Endoplasmic Reticulum Stress and Lipid MetabolismView this Special Issue
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UPR-Mediated Membrane Biogenesis in B Cells
The unfolded protein response (UPR) can coordinate the regulation of gene transcription and protein translation to balance the load of client proteins with the protein folding and degradative capacities of the ER. Increasing evidence also implicates the UPR in the regulation of lipid synthesis and membrane biogenesis. The differentiation of B lymphocytes into antibody-secreting cells is marked by significant expansion of the ER, the site for antibody synthesis and assembly. In activated B cells, the demand for membrane protein and lipid components leads to activation of the UPR transcriptional activator XBP1(S) which, in turn, initiates a cascade of biochemical events that enhance supplies of phospholipid precursors and build machinery for the synthesis, maturation, and transport of secretory proteins. The alterations in lipid metabolism that occur during this developmental transition and the impact of membrane phospholipid restriction on B cell secretory characteristics are discussed in this paper.
Activated B lymphocytes proliferate and proceed along distinct developmental pathways that determine their function and fate. Specifically, responding B cells can rapidly differentiate in extrafollicular sites into short-lived antibody-secreting cells that predominantly secrete IgM antibodies . Alternatively, responding B cells can enter germinal centers, undergo somatic hypermutation and isotype switching, and then become memory B cells or long-lived antibody-secreting cells . Extrinsic factors, including the nature of the antigen and T cell help in the form of membrane-bound molecules and soluble cytokines, play key roles in regulating B cell responses. However, intrinsic signals are also pivotal in directing the fate of responding B cells as evidenced by the critical role of the unfolded protein response (UPR) transcription factor XBP1(S) in driving the differentiation of antibody-secreting cells [3, 4], the effectors of humoral immunity. Here, we discuss the current understanding of the relationship between the UPR, lipid biosynthesis and organelle biogenesis in activated B cells.
2. Lipid Supply and Demand
B lymphocytes proliferate and differentiate into antibody-secreting cells upon interaction with specific antigen or certain Toll-like receptor (TLR) ligands. When B cells are stimulated to enter the cell cycle and proliferate, the mechanisms that control the membrane phospholipid supply in rapidly dividing cells are engaged. The division of one cell into two daughter cells requires a doubling of membrane content during cell cycle progression . Phosphatidylcholine (PtdCho) is the major membrane phospholipid in mammalian cells and is a precursor to the two other most abundant membrane phospholipids, sphingomyelin (SM)  and phosphatidylethanolamine (PtdEtn) . PtdCho and the other phospholipids accumulate in a periodic manner during S phase, coincident with DNA synthesis. The net increase in membrane PtdCho results from an interaction between cell cycle-dependent oscillations in the rates of PtdCho biosynthesis and degradation. PtdCho synthesis is stimulated very early during G1 phase [8–10], but is accompanied by rapid PtdCho turnover. Two phospholipases have been implicated in the PtdCho turnover associated with cell cycle progression, the group VIA calcium-independent phospholipase A2  and the neuropathy target esterase . Near the G1/S transition, PtdCho turnover is diminished substantially, yielding a net increase in membrane PtdCho. Toward the latter part of the cell cycle, prior to cytokinesis, PtdCho synthesis is downregulated . This cyclic variation in the supply of membrane phospholipid for cell proliferation is maintained in the absence of differentiation.
B cells are unique, however, and in addition to proliferation also undergo a subcellular membrane expansion as they differentiate into antibody-secreting cells after stimulation. There is a major increase in synthesis and secretion of immunoglobulin (Ig) heavy (H) and light (L) chains . Nascent Ig chains are cotranslationally translocated into the endoplasmic reticulum (ER), an oxidizing, calcium-rich environment containing many resident molecular chaperones and folding enzymes . Within this specialized protein folding compartment, H and L chains are assembled into functional antibodies. Induction of high-rate Ig synthesis during the differentiation process is accompanied by expansion of the rough ER membrane, at least 3- to 4-fold in surface area and volume [15, 16]. Thus, both proliferation and differentiation require an increased supply of phospholipids to fuel membrane and organelle biogenesis. To meet this demand, the synthesis of phospholipids, particularly PtdCho, increases when B cells are activated [15, 17].
3. Phosphatidylcholine Synthesis
The predominant means for PtdCho biosynthesis in mammalian cells proceeds via the three steps of the cytidine diphosphocholine (CDP-choline) pathway  (Figure 1). First, choline kinase (CK) phosphorylates choline in the presence of ATP to yield phosphocholine. CKα and CKβ are two isoforms which are soluble proteins found in the cytosol [19, 20]. Second, choline cytidylyltransferase (CCT) converts phosphocholine to CDP-choline in the presence of CTP, and this is the rate-limiting step in the pathway . In every cell type examined thus far, including B cells , CCT catalyzes the slow step in the pathway and thereby determines the rate of PtdCho formation. Comparatively small amounts of CDP-choline are found in cells, in relation to other phospholipid precursors, as CDP-choline is utilized almost immediately after it is made. CCT, including all mammalian isoforms, transiently associates with the ER membrane and the lipid composition of the ER membrane governs CCT association and activity . Elevated expression of CCT stimulates PtdCho synthesis but often does not result in an increased amount of cellular PtdCho in most proliferating cells due to compensatory elevation of PtdCho turnover mediated by phospholipases [23, 24]. Third, the phosphocholine moiety of CDP-choline is transferred to diacylglycerol (DAG), producing PtdCho. This final step can be catalyzed by either cholinephosphotransferase (CPT1) or choline/ethanolaminephosphotransferase (CEPT1), a bifunctional enzyme that can synthesize both choline- and ethanolamine-containing phospholipids. The CPT enzymes are integral membrane proteins, and the CPT1 is found with the Golgi apparatus while the CEPT1 associates with the ER [25, 26]. Here, we refer to the activities of CPT1  and CEPT1  collectively as CPT activity. The locations of the CPT enzymes designate the subcellular sites of membrane biogenesis; however, enforced overexpression of CPT activity does not enhance PtdCho synthesis [29, 30]. Rather, the supply of CDP-choline and DAG determine the amount of PtdCho. Thus, elevated expression of the CPT enzymes can be considered as a marker for Golgi and/or ER membrane expansion, but not necessarily as a driver of membrane phospholipid synthesis.
In lipopolysaccharide- (LPS-) stimulated splenic B cells, CK activity remains fairly constant, CCT activity modestly increases ≈2-fold, and CPT activity increases ≈6-fold . These modulations of the CDP-choline pathway enzymes in LPS-stimulated splenic B cells correlate with a 6- to 7-fold increase in PtdCho synthesis [15, 31]. Our studies using the CH12 B cell lymphoma indicate that increased CCT activity is pivotal for enhanced flux through the CDP-choline pathway in LPS-stimulated B cells . In this system, the CCT expression and enzyme specific activity do not increase when assayed under optimal in vitro conditions following LPS stimulation. However, radiolabeling experiments of stimulated cells demonstrate that the formation of CDP-choline is substantially enhanced, indicating allosteric activation of CCT by membrane lipids. Indeed, microsomal lipids isolated from stimulated cells contain an elevated amount of DAG and significantly stimulate the activity of purified recombinant CCT, compared to lipids isolated from unstimulated cells. Thus, in this case, the formation of DAG is key to stimulation of PtdCho synthesis: first, by activating CCT, and second, by providing substrate for the CPT enzymes. The CCT, in turn, governs the fate of the DAG as DAG is incorporated either into phospholipid under permissive CCT conditions or into triacylglycerol (TAG) when the CCT activity is reduced  (Figure 1).
4. A “Physiologic” UPR
ER stress occurs when the load of client proteins exceeds the folding capacity of the ER, a condition that can be catastrophic if unresolved. To rebalance load with capacity in the ER, thereby relieving ER stress, the UPR can slow the flow of nascent polypeptides into the ER lumen and enhance the ER machinery needed for folding and/or disposal of client proteins [33, 34]. The mammalian UPR is orchestrated by a trio of signaling pathways that are separately initiated by three ubiquitously expressed ER transmembrane proteins: PERK (PKR-like ER kinase) [35, 36], ATF6 (activating transcription factor 6) α and β [37, 38], and IRE1 (first identified in a yeast mutant with inositol requiring phenotype) α and β [39, 40]. The activation status and role of each UPR pathway has been examined during the differentiation of antibody-secreting B cells.
The PERK protein possesses a serine/threonine kinase domain in its cytoplasmic region through which it mediates translational attenuation [35, 36]. Upon activation, PERK phosphorylates the α subunit of eIF-2 (eukaryotic initiation factor-2) on serine 51, thereby impeding formation of translation initiation complexes and slowing the flow of nascent polypeptides into the ER [41, 42]. PERK does not appear to be activated during the differentiation of antibody-secreting B cells [43, 44]. In support of this concept, studies of gene-targeted mice reveal that the PERK pathway is dispensable for antibody secretion .
ATF6α and ATF6β are type II ER transmembrane proteins [37, 38]. Upon UPR activation, ATF6 traffics from the ER to the Golgi complex where it is clipped by the Site-1 and Site-2 proteases [45, 46]. Once liberated from the membrane by this process of intramembrane proteolysis, the cytosolic N-terminal domain of ATF6 moves into the nucleus where it functions as a transcriptional activator of genes encoding ER resident molecular chaperones, folding enzymes and components involved in ER-associated degradation (ERAD) of misfolded proteins [37, 38, 47–49]. While ATF6α and β are both functional, only ATF6α appears essential for induction of ER stress responsive genes and survival of cells subjected to ER stress conditions [48, 49]. Overexpression of active ATF6α is sufficient to drive synthesis of fatty acids and phospholipids and to induce expansion of rough ER , suggesting that this UPR pathway might participate in the differentiation of antibody-secreting B cells. Indeed, ATF6α is activated in LPS-stimulated B cells [43, 51, 52]. However, recent studies of ATF6α-deficient mice indicate that ATF6α, like PERK, is dispensable for the differentiation of antibody-secreting B cells (Brewer et al., manuscript in preparation).
The IRE1 proteins contain a serine-threonine kinase module and a C-terminal endoribonuclease domain in their cytoplasmic regions [39, 40]. Upon activation, IRE1 executes site-specific cleavage of Xbp1 (X-box binding protein 1) mRNA. A 26-nt intron is excised and an undefined mechanism then ligates the resulting 5′ and 3′ fragments, yielding a spliced Xbp1 mRNA with an altered reading frame [53–55]. Both unspliced and UPR-spliced Xbp1 transcripts encode basic leucine zipper (bZIP) transcription factors, XBP1(U) and XBP1(S), respectively. The XBP1(S) factor exhibits enhanced transactivating capacity and greater stability as compared to XBP1(U) [53–56]. Like ATF6α, XBP1(S) is sufficient to upregulate synthesis of fatty acids and phospholipids and to drive expansion of rough ER [30, 50]. Xbp1 is essential for optimal induction of genes encoding proteins that function throughout the secretory pathway and for proper development of the ER in a variety of specialized secretory cell types [57, 58]. When B cells are stimulated to secrete antibody, Xbp1 mRNA increases and undergoes UPR-mediated splicing to yield XBP1(S) [3, 52, 53], a factor required for the generation of antibody-secreting B cells [3, 4]. Thus, the physiologic UPR of activated B cells features the IRE1/XBP1 pathway.
5. XBP1(S), Lipid Synthesis, and ER Biogenesis
Xbp1 is required for embryonic development ; thus, the role of this UPR transcription factor in lymphocytes was first investigated using the Rag-2 complementation system . Those experiments revealed that XBP1-deficient B cells are markedly defective in antibody secretion in vivo in response to immunization and in vitro in response to LPS. Importantly, it was shown that XBP1(S), but not XBP1(U), effectively restores the ability of XBP1-deficient B cells to secrete antibody in response to LPS in vitro  and is sufficient to drive ER expansion [30, 58]. More recently, the Cre-loxP system has been employed for selective deletion of Xbp1 in B cells and studies using this system have corroborated the earlier findings [60, 61]. Using this system, the abundance of PtdCho was shown to increase in LPS-stimulated XBP1-deficient B cells, but to a lesser degree than in wild-type cells . The levels of PtdCho, SM, and phosphatidylinositol were significantly reduced in activated XBP1-deficient B cells, but PtdEtn, phosphatidylserine, and phosphatidylglycerol were similar to corresponding amounts in wild-type activated B cells. In addition, a meager, but discernible, expansion of the rough ER was observed in LPS-stimulated XBP1-deficient B cells .
PtdCho is most drastically affected by XBP1 deficiency because it is the most abundant phospholipid of the ER membranes. SM is derived directly from PtdCho, where the phosphocholine headgroup of PtdCho is transferred to ceramide by the SM synthase  (Figure 1). Thus, a reduction in PtdCho availability would be reflected by a reduction in SM. The pathway for PtdCho conversion to PtdEtn is not as direct, however, and a second pathway of PtdEtn synthesis via CDP-ethanolamine can bypass a deficiency in PtdCho . Thus, the amount of PtdEtn is less affected following activation of XBP1-deficient B cells and PtdEtn increases to almost the same extent as in activated wild-type B cells. On the other hand, the enforced expression of XBP1(S) in NIH-3T3 fibroblasts leads to a substantial increase in PtdEtn , augmenting the XBP1(S)-independent mechanism(s) of lipogenesis. The de novo synthesis of ceramides, key precursors in SM production, is upregulated upon LPS stimulation  and contributes to the increase in SM. Inhibition of ceramide formation impairs ER expansion and protein glycosylation in the ER lumen , suggesting a link among these processes. These data establish that XBP1 is required for maximal increases in PtdCho, SM, and rough ER in LPS-stimulated B cells, but the mechanisms by which XBP1 mediates these events remain to be elucidated. The scheme in Figure 1 shows a cascade of biochemical events which illustrates how XBP1(S) stimulation of fatty acid synthesis  is a key feature that drives membrane phospholipid expansion in B cells . Furthermore, these data suggest that XBP1-independent mechanisms, as yet undefined, must also contribute to the regulation of PtdCho synthesis and ER biogenesis during the differentiation process.
It has been proposed that the escalation of Ig synthesis in differentiating B cells taxes the protein folding machinery of the ER and, consequently, triggers the UPR . This model was supported by an experiment showing reduced induction of XBP1(S) in B cells that had undergone ex vivo Cre-mediated deletion of IgH chain prior to LPS stimulation . In contrast, recent studies have shown strong induction of XBP1(S) in B cells stimulated with LPS [60, 62], indicating that increased synthesis of soluble μ H chains is not a prerequisite for UPR activation. In keeping with these data, we previously showed that synthesis of XBP1(S) precedes induction of maximal Ig translation in LPS-stimulated CH12 B cells , indicating that the IRE1/XBP1 pathway is activated at an earlier stage of the differentiation process. What then is the signal(s) for UPR activation in stimulated B cells? This remains a fundamental question, and its answer is integral to understanding the mechanisms that drive development of antibody-secreting B cells.
6. Phosphatidylcholine Synthesis and UPR Signaling
Mammals express three CCT isoforms that are similar in enzymatic activity and regulation. CCTα is encoded by the Pcyt1a gene whereas CCTβ2 and CCTβ3 are encoded by alternatively spliced transcripts from the Pcyt1b gene . CCTα is predominantly expressed in most tissues, including B cells , and is required for early embryonic development . Tissue-specific deletion of the Pcyt1a gene using the Cre-loxP system has revealed critical roles for CCTα in specialized secretory cells, including surfactant lipid production and secretion by alveolar epithelial cells , assembly and secretion of lipoproteins by hepatocytes , and cytokine secretion by activated macrophages . We recently showed that selective deletion of CCTα significantly hampers the ability of B cells to upregulate PtdCho synthesis upon stimulation, and interestingly, this correlates with heightened induction of the IRE1/XBP1 branch of the UPR .
When challenged with a T cell-dependent protein antigen, the animals harboring CCTα-deficient B cells were unable to produce normal levels of IgG but secreted hyperlevels of IgM . The correlation between the reduced PtdCho synthesis and elevated IgM secretion in the CCTα-deficient B cells was counterintuitive, however, based on the implied need for membrane PtdCho expansion during plasma cell differentiation. Investigation of the UPR components revealed that the impaired production of PtdCho triggers IRE-mediated splicing of Xbp1 mRNA early after activation, thereby promoting differentiation of IgM-secreting cells. The inability of CCTα-deficient B cells to undergo isotype switching correlates with a proliferation defect. However, blocking proliferation by a different mechanism did not elicit XBP1(S) activation, supporting the idea that the early and potent induction of XBP1(S) by PtdCho deficiency in CCTα-deficient B cells accelerates and augments the transition into antibody secretion. From these observations, we propose that the IRE1/XBP1 branch of the UPR responds to increased demand for phospholipids as well as increased demand on the protein folding capacity of the ER (Figure 2). In agreement, restriction of either PtdCho  or fatty acid synthesis  has been shown to elicit activation of UPR components in other systems. It is intriguing to speculate that lipid supply might function as a metabolic cue for induction of the IRE1/XBP1 pathway in activated B cells.
The authors are supported in part by National Institutes of Health (NIH) Grants GM061970 (J. W. Brewer), GM062896 (S. Jackowski), and by ALSAC (S. Jackowski).
- D. Tarlinton, A. Radbruch, F. Hiepe, and T. Dorner, “Plasma cell differentiation and survival,” Current Opinion in Immunology, vol. 20, no. 2, pp. 162–169, 2008.
- L. J. McHeyzer-Williams and M. G. McHeyzer-Williams, “Antigen-specific memory B cell development,” Annual Review of Immunology, vol. 23, pp. 487–513, 2005.
- N. N. Iwakoshi, A. H. Lee, P. Vallabhajosyula, K. L. Otipoby, K. Rajewsky, and L. H. Glimcher, “Plasma cell differentiation and the unfolded protein response intersect at the transcription factor XBP-I,” Nature Immunology, vol. 4, no. 4, pp. 321–329, 2003.
- A. M. Reimold, N. N. Iwakoshi, J. Manis et al., “Plasma cell differentiation requires the transcription factor XBP-1,” Nature, vol. 412, no. 6844, pp. 300–307, 2001.
- S. Jackowski, “Coordination of membrane phospholipid synthesis with the cell cycle,” Journal of Biological Chemistry, vol. 269, no. 5, pp. 3858–3867, 1994.
- D. R. Voelker and E. P. Kennedy, “Cellular and enzymic synthesis of sphingomyelin,” Biochemistry, vol. 21, no. 11, pp. 2753–2759, 1982.
- D. R. Voelker, “Phosphatidylserine functions as the major precursor of phosphatidylethanolamine in cultured BHK 21 cells,” Proceedings of the National Academy of Sciences of the United States of America, vol. 81, no. 9 I, pp. 2669–2673, 1984.
- T. G. Tessner, C. O. Rock, G. B. Kalmar, R. B. Cornell, and S. Jackowski, “Colony-stimulating factor 1 regulates CTP: phosphocholine cytidylytransferase mRNA levels,” Journal of Biological Chemistry, vol. 266, no. 25, pp. 16261–16264, 1991.
- I. C. Northwood, A. H. Y. Tong, B. Crawford, A. E. Drobnies, and R. B. Cornell, “Shuttling of CTP:phosphocholine cytidylyltransferase between the nucleus and endoplasmic reticulum accompanies the wave of phosphatidylcholine synthesis during the G0 → G1 transition,” Journal of Biological Chemistry, vol. 274, no. 37, pp. 26240–26248, 1999.
- M. N. P. Ng, T. E. Kitos, and R. B. Cornell, “Contribution of lipid second messengers to the regulation of phosphatidylcholine synthesis during cell cycle re-entry,” Biochimica et Biophysica Acta, vol. 1686, no. 1-2, pp. 85–99, 2004.
- A. D. Manguikian and S. E. Barbour, “Cell cycle dependence of group VIA calcium-independent phospholipase A2 activity,” Journal of Biological Chemistry, vol. 279, no. 51, pp. 52881–52892, 2004.
- O. Zaccheo, D. Dinsdale, P. A. Meacock, and P. Glynn, “Neuropathy target esterase and its yeast homologue degrade phosphatidylcholine to glycerophosphocholine in living cells,” Journal of Biological Chemistry, vol. 279, no. 23, pp. 24024–24033, 2004.
- K. L. Calame, K. I. Lin, and C. Tunyaplin, “Regulatory mechanisms that determine the development and function of plasma cells,” Annual Review of Immunology, vol. 21, pp. 205–230, 2003.
- E. van Anken and I. Braakman, “Versatility of the endoplasmic reticulum protein folding factory,” Critical Reviews in Biochemistry and Molecular Biology, vol. 40, no. 4, pp. 191–228, 2005.
- J. S. Rush, T. Sweitzer, C. Kent, G. L. Decker, and C. J. Waechter, “Biogenesis of the endoplasmic reticulum in activated B lymphocytes: temporal relationships between the induction of protein N-glycosylation activity and the biosynthesis of membrane protein and phospholipid,” Archives of Biochemistry and Biophysics, vol. 284, no. 1, pp. 63–70, 1991.
- D. L. Wiest, J. K. Burkhardt, S. Hester, M. Hortsch, D. I. Meyer, and Y. Argon, “Membrane biogenesis during B cell differentiation: most endoplasmic reticulum proteins are expressed coordinately,” Journal of Cell Biology, vol. 110, no. 5, pp. 1501–1511, 1990.
- P. Fagone, R. Sriburi, C. Ward-Chapman et al., “Phospholipid biosynthesis program underlying membrane expansion during B-lymphocyte differentiation,” Journal of Biological Chemistry, vol. 282, no. 10, pp. 7591–7605, 2007.
- C. Kent, “Eukaryotic phospholipid biosynthesis,” Annual Review of Biochemistry, vol. 64, pp. 315–343, 1995.
- G. Wu and D. E. Vance, “Choline kinase and its function,” Biochemistry and Cell Biology, vol. 88, no. 4, pp. 559–564, 2010.
- C. Aoyama, H. Liao, and K. Ishidate, “Structure and function of choline kinase isoforms in mammalian cells,” Progress in Lipid Research, vol. 43, no. 3, pp. 266–281, 2004.
- C. Kent, “CTP:phosphocholine cytidylyltransferase,” Biochimica et Biophysica Acta, vol. 1348, no. 1-2, pp. 79–90, 1997.
- G. S. Attard, R. H. Templer, W. S. Smith, A. N. Hunt, and S. Jackowski, “Modulation of CTP:phosphocholine cytidylyltransferase by membrane curvature elastic stress,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 16, pp. 9032–9036, 2000.
- C. J. Walkey, G. B. Kalmar, and R. B. Cornell, “Overexpression of rat liver CTP:phosphocholine cytidylyltransferase accelerates phosphatidylcholine synthesis and degradation,” Journal of Biological Chemistry, vol. 269, no. 8, pp. 5742–5749, 1994.
- I. Baburina and S. Jackowski, “Cellular responses to excess phospholipid,” Journal of Biological Chemistry, vol. 274, no. 14, pp. 9400–9408, 1999.
- A. L. Henneberry, M. M. Wright, and C. R. McMaster, “The major sites of cellular phospholipid synthesis and molecular determinants of fatty acid and lipid head group specificity,” Molecular Biology of the Cell, vol. 13, no. 9, pp. 3148–3161, 2002.
- P. Fagone and S. Jackowski, “Membrane phospholipid synthesis and endoplasmic reticulum function,” Journal of lipid research, vol. 50, pp. S311–S316, 2009.
- A. L. Henneberry, G. Wistow, and C. R. McMaster, “Cloning, genomic organization, and characterization of a human cholinephosphotransferase,” Journal of Biological Chemistry, vol. 275, no. 38, pp. 29808–29815, 2000.
- A. L. Henneberry and C. R. McMaster, “Cloning and expression of a human choline/ethanolaminephosphotransferase: synthesis of phosphatidylcholine and phosphatidylethanolamine,” Biochemical Journal, vol. 339, no. 2, pp. 291–298, 1999.
- M. M. Wright, A. L. Henneberry, T. A. Lagace, N. D. Ridgway, and C. R. McMaster, “Uncoupling farnesol-induced apoptosis from its inhibition of phosphatidylcholine synthesis,” Journal of Biological Chemistry, vol. 276, no. 27, pp. 25254–25261, 2001.
- R. Sriburi, H. Bommiasamy, G. L. Buldak et al., “Coordinate regulation of phospholipid biosynthesis and secretory pathway gene expression in XBP-1(S)-induced endoplasmic reticulum biogenesis,” Journal of Biological Chemistry, vol. 282, no. 10, pp. 7024–7034, 2007.
- P. Fagone, C. Gunter, C. R. Sage, K. E. Gunn, J. W. Brewer, and S. Jackowski, “CTP:phosphocholine cytidylyltransferase α is required for B-cell proliferation and class switch recombination,” Journal of Biological Chemistry, vol. 284, no. 11, pp. 6847–6854, 2009.
- S. Jackowski, J. Wang, and I. Baburina, “Activity of the phosphatidylcholine biosynthetic pathway modulates the distribution of fatty acids into glycerolipids in proliferating cells,” Biochimica et Biophysica Acta, vol. 1483, no. 3, pp. 301–315, 2000.
- D. Ron and P. Walter, “Signal integration in the endoplasmic reticulum unfolded protein response,” Nature Reviews Molecular Cell Biology, vol. 8, no. 7, pp. 519–529, 2007.
- M. Schroder and R. J. Kaufman, “The mammalian unfolded protein response,” Annual Review of Biochemistry, vol. 74, pp. 739–789, 2005.
- H. P. Harding, Y. Zhang, and D. Ron, “Protein translation and folding are coupled by an endoplasmic- reticulum-resident kinase,” Nature, vol. 397, no. 6716, pp. 271–274, 1999.
- Y. Shi, K. M. Vattem, R. Sood et al., “Identification and characterization of pancreatic eukaryotic initiation factor 2 alpha-subunit kinase, PEK, involved in translational control,” Molecular and Cellular Biology, vol. 18, no. 12, pp. 7499–7509, 1998.
- K. Haze, T. Okada, H. Yoshida et al., “Identification of the G13 (cAMP-response-element-binding protein-related protein) gene product related to activating transcription factor 6 as a transcriptional activator of the mammalian unfolded protein response,” Biochemical Journal, vol. 355, no. 1, pp. 19–28, 2001.
- K. Haze, H. Yoshida, H. Yanagi, T. Yura, and K. Mori, “Mammalian transcription factor ATF6 is synthesized as a transmembrane protein and activated by proteolysis in response to endoplasmic reticulum stress,” Molecular Biology of the Cell, vol. 10, no. 11, pp. 3787–3799, 1999.
- W. Tirasophon, A. A. Welihinda, and R. J. Kaufman, “A stress response pathway from the endoplasmic reticulum to the nucleus requires a novel bifunctional protein kinase/endoribonuclease (Ire1p) in mammalian cells,” Genes and Development, vol. 12, no. 12, pp. 1812–1824, 1998.
- X. Z. Wang, H. P. Harding, Y. Zhang, E. M. Jolicoeur, M. Kuroda, and D. Ron, “Cloning of mammalian Ire1 reveals diversity in the ER stress responses,” EMBO Journal, vol. 17, no. 19, pp. 5708–5717, 1998.
- H. P. Harding, Y. Zhang, A. Bertolotti, H. Zeng, and D. Ron, “Perk is essential for translational regulation and cell survival during the unfolded protein response,” Molecular Cell, vol. 5, no. 5, pp. 897–904, 2000.
- D. Scheuner, B. Song, E. McEwen et al., “Translational control is required for the unfolded protein response and in vivo glucose homeostasis,” Molecular Cell, vol. 7, no. 6, pp. 1165–1176, 2001.
- J. N. Gass, H. Y. Jiang, R. C. Wek, and J. W. Brewer, “The unfolded protein response of B-lymphocytes: PERK-independent development of antibody-secreting cells,” Molecular Immunology, vol. 45, no. 4, pp. 1035–1043, 2008.
- K. Zhang, H. N. Wong, B. Song, C. N. Miller, D. Scheuner, and R. J. Kaufman, “The unfolded protein response sensor IRE1alpha is required at 2 distinct steps in B cell lymphopoiesis,” Journal of Clinical Investigation, vol. 115, no. 2, pp. 268–281, 2005.
- J. Shen, X. Chen, L. Hendershot, and R. Prywes, “ER stress regulation of ATF6 localization by dissociation of BiP/GRP78 binding and unmasking of golgi localization signals,” Developmental Cell, vol. 3, no. 1, pp. 99–111, 2002.
- J. Ye, R. B. Rawson, R. Komuro et al., “ER stress induces cleavage of membrane-bound ATF6 by the same proteases that process SREBPs,” Molecular Cell, vol. 6, no. 6, pp. 1355–1364, 2000.
- Y. Adachi, K. Yamamoto, T. Okada, H. Yoshida, A. Harada, and K. Mori, “ATF6 is a transcription factor specializing in the regulation of quality control proteins in the endoplasmic reticulum,” Cell Structure and Function, vol. 33, no. 1, pp. 75–89, 2008.
- J. Wu, D. T. Rutkowski, M. Dubois et al., “ATF6alpha optimizes long-term endoplasmic reticulum function to protect cells from chronic stress,” Developmental Cell, vol. 13, no. 3, pp. 351–364, 2007.
- K. Yamamoto, T. Sato, T. Matsui et al., “Transcriptional induction of mammalian ER quality control proteins is mediated by single or combined action of ATF6 α and XBP1,” Developmental Cell, vol. 13, no. 3, pp. 365–376, 2007.
- H. Bommiasamy, S. H. Back, P. Fagone et al., “ATF6α induces XBP1-independent expansion of the endoplasmic reticulum,” Journal of Cell Science, vol. 122, no. 10, pp. 1626–1636, 2009.
- R. Brunsing, S. A. Omori, F. Weber et al., “B- and T-cell development both involve activity of the unfolded protein response pathway,” Journal of Biological Chemistry, vol. 283, no. 26, pp. 17954–17961, 2008.
- J. N. Gass, N. M. Gifford, and J. W. Brewer, “Activation of an unfolded protein response during differentiation of antibody-secreting B cells,” Journal of Biological Chemistry, vol. 277, no. 50, pp. 49047–49054, 2002.
- M. Calfon, H. Zeng, F. Urano et al., “IRE1 couples endoplasmic reticulum load to secretory capacity by processing the XBP-1 mRNA,” Nature, vol. 415, no. 6867, pp. 92–96, 2002.
- X. Shen, R. E. Ellis, K. Lee et al., “Complementary signaling pathways regulate the unfolded protein response and are required for C. elegans development,” Cell, vol. 107, no. 7, pp. 893–903, 2001.
- H. Yoshida, T. Matsui, A. Yamamoto, T. Okada, and K. Mori, “XBP1 mRNA is induced by ATF6 and spliced by IRE1 in response to ER stress to produce a highly active transcription factor,” Cell, vol. 107, no. 7, pp. 881–891, 2001.
- A. H. Lee, N. N. Iwakoshi, K. C. Anderson, and L. H. Glimcher, “Proteasome inhibitors disrupt the unfolded protein response in myeloma cells,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 17, pp. 9946–9951, 2003.
- A. H. Lee, G. C. Chu, N. N. Iwakoshi, and L. H. Glimcher, “XBP-1 is required for biogenesis of cellular secretory machinery of exocrine glands,” EMBO Journal, vol. 24, no. 24, pp. 4368–4380, 2005.
- A. L. Shaffer, M. Shapiro-Shelef, N. N. Iwakoshi et al., “XBP1, downstream of Blimp-1, expands the secretory apparatus and other organelles, and increases protein synthesis in plasma cell differentiation,” Immunity, vol. 21, no. 1, pp. 81–93, 2004.
- A. M. Reimold, A. Etkin, I. Clauss et al., “An essential role in liver development for transcription factor XBP-1,” Genes and Development, vol. 14, no. 2, pp. 152–157, 2000.
- C. C. A. Hu, S. K. Dougan, A. M. McGehee, J. C. Love, and H. L. Ploegh, “XBP-1 regulates signal transduction, transcription factors and bone marrow colonization in B cells,” EMBO Journal, vol. 28, no. 11, pp. 1624–1636, 2009.
- D. J. Todd, L. J. McHeyzer-Williams, C. Kowal et al., “XBP1 governs late events in plasma cell differentiation and is not required for antigen-specific memory B cell development,” The Journal of Experimental Medicine, vol. 206, no. 10, pp. 2151–2159, 2009.
- A. M. McGehee, S. K. Dougan, E. J. Klemm et al., “XBP-1-deficient plasmablasts show normal protein folding but altered glycosylation and lipid synthesis,” Journal of Immunology, vol. 183, no. 6, pp. 3690–3699, 2009.
- K. Huitema, J. van den Dikkenberg, J. F. H. M. Brouwers, and J. C. M. Holthuis, “Identification of a family of animal sphingomyelin synthases,” EMBO Journal, vol. 23, no. 1, pp. 33–44, 2004.
- J. E. Vance and D. E. Vance, “Phospholipid biosynthesis in mammalian cells,” Biochemistry and Cell Biology, vol. 82, no. 1, pp. 113–128, 2004.
- M. Goldfinger, E. L. Laviad, R. Hadar et al., “De novo ceramide synthesis is required for n-linked glycosylation in plasma cells,” Journal of Immunology, vol. 182, no. 11, pp. 7038–7047, 2009.
- A. Lykidis, I. Baburina, and S. Jackowski, “Distribution of CTP:phosphocholine cytidylyltransferase (CCT) isoforms. Identification of a new CCTβ splice variant,” Journal of Biological Chemistry, vol. 274, no. 38, pp. 26992–27001, 1999.
- L. Wang, S. Magdaleno, I. Tabas, and S. Jackowski, “Early embryonic lethality in mice with targeted deletion of the CTP:phosphocholine cytidylyltransferase α gene (Pcyt1a),” Molecular and Cellular Biology, vol. 25, no. 8, pp. 3357–3363, 2005.
- Y. Tian, R. Zhou, J. E. Rehg, and S. Jackowski, “Role of phosphocholine cytidylyltransferase α in lung development,” Molecular and Cellular Biology, vol. 27, no. 3, pp. 975–982, 2007.
- R. L. Jacobs, C. Devlin, I. Tabas, and D. E. Vance, “Targeted deletion of hepatic CTP:phosphocholine cytidylyltransferase α in mice decreases plasma high density and very low density lipoproteins,” Journal of Biological Chemistry, vol. 279, no. 45, pp. 47402–47410, 2004.
- Y. Tian, C. Pate, A. Andreolotti et al., “Cytokine secretion requires phosphatidylcholine synthesis,” Journal of Cell Biology, vol. 181, no. 6, pp. 945–957, 2008.
- M. H. M. Van Der Sanden, M. Houweling, L. M. G. van Golde, and A. B. Vaandrager, “Inhibition of phosphatidylcholine synthesis induces expression of the endoplasmic reticulum stress and apoptosis-related protein CCAAT/enhancer-binding protein-homologous protein (CHOP/GADD153),” Biochemical Journal, vol. 369, no. 3, pp. 643–650, 2003.
- J. L. Little, F. B. Wheeler, D. R. Fels, C. Koumenis, and S. J. Kridel, “Inhibition of fatty acid synthase induces endoplasmic reticulum stress in tumor cells,” Cancer Research, vol. 67, no. 3, pp. 1262–1269, 2007.
Copyright © 2012 Joseph W. Brewer and Suzanne Jackowski. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.