.

shRNAs and the NT9 control in a pLKO.1-puro vector backbone were purchased from Sigma-Aldrich. The sequences of shRNAs were as follows: for Lat3 shRNA-1, 5′-CCGGCCCTGGAATCAAGCTGATCTACTCGAGTAGATCAGCTTGATTCCAGGGTTTTTG-3′; for Lat3 shRNA-2, 5′-CCGGGCTTCGGGTCATCTTCTATATCTCGAGATATAGAAGATGACCCGAAGCTTTTTG-3′.

In situ hybridizations

In situ hybridization of sectioned murine embryonic tissue and zebrafish embryos was performed as previously described (47, 53).

CRISPR/Cas9-mediated genomic excision of Eif4ebp1 and Eif4ebp2

Eif4ebp1 and Eif4ebp2 were sequentially deleted in MEL cells as described previously with modifications (100, 101). Briefly, CRISPR guide sequences were designed to direct two cleavages at the Eif4ebp1 and Eif4ebp2 loci to generate a chromosomal deletion (101). CRISPR guide sequences were designed to have a unique 12-nucleotide seed sequence 5′-NNNNNNNNNNNN-NGG-3′ in the mouse genome ( to minimize off-target cleavages. CRISPR guides were cloned into pX330 plasmid (Addgene) with Bbs I ligation as previously described (100). Deletion of both genes was performed in a similar manner to previous reports (100102). The CRISPR oligo sequences were as follows. For Eif4ebp1, the 5′ CRISPR oligos were 5′-CACCGTTCTTCTCTGAGGATCGGCC-3′ and 5′-AAACGGCCGATCCTCAGAGAAGAAC-3′, and the 3′ CRISPR oligos were 5′-CACCGTATAAAGGAGAGCGTTTAGC-3′ and 5′-AAACGCTAAACGCTCTCCTTTATAC-3′. For Eif4ebp2, the 5′ CRISPR oligos were 5′-CACCGCTACCGGAAGCGGTCGAAGG-3′ and 5′-AAACCCTTCGACCGCTTCCGGTAGC-3′, and the 3′ CRISPR oligos were 5′-CACCGCATGCACACGGCTCCGGTGT-3′ and 5′-AAACACACCGGAGCCGTGTGCATGC-3′.

CRISPR/Cas9 constructs were delivered to MEL cells by electroporation. One million MEL cells were resuspended in BTX solution with 2 μg of each of two CRISPR/Cas9 constructs (which had been designed to generate flanking cleavages resulting in a deletion) and 0.2 μg of pmaxGFP (Lonza), transferred to a 2-mm cuvette, and electroporated at 250 V and 5 ms using a BTX ECM 830 electroporator (Harvard Apparatus). Cells were placed immediately in 5 ml of medium at 30°C. After 1 to 3 days, cells were sorted by fluorescence-activated cell sorting (FACS) with gating on the 1 to 3% brightest GFP-positive live events. Cells were plated by limiting dilution at 0.3 cells per well in 96-well plates and cultured at 37°C. Genomic DNA was isolated from individual clones using QuickExtract (Epicentre) according to the manufacturer’s instructions and were screened by PCR for the wild-type and deletion allele with HotStartTaq DNA Polymerase Kit and confirmed by immunoblot analysis. The primers used for genotyping were as follows. For Eif4ebp1, the forward (F) primer was 5′-AGTACGCAGAGCTTCGATCC-3′, the reverse-1 (R1) primer was 5′-GAGTCTGGCTGCAGCTGCTG-3′, and the reverse-2 (R2) primer was 5′-ACCCTCCCTCTCTTCTCCAG-3′. For Eif4ebp2, the F primer was 5′-ACCCTCTGCCTCTAGCCTTC-3′, the R1 primer was 5′-CACGCTCGGCTCTCAACTCG-3′, and the R2 primer was 5′-CCACCTTCCTGTGGTAAGGA-3′.


Immunoblotting was performed as previously described (99). Anti-LAT3 (ab55552), anti-PDHD (ab67592), and anti–COX-IV (ab16056) rabbit polyclonal antibodies were purchased from Abcam. Anti-GAPDH (MAB374) and anti-TFRC (136800) mouse monoclonal antibodies were purchased from Millipore and Invitrogen, respectively. Mouse monoclonal anti-ATP6V1H (G-2), anti-TUBA1A (DM1A), and anti-ACTB (C-2) and goat polyclonal anti-FECH (C-20), anti-HSPD1 (K-19), and anti-GATA1 (N-1) antibodies were purchased from Santa Cruz Biotechnology. Rabbit monoclonal anti-LC3B (2775S), anti-(pS51)eIF2α (D9G8), anti-eIF2α (D7D3), anti-(pT37/pT46)4E-BP1 (236B4), anti-(pT389)S6K1 (108D2), anti–4E-BP1 (53H11), anti–4E-BP2 (#2845), anti-S6K1 (49D7), and anti-(pS240/244)S6 (D68F8) and mouse monoclonal anti-S6 (54D2) were purchased from Cell Signaling Technology. The rabbit polyclonal anti-PPOX antibody was a gift from H. A. Dailey (University of Georgia, Athens, GA). The rabbit polyclonal anti-ankyrin1 and anti-EPB42 antibodies were gifts from S. E. Lux IV (Harvard Medical School, Boston, MA). The anti-ALAS2 rabbit polyclonal antibody was a gift from H. Munakata (Kinki University, Osaka-Sayama, Japan).

Gas chromatography–mass spectrometry

Twelve million differentiated cells were washed once in PBS and frozen at −80°C. Metabolite extraction and GC-MS were performed at the Metabolomics Core at the University of Utah (Salt Lake City, UT). Three hundred sixty microliters of 90% methanol was added to the cell pellet to give an approximate final concentration of 80% methanol. Samples were incubated for 1 hour at −20°C followed by centrifugation at 30,000g for 10 min at −20°C. The supernatant was transferred to a new tube and vacuum-dried. GC-MS analysis was performed using a Waters (Milford) GCT Premier mass spectrometer fitted with an Agilent 6890 gas chromatograph and a Gerstel MPS2 autosampler. Dried samples were suspended in 40 μl of O-methoxylamine hydrochloride in pyridine (40 mg/ml) and incubated for 1 hour at 30°C. Twenty-five microliters of this solution and 10 μl of N-methyl-N-trimethylsilyltrifluoracetamide were added to the autosampler vials and incubated for 1 hour at 30°C with shaking. Three microliters of fatty acid methyl ester standard solution was added, and 1 μl of this final sample was injected to the gas chromatograph inlet in the split mode with the inlet temperature held at 250°C. A 10:1 split ratio was used for analysis. The gas chromatograph had an initial temperature of 95°C for 1 min followed by a 40°C/min ramp to 110°C and held for 2 min. This was followed by a second 5°C/min ramp to 250°C, a third ramp to 350°C, and then a final hold of 3 min. A 30-m Phenomenex ZB-5 MSi column with a 5-m-long guard column was used for chromatographic separation. Helium was used as the carrier gas at 1 ml/min. Data were collected using MassLynx4.1 software (Waters). Metabolites were identified, and their peak area was recorded using QuanLynx (Waters). These data were then transferred to an Excel (Microsoft) spreadsheet for further data analysis.

Polysome profiling

Polysome profiling was performed as previously described with modifications (103). Briefly, MEL cells expressing control or Lat3-specific shRNA (shRNA-1) were differentiated using 2% DMSO. At day 3 of differentiation, cells were harvested by centrifugation and lysed in buffer containing KCl (0.15 M), tris-Cl (pH 7, 0.010 M), NP-40 (0.5%), cycloheximide (150 μg/ml), dithiothreitol (0.020 M), MgCl2 (0.010 M), and rRNasin (100 U/ml). Lysates were diluted in polysome buffer (pH 7.4) containing Hepes (0.04 M), KCl (0.1 M), MgCl2 (0.005 M), and trisodium citrate (0.002 M) and treated with polysome detergent by combining 9 volumes of lysate, representative of 20 million cells, with 1 volume of polysome detergent and incubating at 4°C with gentle rocking for 10 min. Treated lysates were gently loaded onto a linear sucrose gradient (15 to 60% ultrapure sucrose in polysome buffer) for polysome analysis. Gradients were centrifuged at 180,000g at 4°C for 2 hours in a Sorvall TH-641 swinging bucket rotor. Tubes containing resolved gradients were fractionated using an ISCO gradient fractionator including the Type 11 Optical Unit at about 1 ml/min, and fractions were collected at 1-min intervals as they left the optical unit. The optical density at 254 nm from the optical unit was imported into an Agilent Technologies SS420X interface and exported as millivolts by the EZChrom SI software. Thus, the polysome figures are shown as millivolts as a function of time (minutes). The dead time before the start of fraction collection was about 3 min, and the final (tenth) fraction was collected after 13 min. Fractions were snap-frozen in liquid nitrogen and stored at −80°C until use. Reverse transcription was performed as described above, and semiquantitative PCR was performed using the HotStartTaq DNA Polymerase Kit. For drug treatment, differentiating MEL cells were treated on day 3 of differentiation with 250 nM torin 1 or vehicle for 2 hours before harvest, lysis, and polysome analysis. Densitometry analysis was performed by averaging three independent experiments using ImageJ software (104). Data were normalized to total RNA collected in all fractions.

Flow cytometry and fluorescence microscopy analysis

Flow cytometric analysis of zebrafish embryos was performed as described elsewhere (47, 96, 97, 105). Fluorescence microscopy analysis was performed on Tg(rag2:eGFP) zebrafish embryos at 96 hpf using a Leica MZ TLIII microscope and a Leica DC500 camera. Phase-contrast and fluorescent images were merged using Adobe Photoshop CS3.

To examine mitochondrial mass, cells were stained with 200 nM MitoTracker Red 580 (Molecular Probes) according to the manufacturer’s instructions. Flow cytometry was performed on a BD FACSCanto II (BD Biosciences) using BD FACSDiva software (BD Biosciences). For analysis of erythroid differentiation and viability, primary murine fetal liver cells were simultaneously stained with allophycocyanin-conjugated c-KIT and phycoerythrin-conjugated TER119 antibodies (BD Biosciences) followed by annexin V (BD Biosciences) and 7-aminoactinomycin D (BD Biosciences) staining to measure cell viability. Flow cytometry was carried out on a BD LSRII flow cytometer (BD Biosciences), and data analysis was performed using FACSDiva software.

Quantitative and semiquantitative RT-PCR

PCRs were performed as previously described with modifications (47, 97). Total RNA was isolated from cells or 72-hpf zebrafish embryos using the Qiagen RNeasy Plus Mini Kit with on-column DNase digestion with the RNase-free DNase set (Qiagen) according to the manufacturer’s instructions. One microgram of total RNA was used for reverse transcription with the High Capacity cDNA Reverse Transcription Kit (Applied Biosystems). Quantitative RT-PCR was performed using gene- and species-specific TaqMan probes (Applied Biosystems) or the α/β-globin and Hprt primers listed below. Semiquantitative RT-PCR expression and polysome profiling analyses were carried out using FastStart Taq DNA Polymerase (Roche) and HotStartTaq DNA Polymerase Kit (Qiagen), respectively, with the following primers specific for murine genes: for α-globin, 5′-TGGCTAGCCAAGGTCACCAGC-3′ and 5′-CTCTCTGGGAAGACAAAAGCAAC-3′; for β-major-globin, 5′-GGTTTAGTGGTACTTGTGAGCC-3′ and 5′-ATGGTGCACCTGACTGATGCTG-3′; and for Hprt, 5′-CACAGGACTAGAACACCTGC-3′ and 5′-GCTGGTGAAAAGGACCTCT-3′. All other primers were as previously described (28). Primers specific for zebrafish genes were as follows: for lat1, 5′-TGAAACTGTGGATCGAGCTG-3′ and 5′-AGGCATCTTGAACCCTTGTG-3′; for β-actin, 5′-ACCAGAGGCATACAGGGACAG-3′ and 5′-GTTGGTATGGGACAGAAAGAC-3′.

Bioinformatics and statistical analysis

Analysis of primary fetal liver RNAseq data based on TER119 and CD71 expression was performed as previously described (45, 47). The accession number for the RNAseq data set is GSE32110 ( (45). Amino acid composition was calculated using Expasy ( and plotted as a heat map using MultiExperiment Viewer. Phylogenetic analysis of Lat3 isoforms of various species was performed as previously described (53). The accession numbers of the genes are as follows: H. sapiens, NM_003627; P. troglodytes, XM_003318000; M. musculus, NM_024497; D. rerio (lat3a), NM_199897; D. rerio (lat3b), NM_001083000.

The transcription start sites of murine and human α/β-globin transcripts were analyzed using sequences from RefSeq, Ensembl, and UCSC databases. The most common transcription start site was compared to consensus sequences defined by previous studies (27, 28). Student’s t test was used for all statistical analysis except for amino acid competition assay (Fig. 1I) where a two-way ANOVA (analysis of variance) was used.


Fig. S1. Lat3 expression and function during erythroid development.

Fig. S2. LAT3 inhibition specifically decreases hemoglobinization.

Fig. S3. NEAA insufficiency does not affect hemoglobinization through mitochondrial function or iron uptake.

Fig. S4. mTORC1 activity is not affected by LAT3 inhibition in undifferentiated erythroid cells.

Fig. S5. 4E-BP proteins are critical regulators of hemoglobin translation.

Table S1. Essential amino acid composition.


Acknowledgments: We would like to thank the members of our laboratory as well as R. I. Handin, V. Sankaran, H. Franklin Bunn, J. E. Italiano Jr., D. J. Kwiatkowski, A. Gutierrez, B. Ebert, E. Chen, M. Côté, J. Misasi, J. Kaplan, A. Khanna-Gupta, L. Li, M. S. Irwin, C. Patry, T. Reddi, and M. Maynard for technical assistance and insightful discussions. We thank S. Lin (UCLA, Los Angeles, CA) for the Tg(gata-1:eGFP) transgenic line, L. I. Zon (Harvard Medical School, Boston, MA) for the Tg(globin-LCR:eGFP) transgenic line, R. I. Handin (Harvard Medical School, Boston, MA) for the Tg(cd41:eGFP) transgenic line, T. Look (Harvard Medical School, Boston, MA) for the Tg(rag2:eGFP) and the Tg(pu.1:eGFP) transgenic lines, K. Hoffmeister (Harvard Medical School, Boston, MA) for the use of the FACS machine, H. A. Dailey (University of Georgia, Athens, GA) for the anti-PPOX antisera, S. E. Lux IV (Harvard Medical School, Boston, MA) for the anti-ankyrin1 and anti-EPB42 antisera, H. Munakata (Kinki University, Osaka-Sayama, Japan) for the anti-ALAS2 antisera, A. Skoultchi (Albert Einstein Medical College, Bronx, NY) for the DS19 MEL subclone, J. Cunningham (Harvard Medical School, Boston, MA) for chloroquine, and C. Lawrence and his team for the zebrafish husbandry (Boston Children’s Hospital). Metabolomics GC-MS studies were performed at the Metabolomics Core at the University of Utah (J. Phillips and J. Cox). Funding: This work was supported by grants from the Canadian Institutes of Health Research (CIHR Postdoctoral Fellowship, J.C.), the Cooley’s Anemia Foundation (C.C.), the Dutch National Science Fund-NWO (I.J.S.), the American Heart Association (A.J.D.), the March of Dimes Foundation (6-FY09-289, B.H.P.), and the NIH (K08 DK093705, D.E.B.; T32 HL007574 and F32 DK098866, Y.Y.Y.; R01 DK09361, J.P.; R01 DK066600, R.S.E.; R01 DK070838, B.H.P.; P01 HL032262, B.H.P., A.B.C., H.F.L., and S.H.O.). Author contributions: J.C. and B.H.P. conceived the project, designed and performed most of the experiments and data analysis, and wrote the manuscript. D.E.B. designed and performed the CRISPR genome editing strategy and electroporation into DS19 MEL cells. A.G. performed the fetal liver dissections and analysis. C.P.N. and K.M.D. prepared the polysome gradients. P.D.K. performed murine in situ hybridizations. C.C. and I.J.S. did the initial bioinformatics analysis of the RNAseq data. Y.Y.Y., N.C.H., C.C., I.J.S., A.J.D., and J.G.W. assisted with flow cytometric analysis and zebrafish husbandry. H.F.L. provided the RNAseq database. J.P., S.H.O., H.F.L., R.S.E., and A.B.C. discussed the results and critically revised the manuscript. B.H.P. supervised and coordinated the project. Competing interests: The authors declare that they have no competing interests.
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