Open Access

Gene expression profile of HIV-1 Tat expressing cells: a close interplay between proliferative and differentiation signals

  • Cynthia de la Fuente2,
  • Francisco Santiago2,
  • Longwen Deng2,
  • Carolyne Eadie2,
  • Irene Zilberman2,
  • Kylene Kehn2,
  • Anil Maddukuri2,
  • Shanese Baylor2,
  • Kaili Wu2,
  • Chee Gun Lee1,
  • Anne Pumfery2 and
  • Fatah Kashanchi2Email author
BMC Biochemistry20023:14

https://doi.org/10.1186/1471-2091-3-14

Received: 29 January 2002

Accepted: 10 June 2002

Published: 10 June 2002

Abstract

Background

Expression profiling holds great promise for rapid host genome functional analysis. It is plausible that host expression profiling in an infection could serve as a universal phenotype in virally infected cells. Here, we describe the effect of one of the most critical viral activators, Tat, in HIV-1 infected and Tat expressing cells. We utilized microarray analysis from uninfected, latently HIV-1 infected cells, as well as cells that express Tat, to decipher some of the cellular changes associated with this viral activator.

Results

Utilizing uninfected, HIV-1 latently infected cells, and Tat expressing cells, we observed that most of the cellular host genes in Tat expressing cells were down-regulated. The down-regulation in Tat expressing cells is most apparent on cellular receptors that have intrinsic receptor tyrosine kinase (RTK) activity and signal transduction members that mediate RTK function, including Ras-Raf-MEK pathway. Co-activators of transcription, such as p300/CBP and SRC-1, which mediate gene expression related to hormone receptor genes, were also found to be down-regulated. Down-regulation of receptors may allow latent HIV-1 infected cells to either hide from the immune system or avoid extracellular differentiation signals. Some of the genes that were up-regulated included co-receptors for HIV-1 entry, translation machinery, and cell cycle regulatory proteins.

Conclusions

We have demonstrated, through a microarray approach, that HIV-1 Tat is able to regulate many cellular genes that are involved in cell signaling, translation and ultimately control the host proliferative and differentiation signals.

Background

Whole-genome expression profiling exemplified by the development of DNA microarrays represents a major advance in genome-wide functional analysis [1, 2]. In a single assay, the transcriptional response of each gene to a change in cellular state can be measured, whether it is a viral infection, host cell cycle changes, chemical treatment, or genetic perturbation. Specifically, systematic approaches for identifying the biological functions of cellular genes altered during these changes, such as HIV-1 infection, are needed to ensure rapid progress in defining significant host and viral genome sequences in directed experimentation and applications. Therefore, host cellular states can be inferred from the expression profiles, and the notion that the global transcriptional response constitutes a detailed molecular phenotype, such as class discovery, class prediction, drug target validation, and the classification of tumors by expression profiling has begun to receive considerable attention [311].

Since its discovery, much of the mainstream human immunodeficiency virus type 1 (HIV-1) Tat research has focused on its ability to activate the HIV-1 LTR. However, to date, besides the transactivation activity on the HIV-1 promoter, few other effects exerted by HIV-1 Tat on cellular and viral genes has also been observed. The Tat protein has been shown to transcriptionally repress host cellular genes and be involved in the immunosuppression associated with viral infection. For instance, HIV-1 infection is able to down-regulate major histocompatibility complex type I (MHC-I) by various different viral proteins, including Tat which represses the transcription of MHC-I, Vpu which retains nascent MHC-I chains in the endoplasmic reticulum, and Nef which can mediate selective internalization of MHC-I molecules from the plasma membrane. MHC class I gene expression has also been shown to be reduced upon infection with the wild-type LAI virus or a Tat exon one recombinant virus [12, 13].

Tat has been shown to down-regulate mannose receptor, EDF-1, CD3-gamma, and TCR/CD3 surface receptor [14]. Tat reduces mannose receptor levels and promoter activity in mature macrophages and dendritic cells by interfering with the host transcriptional machinery; resulting in decreased levels of surface mannose receptor needed for Ag (mannosylated albumin uptake) or pathogen capture (Pneumocystis carinii phagocytosis), and eventual delivery to MHC class II-containing intracellular compartments [15]. EDF-1, a gene down-regulated when endothelial cells are induced to differentiate in vitro, was shown to be down-regulated by Tat at the transcriptional level, resulting in the inhibition of endothelial cell growth and in the transition from a nonpolar cobblestone phenotype to a polar fibroblast-like phenotype [16].

When examining the in vivo effects of HIV-1 Tat protein in the Xenopus embryo, it was found that upon injection of synthetic Tat mRNA into zygotes, a marked delay in gastrulation occurred. This led to the altered specification of the anterior-posterior axis and partial loss of the anterior embryo structures. Mechanistically, HIV-1 Tat elicited a general suppression of gene expression, including that of Xbra and gsc, two early genes whose expression are required for proper gastrulation [17].

In relation to the cell cycle, Tat has also been shown to bind to p53 and inhibit the transcription of p53 responsive elements, such as the p21/Waf1 gene promoter. Consequently, upon introduction of stress signals (e.g., gamma irradiation), HIV-1-infected cells lose their G1/S checkpoint, enter the S-phase inappropriately, and apoptose [1820]. Finally, the inhibition of Tat on translational machinery has also been noted. The potential translational inhibitory effects of the TAR RNA region is mediated by the activation of p68 (the interferon-induced 68-kilodalton protein kinase) kinase, which was down-regulated by Tat during productive HIV-1 infection [22].

Although the mechanism of the host cellular down-regulation remains largely unknown, few reports have attempted to decipher the mechanism of the observed inhibition. For instance, the addition of Tat to PC12 cells up-regulated the expression of the inducible cAMP early repressor (ICER), a specific member of the cAMP-responsive element modulator transcription factor family, in a cAMP-dependent manner. In turn, ICER overexpression abrogated the transcriptional activity of the TH promoter, strongly suggesting ICER's involvement in Tat-mediated inhibition of gene expression [23].

Aside from induction of ICER, Tat is capable of forming complex (es) with a component of TFIID, TAFII250 [24] and Tip60 [25] both of which contain histone acetyltransferase (HAT) activity. In these cases, Tat-TAFII250 and Tat-Tip60 do not affect the transcription from the HIV-1 LTR, but interfere with the transcription activity of cellular genes. It is postulated that different targets of HATs by Tat have different consequences. The interaction of Tat with p300/CBP and P/CAF stimulates its ability to transactivate LTR-dependent transcription, while Tat-TAFII250 or Tat-Tip60 interactions control the transcription of cellular genes.

Here to better understand the host response to Tat, we have performed microarray experiments on HIV-1 infected cells expressing the Tat protein. To our surprise many host cellular genes were down-regulated when comparing HIV-1 infected latent cells to uninfected parental cells. Because most, if not all, latent infected cells available to date (e.g., ACH2, U1, J1.1, OM.10) have various expression levels of doubly spliced viral mRNAs, including Tat, Rev, Nef, Vpr, and other accessory proteins, we decided to perform the microarray in a system where Tat was constitutively expressed; asking whether Tat by itself, or in the absence of other accessory proteins, could still down-regulate host cellular genes. Consistent with latently infected cells, we found many cellular genes to be down-regulated in Tat expressing lymphocytes. The down-regulation is most apparent on cellular receptors that have intrinsic receptor tyrosine kinase (RTK) activity and signal transduction members that mediate RTK function; including the Ras-Raf-MEK pathway, and co-activators such as p300/CBP and SRC-1, which mediate gene expression related to hormone receptor genes. Interestingly, we also observed up-regulation of S-phase genes, as well as ribosomal genes involved in translation. Functionally, down-regulation of receptors may allow latent HIV-1 infected cells to either hide from the immune system or avoid extracellular differentiation signals normally regulated by receptors. Up-regulation of S-phase and translation genes may allow speeding of cells through the S-phase and subsequent accumulation at the G2 phase, where most of the cellular and viral translation may take place. Therefore, the presence of Tat may not only control activated transcription on HIV-1 LTR, but also aid in the subsequent translation of viral mRNA in the cytoplasm.

Results and discussion

Host expression profiling in a sufficiently large and diverse set of profiles could allow additional hypotheses to be drawn regarding the function of genes based on the regulatory characteristics of their own transcripts [9, 11]. Here, we describe the effect of one of the most critical viral activators, Tat, involved in HIV-1 infection and pathogenesis. The rationale for these experiments came from the fact that many AIDS-infected patients who are either at stage III (non-progressors) or under highly active antiretroviral therapy (HAART) treatment show some level of doubly spliced viral messages in their infected cells. One of these messages, Tat, has been well studied and characterized, both from a viral activator standpoint, its effect on few host cellular genes, and its effect as an extracellular cytokine. However, to date there are no reported Tat gene expression analyses that detect more than a few cellular genes.

We performed our microarray analysis first with a cDNA blot of 588 genes, which is known to contain various receptors, cytokines, transcription factors, DNA replication genes, and other additional well characterized genes. Figure 1A shows the results of a microarray experiment from uninfected (CEM) and latently HIV-1 infected (ACH2) cells. By definition, latently HIV-1 infected cells contain integrated HIV-1 sequences in the host genome. To our surprise, we detected many cellular genes that were down-regulated in ACH2 cells as compared to CEM uninfected cells. ACH2 cells, similar to many other latent HIV-1 infected cells including U1, OM10.1, 8E5, and J1-1, express multiple doubly spliced messages including Tat, Rev, Nef, and Vpr [20]. Therefore, it would be difficult to determine which one of these viral open reading frames was in fact controlling the observed changes in host gene expression.
Figure 1

Gene expression analysis of uninfected and HIV-1 infected cells. A) Both CEM (uninfected) and ACH2 (latently HIV-1 infected) cells were grown to mid-log phase of growth and processed for RNA isolation. Total RNA was labeled with 32P-ATP and hybridized to human cDNA filters (Clontech, 588 genes). Blots were hybridized overnight, washed the next day, and exposed to a PhosphorImager cassette. B) Same as in panel A, except all the 588 genes were plotted as fold change vs. gene index (individual genes). Examples of three genes such as prothymosin-α, C-myc, and p21/Waf1, is shown on the diagram. C) Northern blot analysis of prothymosin-α, C-myc, p21/Waf1 and ubiquitin using 10 μg of total RNA, separated on 0.8% formaldehyde gel, and probed with 40 mer anti-sense oligos against respective genes. Bottom of panel C, last insert shows RNA ethidium bromide stain from CEM and ACH2 cells.

Nonetheless, when mapping all the 588 genes, we found that 139 genes were activated above 1 fold and 449 genes were expressed below 1 fold (Figure 1B). This is in sharp contrast to latent HTLV-1 infected Tax expressing cells, where more than two-thirds of the same set of genes were activated and scored above one [26]. Some of the genes from HIV-1 latent cells were further processed as control experiments using Northern blot analysis. As can be seen in Figure 1C, and consistent with previously published reports, p21/Waf1 [1921] was down-regulated and C-myc and pro-thymosin-α were up-regulated in HIV-1 latent cells. Collectively, these experiments point toward host cellular changes in the presence of doubly spliced HIV-1 RNA; however they do not explain whether Tat or other viral genes are responsible for the observed cellular changes.

Therefore, we focused our attention on HIV-1 Tat protein, since Tat could readily be detected in immunoprecipitations from 35S labeled latent ACH2, U1, OM10.1, 8E5, and J1-1 cells (20, data not shown). We utilized a well-characterized system of H9 and H9/Tat cell lines for our next set of microarray experiments and increased our repertoire of the known cDNA genes from 588 to 2400. This was accomplished by using glass slides which were printed with cDNAs of 500 bases or higher, and could be used in hybridization with two different sets of RNAs labeled with either Tyramide linked Cy-3 or Cy-5.

Results of such an experiment is shown in Figure 2, where H9 cytoplasmic Poly A+ selected RNA was labeled with Cy-5 and the H9/Tat RNA with Cy-3 prior to hybridization. When all the 2400 genes were plotted, some 695 genes were shown to be up-regulated above one fold and 1705 genes were down-regulated below one fold (right hand graphs). This was consistent with the results obtained from the ACH2 microarray experiment, where more than 2/3 of the cellular genes were down-regulated by one or more of the doubly spliced genes. We then arbitrarily chose a cut-off of three fold change for our next set of analyses. This was mainly because many of our in house microarray experiments with HIV-1, HTLV-1, and HHV-8 infection has shown a reproducible correlation between protein and mRNA levels when gene expression levels were up- or down-regulated by more than three fold (data not shown). A collection of all the genes above and below three fold are shown in Tables 1, 2, and 3. Based on existing literature, we categorized all of these genes into known pathways. For instance, genes in Table 1 belong to receptors, co-receptors, and co-activators, genes in Table 2 are all the translation related factors, and those in Table 3 indicate genes that are involved in cytoskeleton, signal transduction, cell cycle, DNA repair, transcription, and chromatin remodeling processes. All genes have a number ratio of Cy3 to Cy5 (C3/C5) indicating a ratio of mRNA from H9/Tat over H9 cells. A brief name description and gene ID accession number is given to the right hand side of each ratio. All genes are divided into up (3 fold and higher) and down (3 fold and lower) regulated in Tat expressing cells. Below is a brief description of genes that we, along with the existing literature, were able to correlate with proliferative and/or differentiation signals.
Figure 2

Gene expression analysis from Tat expressing cells. Both H9 and H9/Tat cells were grown to mid-log phase of growth, processed for RNA preparation, and labeled with Tyramide linked Cy-5 (H9) or Cy-3 (H9/TAT). Labeled RNAs were hybridized simultaneously to a glass slide containing 2400 known cDNA genes (NEN Inc.). All genes were plotted similar to Figure 1 and genes above & below 1 fold change were plotted (on the right hand side) to show activation and suppression of all genes.

Table 1

Receptors

Ratio (C3/C5)

Gene ID

Receptors

 

up

12.46

Beta 2-microglobulin. [Acc# S82300]

9.73

coxsackievirus and adenovirus receptor (CAR) protein. [Acc# Y07593]

8.5

SSR2 mRNA for beta-signal sequence receptor. [Acc# D37991]

6.29

Androgen receptor associated protein 24 (ARA24). [Acc# AF052578]

5.84

Beta 2- mu, beta 2-microglobulin. [Acc# S54761]

5.25

mRNA for neuropeptide Y-like receptor. [Acc# X71635]

4.23

mRNA for GABA-A receptor, gamma 2 subunit. [Acc# X15376]

4.06

67 kda laminin receptor. [Acc# S37431]

down

0.3

mRNA for receptor of retinoic acid. [Acc# X06614]

0.3

mRNA for key subunit of N-methyl-D-aspartate receptor. [Acc# D13515]

0.3

Endothelial cell protein C/APC receptor (EPCR). [Acc# L35545]

0.28

Receptor protein-tyrosine kinase (HEK8). [Acc# L36645]

0.28

Cation-dependent mannose 6-phosphate-specific receptor. [Acc# M16985]

0.28

GM-CSF receptor (GM-CSF receptor). [Acc# M73832]

0.27

Protein tyrosine phosphatase receptor pi (PTPRP). [Acc# U81561]

0.26

N-methyl-D-aspartate receptor 2A subunit precursor. [Acc# U90277]

0.26

Serotonin 1D receptor (5-HT1D~). [Acc# M81590]

0.25

mRNA for steroid receptor coactivator 1e. [Acc# AJ000882]

0.25

Insulin receptor substrate-1. [Acc# S62539]

0.25

mRNA for LDL-receptor related protein. [Acc# X13916]

0.24

Transforming growth factor-beta type III receptor (TGF-beta). [Acc# L07594]

0.24

Glucocorticoid receptor repression factor 1 (GRF-1). [Acc# M73077]

0.24

Leukocyte-associated Ig-like receptor-1 (LAIR-1). [Acc# AF013249]

0.24

Putative EPH-related PTK receptor ligand LERK-8 (Eplg8). [Acc# U66406]

0.23

TRAIL receptor 2. [Acc# AF016266]

0.23

Steroid receptor coactivator-1. [Acc# U90661]

0.22

mRNA for apolipoprotein E receptor 2. [Acc# D50678]

0.22

Leptin receptor splice variant form 12.1. [Acc# U66496]

0.21

vasopressin activated calcium mobilizing receptor-like. [Acc# X81882]

0.21

Insulin receptor. [Acc# M10051]

0.21

docking protein (signal recognition particle receptor). [Acc# X06272]

0.21

mRNA for fibronectin receptor alpha subunit. [Acc# X06256]

0.21

GRB2 (EGFRBP-GRB2) mRNA sequence. [Acc# M96995]

0.21

mRNA for urokinase plasminogen activator receptor. [Acc# X74039]

0.2

Glycine receptor beta subunit (GLRB). [Acc# U33267]

0.19

mRNA for endothelin receptor (ETR). [Acc# D90402]

0.19

mRNA for A1 adenosine receptor. [Acc# X68485]

0.19

mRNA for EHK-1 receptor tyrosine kinase. [Acc# X95425]

0.18

alpha-2-macroglobulin receptor-associated protein. [Acc# M63959]

0.18

Glutamate receptor type 1 (HBGR1). [Acc# M81886]

0.18

Sigma receptor. [Acc# U75283]

0.18

mRNA for type 1 inositol 1,4,5-trisphosphate receptor. [Acc# D26070]

0.18

GABA-benzodiazepine receptor alpha-5-subunit (GABRA5). [Acc# L08485]

0.18

Glutamate receptor flop isoform (GluR3-flop). [Acc# U10302]

0.18

mRNA for insuline-like growth factor II receptor. [Acc# Y00285]

0.17

N-methyl-D-aspartate receptor subunit 2A (hNR2A). [Acc# U09002]

0.17

mRNA for type 3 inositol 1,4,5-trisphosphate receptor. [Acc# D26351]

0.17

Beta-adrenergic receptor kinase 1. [Acc# M80776]

0.17

Receptor tyrosine kinase (DTK). [Acc# U18934]

0.16

mRNA for brain ryanodine receptor. [Acc# AB001025]

0.15

Nicotinic acetylcholine receptor aloha3 subunit precursor. [Acc# U62432]

0.15

mRNA for steroid hormone receptor hERR1. [Acc# X51416]

0.15

mRNA for leukotriene b4 receptor. [Acc# D89078]

0.15

IgG Fc receptor hFcRn. [Acc# U12255]

0.14

Putative endothelin receptor type B-like protein. [Acc# U87460]

0.14

Peroxisome proliferator activated receptor. [Acc# L07592]

0.13

mRNA for a presumptive KDEL receptor. [Acc# X55885]

0.13

GM-CSF receptor. [Acc# M64445]

0.11

Hap mRNA encoding a DNA-binding hormone receptor. [Acc# Y00291]

0.09

mRNA for leukemia inhibitory factor (LIF) receptor. [Acc# X61615]

0.09

mRNA for metabotropic glutamate receptor subtype 5a. [Acc# D28538]

Table 2

Translation Factors

Ratio (C3/C5)

Gene ID

Translation

 

up

10.32

mRNA for ribosomal protein L26. [Acc# X69392]

9.69

mRNA for ribosomal protein L6. [Acc# X69391]

8.83

mRNA for ribosomal protein S12. [Acc# X53505]

8.36

mRNA for ribosomal protein L31. [Acc# X15940]

8.35

Ribosomal protein S13 (RPS13). [Acc# L01124]

7.99

mRNA for ribosomal protein L35a. [Acc# X52966]

7.97

Ribosomal protein L7a (surf 3) large subunit. [Acc# M36072]

7.56

Ribosomal protein S17. [Acc# M13932]

7.51

Translation initiation factor eIF3 p40 subunit. [Acc# U54559]

7.48

Ribosomal protein L5. [Acc# U14966]

7.2

Translation initiation factor eIF3 p66 subunit. [Acc# U54558]

6.91

mRNA for translationally controlled tumor protein. [Acc# X16064]

6.78

Gene for ribosomal protein L38. [Acc# Z26876]

6.62

Ribosomal protein S24 mRNA. [Acc# M31520]

6.53

mRNA for ribosomal protein. [Acc# D23660]

6.47

Ribosomal protein L41. [Acc# AF026844]

6.35

S3 ribosomal protein. [Acc# S42658]

6.29

Elongation factor 1-alpha 1 (PTI-1). [Acc# L41490]

5.99

Ribosomal protein S20 (RPS20). [Acc# L06498]

5.98

Ribosomal protein. [Acc# M15661]

5.97

mRNA for ribosomal protein L39. [Acc# D79205]

5.92

Ribosomal protein L10. [Acc# L25899]

5.8

Ribosomal protein L28. [Acc# U14969]

5.72

mRNA for 26S proteasome subunit p97. [Acc# D78151]

up

5.7

Translation initiation factor 3 47 kDa subunit. [Acc# U94855]

5.53

Ribosomal protein S6. [Acc# M20020]

5.27

Ribosomal protein L27a. [Acc# U14968]

5.27

Ribosomal protein L29 (humrpl29). [Acc# U10248]

5.21

mRNA for eukaryotic initiation factor 4AI. [Acc# D13748]

5.2

mRNA for polyA binding protein. [Acc# Y00345]

5.08

Ribosomal protein S9. [Acc# U14971]

5.06

Ribosomal protein S5. [Acc# U14970]

4.87

mRNA for elongation factor-1-gamma. [Acc# Z11531]

4.82

mRNA for HL23 ribosomal protein homologue. [Acc# X55954]

4.4

mRNA for ribosomal protein S11. [Acc# X06617]

4.34

Acidic ribosomal phosphoprotein P0. [Acc# M17885]

3.94

mRNA for ribosomal protein L8. [Acc# Z28407]

3.92

Ribosomal protein L3-like. [Acc# U65581]

3.72

Acidic ribosomal phosphoprotein P1. [Acc# M17886]

3.44

mRNA for ribosomal protein (similar to yeast S24). [Acc# X62691]

3.1

mRNA for ribosomal protein L7. [Acc# X52967]

down

0.29

Ribosomal protein L34 (RPL34). [Acc# L38941]

0.28

mRNA for ribosomal protein L32. [Acc# X03342]

0.17

mRNA for ribosomal protein L19. [Acc# X63527]

0.16

Translation initiation factor 5 (eIF5). [Acc# U49436]

0.16

mRNA for eIF-2B alpha subunit. [Acc# X95648]

Table 3

Ratio (C3/C5)

Gene ID

Signal Transduction

 

up

8.82

ras-related small GTP binding protein Rab5 (rab5). [Acc# U18420]

down

0.29

MAP kinase-activating death domain protein (MADD). [Acc# U77352]

0.27

MAP kinase kinase kinase (MTK1). [Acc# AF002715]

0.19

p38 gamma MAP kinase. [Acc# U66243]

0.18

ERK3 protein kinase. [Acc# L77964]

0.14

ERK1 mRNA for protein serine/threonine kinase. [Acc# X60188]

0.14

mRNA for TRAF5. [Acc# AB000509]

Thymosin

 

up

5.16

Thymosin beta-10. [Acc# S54005]

5.09

Prothymosin alpha mRNA (ProT-alpha). [Acc# M26708]

4.38

Thymosin beta-10. [Acc# M20259]

4.15

m-RNA for NB Thymosin beta. [Acc# D82345]

4.1

Parathymosin. [Acc# M24398]

3.54

Thymosin beta-4. [Acc# M17733]

2.73

Prothymosin alpha. [Acc# M14630]

Cell Cycle

 

up

9.62

Cyclin protein gene. [Acc# M15796]

8.88

14-3-3 epsilon. [Acc# U54778]

8.04

mRNA for proliferation-associated gene (pag). [Acc# X67951]

7.8

poly(ADP-ribose) polymerase. [Acc# M18112]

7.46

p18 protein. [Acc# J04991]

6.46

hCDC37 homolog, [Acc# U43077]

5.12

hCDC10, CDC10 homolog. [Acc# S72008]

2.39

hCDC2, [Acc# X05360]

down

0.24

mRNA for putative serine/threonine protein kinase. [Acc# Y10032]

0.22

Cam Kinase I. [Acc# L41816]

0.2

Checkpoint suppressor 1 [Acc# U68723]

0.16

PLSTIRE for serine/threonine protein kinase. [Acc# X66365]

0.15

PCTAIRE-2 for serine/threonine protein kinase. [Acc# X66360]

DNA Repair/Replication

 

up

9.62

PCNA [Acc# M15796]

7.8

poly(ADP-ribose) polymerase. [Acc# M18112]

3.85

Lupus p70 (Ku) autoantigen protein. [Acc# J04611]

2.56

Excision repair protein (ERCC1). [Acc# M13194]

3.1

DNA-PKcs [Acc# U34994]

down

0.25

Rad51C (RAD51C). [Acc# AF029669]

0.23

DNA repair protein XRCC9 (XRCC9). [Acc# U70310]

0.21

DNA mismatch repair protein homolog (hMLH1). [Acc# U07343]

0.19

Topoisomerase I. [Acc# J03250]

0.18

RAD51D. [Acc# AF034956]

0.13

DNA replication licensing factor (huMCM2). [Acc# D83987]

Transcription

 

Pol I

 

up

3.19

Transcription factor SL1. [Acc# L39059]

Pol II

 

up

7.17

100 kDa coactivator. [Acc# U22055]

6.42

RNA polymerase II elongation factor-like protein. [Acc# Z47087]

3.34

TFIID subunit TAFII55 (TAFII55). [Acc# U18062]

3.1

mRNA for TBP associated factor, TAFII68. [Acc# X98893]

down

 

0.3

TFIIB related factor hBRF (HBRF). [Acc# U75276]

0.29

mRNA for transcriptional activator hSNF2b. [Acc# D26156]

0.27

mRNA for RNA polymerase II 140 kDa subunit. [Acc# X63563]

0.25

RNA polymerase II. [Acc# L37127]

0.22

p300 protein. [Acc# U01877]

0.16

Rac3 (RAC3). [Acc# AF008591]

0.14

RNA polymerase II elongation factor SIII. [Acc# L34587]

Pol III

 

down

0.13

TFIIIC Box B-binding subunit. [Acc# U02619]

0.12

Transcription factor TFIIIB (hTFIIIB90). [Acc# U28838]

Chromatin Remodeling

 

up

4.93

NAP (nucleosome assembly protein). [Acc# M86667]

4.83

RNA polymerase transcriptional mediator (h-MED6). [Acc# U78082]

4.39

sin3 associated polypeptide p18 (SAP18). [Acc# U96915]

3.81

mRNA for nucleosome assembly protein. [Acc# D50370]

down

0.21

SWI/SNF complex 170 KDa subunit (BAF170). [Acc# U66616]

0.21

Chromatin assembly factor-I p150 subunit. [Acc# U20979]

0.19

SWI/SNF complex 60 KDa subunit (BAF60c). [Acc# U66619]

DNA Binding

 

up

10.17

mRNA for DNA binding protein TAXREB67. [Acc# D90209]

5.76

Pur (pur-alpha). [Acc# M96684]

5.25

Nuclear factor NF45. [Acc# U10323]

5.28

mRNA for transcription factor AREB6. [Acc# D15050]

7.17

Insulin-like growth factor binding protein 2 (IGFBP2). [Acc# M35410]

6.33

Non-histone chromosomal protein HMG-17. [Acc# M12623]

down

0.27

Kruppel related zinc finger protein (HTF10). [Acc# L11672]

0.26

Transcription factor ETR101. [Acc# M62831]

0.21

Helix-loop-helix protein (Id-2). [Acc# M97796]

0.2

Transcription factor IL-4 Stat. [Acc# U16031]

0.2

Activating transcription factor 3 (ATF3). [Acc# L19871]

0.16

ATF family member ATF6 (ATF6). [Acc# AF005887]

0.16

Paired box gene (PAX6) homologue. [Acc# M93650]

0.17

MADS/MEF2-family transcription factor (MEF2C). [Acc# L08895]

Receptor family members

It has long been known that infection by HIV-1 commonly leads to the down-regulation and the disappearance of CD4 receptors from the plasma membrane, a phenomenon referred to as receptor down-modulation. This, in turn, renders cells refractory to subsequent infection by the same or other viruses that use the CD4 receptor for entry; thus creating a state of super-infection immunity. Results in Table 1 indicate that although few receptor genes were up-regulated, most of the cellular receptors in general, were down-regulated in the presence of the Tat protein. Most of these receptors or membranous proteins were initially discovered from immune or neuronal cells, hence they were given names related to the immune or nervous system. For instance, mRNA for the neuropeptide Y-like receptor (Acc# X71635), which was up-regulated in Tat expressing cells, was initially discovered as a G-protein coupled neuropeptide Y receptor, and later found to be homologous to the co-receptor CCR5 needed for HIV-1 infection of monocyte/macrophage cells. Therefore, most of the receptors listed in Table 1 may in fact be expressed in various tissues and have multiple functions.

Consistent with our microarray results on CCR5 up-regulation, experiments performed in peripheral blood mononuclear cells (PBMCs) with soluble Tat has shown selective entry and replication of CCR5 virus into cells [27, 28]. Up-regulation of HIV-1 coreceptor by Tat has also been reported, where a synthetic Tat protein that was immobilized on a solid substrate, up-regulated the surface expression of the chemokine receptors in purified populations of primary resting CD4+ T cells. Also, a similar result was seen from Tat protein actively released by HIV-1 infected cells, implying a potentially important role for extracellular Tat in rendering the bystander CD4+ T cells more susceptible to infection [28].

We therefore tested whether H9/Tat cells, which showed an increase in CCR5 expression, could in fact allow better entry and infection of the CCR5 (R5) virus into cells. Figure 3A shows the result of such an experiment, where H9/Tat cells allowed a better replication profile of the R5 than the CXCR4 (X4) virus. The increase in viral titer peaked after some 18 days of infection with the R5 virus, further implying that the CCR5 co-receptor allowed a better selection of R5 virus in Tat expressing cells.
Figure 3

Functional and physical confirmation of few genes from Tat expressing cells. A) Infection of mono- and T-tropic viruses into Tat expressing cells. Both HXB-2 and BaL strains of HIV-1 were infected into H9 and H9/TAT cells. Supernatants were collected every 3 days and further processed for p24 gag ELISA assays. B) Western blot analysis from H9 and H9/TAT expressing cells using co-activators (SRC-1), DNA damage (DNA-PK), activator (p300), and signal transduction (Ras, RAF, and MAPK) antibodies. TBP stands for TATA binding protein, which served as positive control in western blots. C) Western blot analysis from CEM (uninfected T-cell), ACH2 (infected T-cell), U937 (uninfected promonocytic), U1 (infected promonocytic), and PBMCs treated with purified Tat wild type or K41A mutant (100 ng/ml) proteins. Fifty microgram of whole cells lysates were processed for western blots with anti-DNA-PK, p300, RAF, and TBP antibodies.

Another example of co-receptors with multiple functions is the leukotriene family member B4, which was down-regulated in Tat expressing cells (Acc# D89078, Table 1). The cysteinyl leukotrienes (CysLT), LTC, LTD, and LTE, were first shown to be essential mediators in asthma [29]. However, when the mouse leukotriene B4 receptor (m-BLTR) gene, was cloned it was shown to have significant sequence homology with chemokine receptors (CCR5 and CXCR4), co-receptors for many different HIV-1 clades [30]. Along the same lines, when cells were infected with 10 primary clinical isolates of HIV-1, leukotriene B4 receptor was primarily utilized for efficient entry into cells which were mainly of the syncytium-inducing phenotype [31]. Therefore, up-regulation of neuropeptide Y-like receptor and down-regulation of leukotriene B4 receptor in Tat expressing cells indicates a selective advantage of one class of virus (CCR5) over another (CXCR4).

Other examples of consistency between our microarray results on receptors and the HIV-1 Tat literature, include the down-regulation of gene expression in uPAR (Acc# X74039), IP3 (Acc# D26070, D26351), Glu R flop (Acc# U10302), PPAR (Acc# L07592), alpha-2 macroglobulin receptor protein (Acc# M63959), and receptor tyrosine kinase (Acc# L36645, U66406) genes.

The transmembranous urokinase-type plasminogen activator receptor (uPAR; CD87) focuses the formation of active plasmin at the cell surface, thus enhancing directional extracellular proteolysis. Interestingly, the promoter activity of the CD87 gene was shown to decline after infection [32], implying that post integration of HIV-1 may in fact down-regulate CD87 gene expression. Similarly, inositol 1,4,5-trisphosphate receptors (IP3R) are intracellular calcium release channels involved in diverse signaling pathways and are required for the activation of T lymphocytes [33]. Tat (also implicated as a neurotoxin) has been shown to release calcium from inositol 1,4, 5-trisphosphate (IP3) receptor-regulated stores in neurons and astrocytes causing premature apoptosis [34]. Down-regulation of IP3 may therefore contribute to viral latency and maintenance of an anti-apoptotic state in cells.

HIV-1 infection can cause extensive neuronal loss and clinically, a severe dementia. The cause of the neurotoxicity remains unclear as neurons are not infected, but the disturbance of glutamate-linked calcium entry has been implicated. It has been shown that HIV-infected brain has a decrease of mRNA and protein of the GluR-A flop subtype of alpha-amino-3-hydroxy-5-methyl-4-isoxazole propionic acid (AMPA) glutamate receptor in cerebellar Purkinje cells. The observed disturbance of AMPA receptors may contribute to the neurotoxic process in other vulnerable brain regions and clinically to the development of dementia [35]. Interestingly, in a mouse model AMPA receptors in the cortex, striatum, hippocampus, and cerebellum declined by 29–50% as early as 8 weeks post-retroviral inoculation. Thus, the reduction in AMPA receptor density may contribute to the development of the cognitive abnormalities associated with HIV-1 infection [36].

Finally, patients with AIDS who are receiving therapy with HIV-1 protease inhibitors have been reported to be afflicted with a syndrome characterized by lipodystrophy (fat redistribution favoring the accumulation of abdominal and cervical adipose tissue), hyperlipidemia, and insulin resistance. Potential mechanisms for altered adipocyte function include, direct binding to PPARgamma or inhibition of transcription of PPARgamma promoter [37]. The lipodystrophy syndrome may be a result of the inhibition of 2 proteins involved in lipid metabolism that have significant homology to the catalytic site of HIV proteases; namely cytoplasmic retinoic acid binding protein type 1 and low density lipoprotein-receptor-related protein [38]. An additional mechanism of PPAR down-regulation may be related to Tat expression in latent cells.

Translation associated factors

Viruses have evolved a remarkable variety of strategies to modulate the host cell translation apparatus with the aim of optimizing viral mRNA translation and replication. For instance, viruses including Herpes simplex virus type 1 (HSV-1) have been known to induce severe alterations of the host translational apparatus, including the up-regulation of ribosomal proteins and the progressive association of several nonribosomal proteins, such as VP19C, VP26, and the poly(A)-binding protein 1 (PAB1P) to ribosomes [39]. In the case of HIV-1, approximately one infectious HIV-1 genome in an infected cell could be transcribed and translated into 50,000 to 100,000 physical particles [40]. This poses an immense challenge for the virus to be able to transcribe, splice, transport, and translate its RNA into fully packaged virions in a timely fashion. Therefore, it would be advantageous for the virus to set the stage for each successive step necessary for viral progeny formation. One such event is Tat's ability to control genes that aid in translational machinery. As seen in Table 2, many of the critical components of a functional ribosome, including large subunits L 3, 6, 26, 31, 38, and 41, as well as S 6, 12, 20, and 24, and many of the translation initiation factors are up-regulated by Tat. This would imply that Tat up-regulates many ribosomal genes that may be necessary to produce functional ribosomes needed for viral mRNA translation. Therefore, interfering with translation could provide a new strategy for anti-HIV treatment. Along these lines, when the aminogylcosides (kanamycin, hygromycin B, paromycin and neomycin) due to their ability to inhibit protein synthesis by affecting ribosomal fidelity, or puromycin because of its competing ability with tRNAs for binding on the large ribosomal subunit, or cycloheximide which inhibit the large ribosomal subunit by preventing ribosomal movement along the mRNA, were used in active HIV-1 infection, it was found that both cycloheximide and puromycin produced the greatest decrease in HIV-1 inhibition, presumably by inhibiting the large subunit of the ribosome [41].

Translation of HIV-1 RNAs pose a challenge since they all contain a TAR sequence at their 5' end. The Tat-responsive region (TAR) of HIV-1 exhibits a trans-inhibitory effect on translation by activating the interferon-induced 68-kilodalton protein kinase. Productive infection by HIV-1 has been shown to result in a significant decrease in the amount of cellular p68 kinase. The steady-state amount of p68 kinase was found to be reduced in cells stably expressing Tat. Thus, the potential translational inhibitory effects of the TAR RNA region, mediated by activation of p68 kinase, may be down-regulated by Tat during activation of the latent virus [22]. Along these lines, a Tat peptide antagonist, which bound specifically to TAR RNA and competed with Tat for binding, reduced Tat-dependent translation [42].

Finally, upregulation of translation genes in Tat expressing cells is specially intriguing in light of the recent discovery of internal ribosome entry sites (IRESs) in HIV-1 gag ORF [43]. IRESs are thought to promote initiation of translation by directly binding to ribosomes, in a manner independent of the mRNA cap or of scanning through upstream sequences. Since, the TAR is located at the 5' end of all HIV-1 RNA transcripts and the presence of secondary structure at or near the 5' end of RNAs reduces the accessibility of the 5' cap to eIF4F, it is thought that this feature of HIV-1 mRNAs can inhibit their cap-dependent translation [4446]. Therefore, a possible function of the HIV-1 gag IRES might be to serve as a mechanism to bypass the structural barriers to cap-dependent translation by recruiting ribosomes easily and directly to the gag ORFs. IRES entirely contained within a translated ORF has been shown in the MMLV gag [47], and host mRNA encoding p110PITSLRE and p58PITSLRE[48]. Along these lines, cap-dependent translation may be cell cycle regulated, especially when cells are arrested at the G2 phase of the cell cycle, where the cap-dependent translation of most cellular host cell mRNAs is inhibited [4951].

Modulation of signal transduction pathway

Results in Table 3 indicate that many seemingly different pathways are being regulated by Tat. However, the signal transduction pathway, MAPK, has been shown to control and be upstream of DNA-replication, transcription, and cell cycle pathways [5254]. The mitogen-activated protein kinase (MAPK) pathway, consisting of the MAP kinase kinases (MKKs) 1 and 2, and extracellular signal-regulated kinases (ERKs) 1 and 2, which have been implicated in diverse cellular processes including proliferation, transformation, and cell differentiation [53]. The MAP kinase (MAPK) pathway has emerged as a crucial route between membrane-bound Ras and the nucleus. This MAPK pathway encompasses a cascade of phosphorylation events involving three key kinases, namely Raf, MEK (MAP kinase kinase) and ERK (MAP kinase). The MAPK pathway controls ERKs 1 and 2, c-Jun N-terminal kinase (JNK), and p38. These signaling pathways in turn, activate a variety of transcription factors including NF-kappaB (p50/p65), AP-1 (c-Fos/c-Jun), and CREB phosphorylation, which in turn coordinate the induction of many genes encoding inflammatory mediators.

Cytokine receptors such as IL-3, GM-CSF, and the interferons transmit their regulatory signals primarily by the receptor-associated Jak family of tyrosine kinases, and activate STAT transcription factors. Activated STAT5 proteins are detected in reduced levels in lymphocytes recovered from HIV-infected patients and immunocompromised mice. Both of these types of receptor signaling pathways have recently been shown to interact with serine/threonine kinases such as MAP kinases. A common intermediate pathway initiating from receptors to the nucleus is the Ras/Raf/MEK/ERK (MAPK) cascade, which can result in the phosphorylation and activation of additional downstream kinases and transcription factors such as p90Rsk, CREB, Elk, and Egr-1 [55, 56]. Therefore, it is intriguing that Tat expressing cells show down-regulation of MAPK components (Table 3, Figure 3B and 3C), essential mediators between receptors and nuclear transcription factors. This would imply that latently infected cells that express Tat (doubly spliced RNA) and not the whole virus (all three classes of the RNA), can control signal transduction related to membrane and transcriptional signaling (Figure 6).

Interestingly, Tat, through the RGD motif, which controls integrin-based cell signaling, has been reported to mediate the activity of phosphotyrosine phosphatase(s). This in turn which would lead to a decrease in the levels of phosphotyrosine-containing proteins such as ERK-2/p42MAPK kinases [57]. Cysteine-rich and basic Tat peptides have been shown to inhibit VEGF-induced ERK activation and mitogenesis. These peptides also inhibited proliferation, angiogenesis, and ERK activation induced by basic fibroblast growth factor with similar potency and efficacy [58]. Consistent with this model, it has been shown that treatment of neural cells with culture supernatants from HAART-treated subjects, which presumably contain extracellular Tat, resulted in down-regulation of the JNK, AKT, and ERK kinases [59].

Finally, activation of MAPKs has been shown to activate the singly spliced and unspliced (genomic) latent HIV-1 virus. For instance, the signal transduction pathways that regulate the switch from latent to productive infection have been linked to MAPK. The induction of latent HIV-1 expression has been shown to be inhibited by PD98059 and U0126, specific inhibitors of MAPK activation. The MAPK acts by stimulating AP-1 and a subsequent physical and functional interaction of AP-1 with NF-κB, resulting in a complex that synergistically transactivates the HIV-1 [60]. At the level of infection and entry, the activation of MAPK through the Ras/Raf/MEK (MAPK kinase) signaling pathway enhances the infectivity of HIV-1 virions. Virus infectivity can be enhanced by treatment of cells with MAPK stimulators, such as serum and phorbol myristate acetate, as well as by coexpression of constitutively activated Ras, Raf, or MEK in the absence of extracellular stimulation [61]. Also, following infection, efficient disengagement of the reverse transcription complex from the cell membrane and subsequent nuclear translocation, requires phosphorylation of the reverse transcription complex components by ERK/MAPK; demonstrating a critical regulation of an early step in HIV-1 infection by the host cell MAPK signal transduction pathway [62]. Therefore, Tat down-regulation of the MAPK pathway in latent cells implies that much of the host signal transductions connected to activation are down-regulated, and at the same time, these cells may be refractory to subsequent infection by other viruses.

Thymosin family members, and cell cycle

Prothymosin α (ProTα) belongs to the α-Thymosin family which comprises different polypeptides widely distributed within animal tissues. Although its role has remained controversial, it is involved in the increase of immediate early genes such as c-myc [63], which is upstream of cyclin D synthesis and necessary for cell division [64]. In humans, ProTα is coded by a gene family of six members. One of them contains introns, exons and classic regulatory signals, while the remaining five are intronless genes [59] located on chromosome 2 [66]. There are two mRNA transcripts, which arise in a ratio of 9:1 (shorter/longer form), where only the long transcript is regulated by extracellular signals.

It has been demonstrated that malignant tissues with accelerated cell cycle show higher levels of ProTα expression than normal or surrounding healthy tissues [67]. ProTα was shown as a marker for breast cancer [68], hepatocarcinoma [69], and plasma levels of its derivative Tα1 been proposed as a marker for the prognosis of lung cancer [70]. In ligand blotting assays, ProTα bound only to chromatin pools and nuclear fractions where histone H1 was present [71, 72]. The analysis of the interaction of ProTα with H1-containing chromatin suggests a putative role for ProTα in the fine-tuning of the stoichiometry and/or mode of interaction of H1 with chromatin [73]. Interestingly, HL-60 cells overexpressing ProTα show an enhancement of accessibility of micrococcal nuclease to chromatin, implying relaxed chromatin structure for enhanced cell cycle gene expression [74].

A broad study using several mononuclear and fibroblastic cell lines has shown that ProTα mRNA accumulation is cell cycle phase-dependent. In the U937 monocytic cell line, ProTα mRNA peaked at the end of S/G2 phase and fell towards the entry into the new G1 phase. More prominent mRNA regulation was found in the fibroblastic cell lines CV1 and NIH3T3, with peak mRNA levels at the end of S-phase. In all cases the expression pattern coincided with that of cyclin B and Cdc2/cyclin B activation [75].

It is interesting to note that Cdc2 (Acc# X05360), Cdc10 homolog (Acc# S72008), and Cdc37 (Acc# U43077) were all up-regulated in Tat expressing cells. Cdc2, a catalytic subunit of cyclin-dependent kinases, is required for both the G1-to-S and G2-to-M transitions. In the fission yeast Schizosaccharomyces pombe, the execution of Start requires the activity of the Cdc2 protein kinase and the Cdc10/Sct1 transcription complex. The loss of any of these genes leads to G1 arrest [69].

Cdc37 encodes a 50-kDa protein that targets intrinsically unstable oncoprotein kinases including Cdk4, Raf-1, and v-src to the molecular chaperone Hsp90, an interaction that is thought to be important for the establishment of signaling pathways. Cdc37 expression may not only be required to support proliferation in cells that are developmentally programmed to proliferate, but may also be required in cells that are inappropriately induced to initiate proliferation by oncogenes. For instance, MMTV-Cdc37 transgenic mice develop mammary gland tumors at a rate comparable to that observed previously in MMTV-cyclin D1 mice, indicating that Cdc37 can function as an oncogene in mice and suggests that the establishment of protein kinase pathways mediated by Cdc37-Hsp90 can be a rate-limiting event in transformation [76]. Also, analysis of proteins that co-immunoprecipitated with Cdk6 and Cdk4 has shown complexes containing both Hsp90 and Cdc37 [7779].

Cdc37 also promotes the production of Cak1. Cak1 in yeast is the human homolog of CAK trimeric enzyme containing CDK7, cyclin H, and MAT1. Both human and yeast Caks function as RNA polymerase II CTD kinase, Cdk activating kinase, and DNA damage/repair enzymes. Cdc37, like its higher eukaryotic homologs, promotes the physical integrity of multiple protein kinases, perhaps by virtue of a cotranslational role in protein folding [80]. Finally, Hsp90/Cdc37 has recently been shown in the stabilization/folding of Cdk9 as well as the assembly of an active Cdk9/cyclin T1 complex responsible for P-TEFb-mediated Tat transactivation [81].

Transcription and chromatin remodeling factors

A highly ordered chromatin structure presents a physical obstacle for gene transcription; presumably by limiting the access of transcription factors and RNA polymerase II core machinery to target DNA [82, 83]. In concert with the observation that corepressors are associated with HDAC activities [84, 85], it appears that the transcriptional outcome of nuclear receptors is determined by the balance of histone acetylation and deacetylation activities, and that ligands serve as a switch to recruit HATs with the concomitant dismissal of HDACs. Signal transduction pathways add another layer of regulation to the functions of CBP/p300. In the case of the POU homeodomain factor Pit-1, transcriptional activity is potentiated by MAPK pathways [86]. Therefore, down-regulation of MAPK pathway members in Tat expressing cells, as seen in Table 3, is consistent with decreased phosphorylation of DNA binding factors such as Pit-1, and overall lower DNA binding activity. Here, we describe the effect of coactivator proteins SRC-1 (Acc# AJ000882, U90661, Table 1) and p300 (Acc# U01877, Table 3), and their relation to differentiation genes such as retinoic acid receptor (RAR/PML, Acc#: X06614, Table 1), and Leptin receptor variant (Acc#: U66496, Table 1); all of which are down-regulated in Tat expressing cells (Figure 5).
Figure 4

Synthesis of IL-8 in Tat expressing cells. Hela cells (pCEP4, and eTat) were either unblocked (unt), or blocked with hydroxyurea (Hu) (2 mM) for 14 h, released, washed twice with phosphate-buffered saline (PBS) and subsequent addition of complete medium [103]. Supernatants were collected at 9 hrs after release for ELISA. All remaining suspension cells were treated with 1% serum for 48 hrs prior to addition of Hu. PHA-activated PBMCs were kept in culture for 2 days prior to addition of Tat protein. Approximately 5 × 106 PBMCs were used for treatment with either wild type or K41A Tat mutant (100 ng/ml) proteins. After an initial incubation for one hr with Tat proteins, cells were washed and cultured in complete media for 24 hrs, prior to IL-8 ELISA.

Figure 5

Predictive model for control of gene expression and signal transduction by constitutive Tat expressing cells. Down-regulation of SWI/SNF components such as BAF 170 and 60 along with coactivators CBP/p300 and SRC-1 may down-regulate a subset of cellular genes that depend on chromatin remodeling and/or co-activator function for their gene expression. Such genes depend on the presence of ligand receptors that require either both SRC-1 and p300 or individual co-activator for their activity.

Over the past three decades a great deal of evidence has accumulated in favor of the hypothesis that steroid receptor hormones act via regulation of gene expression. The action is mediated by specific nuclear receptor proteins, which belong to a superfamily of ligand-modulated transcription factors that regulate homeostasis, reproduction, development, and differentiation [87]. This family includes receptors for steroid hormones, thyroid hormones, hormonal forms of vitamin A and D, peroxisomal activators, and ecdysone [88]. Nuclear hormone receptors are ligand-dependent transcription factors that regulate genes critical to such biological processes as development, reproduction, and homeostasis. Interestingly, these receptors can function as molecular switches, alternating between states of transcriptional repression and activation, depending on the absence or presence of a cognate hormone, respectively. In the absence of cognate hormone, several nuclear receptors actively repress transcription of target genes via interactions with the nuclear receptor corepressors SMRT and NCoR. Upon binding of the hormone, these corepressors dissociate from the DNA-bound receptor, which subsequently recruits a nuclear receptor coactivator (NCoA) complex. Prominent among these coactivators is the SRC (steroid receptor coactivator) family, which consists of SRC-1, TIF2/GRIP1, and RAC3/ACTR/pCIP/AIB-1. These cofactors interact with nuclear receptors in a ligand-dependent manner and enhance transcriptional activation via histone acetylation/methylation and recruitment of additional cofactors such as CBP/p300 [89]. CBP/p300 has been implicated in the functions of a large number of regulated transcription factors based primarily on physical interaction and the ability to potentiate transcription when overexpressed [90]. In the case of nuclear receptors, the interaction with CBP/p300 is ligand-dependent and relies on the conserved nuclear receptor functional domain, AF-2 (activation function 2). In vivo studies have supported the conclusion that CBP/p300 are components of the hormonal-regulation of transcription in fibroblasts isolated from a p300-/- mouse; and loss of the p300 gene severely affects retinoic acid (RA)-dependent transcription [91]. In a separate study using hammerhead ribozymes that specifically cleave CBP or p300 mRNA, Kawasaki et al [92] reported that reduced cellular CBP or p300 levels resulted in compromised expression of endogenous RA-inducible genes such as p21/Waf1 and p27 cdk inhibitors. Along this line, Tat expressing cells have lower levels of p21/Waf1 presumably due to inactivation of p53 and a lack of p300/RA- induced gene expression. Consistent with this interpretation, CBP and p300 harbor transcriptional activation of ligand-induced RA or ER function on a chromatinized template [93].

The NcoA family members constitute SRC-1/NcoA-1 [89], TIF2/GRIP1/NcoA-2, [94, 95] and pCIP/ACTR/AIB1 [9698] proteins, which interact with liganded RA receptor (RAR), and CBP/p300. Overexpression of these NCoA factors enhances ligand-induced transactivation of several nuclear receptors [99]. A weak intrinsic HAT activity has been reported in SRC-1/NCoA-1 and pCIP/ACTR/AIB1, suggesting that chromatin remodeling may also be a function of these NCoA factors [99, 100]; although they do not appear to contain regions homologous to the HAT domains of CBP/p300 or p/CAF. Structure-function analysis of the NCoAs have revealed multiple copies of a signature motif, LXXLL, with conserved spacing that is required for interaction with nuclear receptors and CBP/p300 [99, 101]. Intriguingly, different LXXLL motifs are required for PPARγ (Peroxisome Proliferator activated receptor γ, a gene down-regulated in Tat expressing cells; Acc# L07592, Table 1) function in response to different classes of ligands, suggesting distinct configuration of assembled complexes.

Taken together, through the use of microarray technology, we have described one of the first observations about how Tat is able to control various host cellular machineries. Although our data is consistent with most of the cited literature on the effects of Tat in infected host and uninfected bystander cells, we caution that the transcriptional profiling in chronically infected cells such as ACH2 or H9/Tat cells may not necessarily be representative of the pattern of expression observed in most cells infected by other group M, N, or O HIV-1 isolates.

We recently extended our observations by utilizing other HIV-1 infected cells which normally express Tat (U1), and addition of exogenous purified Tat to uninfected PBMCs. Preliminary results using western blots supports the idea that genes which were altered in H9/Tat system also showed a similar level of change in few of the tested genes (Figure 3C). This notion of consistency was further confirmed using the IL-8 activation by Tat. Interleukin-8 (IL-8) belongs to the CXC chemokine family and is secreted by several different cell types, including monocytes, neutrophils, endothelial cells, fibroblasts, and T lymphocytes. IL-8 production (induced by several stimuli, including IL-1, TNF-, and phorbol myristate acetate) is primarily regulated at the transcriptional level. IL-8 is a potent chemotactic factor for granulocytes and T lymphocytes, and is found in HIV-infected individuals. The CXC chemokine IL-8 does not bind to CCR5. It has previously been shown that IL-8 mRNA induction was seen less then 1 h after Tat (72aa) stimulation, and levels remained elevated for up to 24 h, leading to IL-8 protein production [102]. Along these lines, we have previously shown that the IL-8 gene is expressed in a cell cycle-dependent manner in cells that express the Tat protein, and the induction is during the S phase of the cell cycle and regulated by stable NF-kB binding to the IL-8 promoter [103]. When looking for IL-8 at the G1/S border, we found that all Tat containing cells, including PBMCs that were treated with exogenous Tat showed an up-regulation of IL-8 in the supernatant (Figure 4), further implying that results obtained from the H9/Tat system may infact be of general physiological relevance in vivo.
Figure 6

Proposed model for changes in signal transduction. A) Down-regulation of receptor tyrosine kinases (RTK) by Tat which modulates the phosphorylation and transcription of downstream effectors such as Ras, Raf, MEK, MAPK, and control transcription factor phosphorylation. B) Role of Tat in the increase of genes necessary for proliferation, such as Cdc2, Cdc37, and Prothymosin α, and down-regulation of differentiation genes, such as receptors, co-receptors, and signal transduction genes.

Finally, throughout the current study we came across some technical findings that were critical in the confirmation of most of our results. For instance, few genes did not correlate in their activation or suppression levels when comparing fold changes between microarrays and protein levels using western blot analysis. We suspect this is because many genes that are transcribed may not necessarily be translated, due to their cell cycle stage, 5' stem and loop RNA structures, varying half-lives of proteins and mRNAs, and a host of other unknown variables. Also, specific changes that occur in a cell may not be required in redundant pathways that score for a specific function. This is commonly seen in the differences between HIV-1 infected or Tat expressing in vitro cell lines and AIDS patients PBMC samples. Therefore, other microarrays would have to be performed on purified infected PBMCs to confirm most of the changes observed in Tables 1, 2, and 3. Unfortunately, to date this particular issue is not feasibly addressable, since it is not possible to isolate a homogenous population of infected T- or Monocytic cells from AIDS patients. Also, confirmatory tests for protein expression would have to be done with both hydrophilic and hydrophobic extraction buffers. For instance, we have observed that PCNA protein, which is up-regulated in Tat expressing cells, extract best with hydrophobic buffers from the nucleus, presumably due to its binding to DNA replication machinery (data not shown). Future experiments will address issues related to differences between various HIV-1 Tat clades, host expression levels between T- and Monocytic cells, and its effect at various stages of the cell cycle.

Conclusions

Expression profiling from HIV-1 or Tat expressing cells holds great promise for rapid functional analysis. Here, we have described the effect of Tat and its alterations with the host cellular gene expression. We observed that more than 2/3 of the cellular genes tested were down-regulated by Tat. These genes belong to receptor, co-receptor, and co-activator pathways that are part of serine/threonine receptor tyrosine kinase, Ras/Raf/MEK/ERK (MAPK) cascade, which control proliferative and/or differentiation signals. We also observed a great deal of increase in the host cell translation apparatus with the possible aim of optimizing viral mRNA translation prior to viral maturation and release. Therefore, HIV-1 accessory doubly spliced messages such as Tat, may control the host gene expression in latently infected cells, and determine not only viral transcription, but also the fate of post-transcriptional events.

Materials and method

Cell culture

ACH2 cells are HIV-1 infected CD4 lymphocytic cells, with an integrated wild-type single-copy chromatinized DNA. The CEM T cell (12D7) is the parental cell for ACH2 cells. ACH2 cell lines has a single copy of LAI strain proviral sequence. The TAR has a point mutation at (C37 -> T), which no longer responds (efficiently) to Tat. However, the cell line is fully capable of making infectious virus in presence of TNF, PHA, PMA, and a host of other stimuli. H9 and H9/Tat cells are both CD4+ Lymphocytic cells, where H9 cells carry a control integrated vector without the Tat open reading frame, and H9/Tat cells carry integrated Tat expression vector. Both cell lines were a generous gift of George Pavlakis (NCI, NIH). U1 is a monocytic clone harboring two copies of the viral genome from parental U973 cells. All cells were cultured at 37°C up to 105 cells per ml in RPMI-1640 media, containing 10% Fetal Bovine Serum (FBS) treated with a mixture of 1% streptomycin and penicillin antibiotics, and 1% L-glutamine (Gibco/BRL). Phytohemagglutinin-activated PBMC were kept in culture for 2 days prior to addition of Tat protein. Isolation and treatment of PBMC were performed by following the guidelines of the Centers for Disease Control. Approximately 5 × 106 PBMC were used for treatment of wild type and K41A Tat mutant (100 ng/ml) proteins. After an initial incubation for one hr with Tat proteins, cells were washed and cultured in complete media for 24 hrs, prior to western blots. pCEP4, eTat cells were HeLa cells stably transfected with either a backbone control plasmid (pCEP4; Invitrogen) or a plasmid expressing Tat (1–86) with a C-terminal epitope tag (eTat) [103]. HeLa cell lines containing either the control or eTat plasmid were selected by single-cell dilution. Both cell types were selected and maintained under 200 μg of hygromycin per ml. Verification of Tat transcriptional activity was achieved by electroporation of reporter plasmids as previously described [103].

Cell cycle analysis

Hela cells were blocked with hydroxyurea (Hu) (2 mM) for 14 h. Following the block, cells were released by being washed twice with phosphate-buffered saline (PBS) and by the addition of complete medium. All suspension cells were treated with 1% serum for 48 hrs prior to addition of Hu. Supernatants were collected and analyzed by an IL-8 ELISA according to the manufacturer's instructions (Biosource International). For controls, each sample, approximately 1 × 106 cells was processed for cell sorting. Cells were washed with PBS and fixed by addition of 500 μl of 70% ethanol. For fluorescence-activated cell sorting (FACS) analysis, cells were stained with a cocktail of propidium iodide (PI) buffer (PBS with Ca2+ and Mg2+, RNase A [10 μg/ml], NP-40 [0.1%], and PI [50 μg/ml]) followed by cell-sorting analysis. FACS data acquired were analyzed by ModFit LT software (Verity Software House, Inc.).

Cell extract preparation and immunoblotting

All cells were cultured to mid-log phase of growth, washed with PBS without Ca2+ and Mg2+, and lysed in a buffer containing 50 mM Tris-HCl (pH 7.5), 120 mM NaCl, 5 mM EDTA, 50 mM NaF, 0.2 mM Na3VO4, 1 mM DTT, 0.5% NP-40 and protease inhibitors (Protease inhibitor cocktail tablets, Boehringer Mannheim, one tablet per 50 ml). The lysate was incubated on ice for 15 min, and microcentrifuged at 4°C for 10 min. Total cellular protein was separated on 4–20% Tris-glycine gels (Novex, Inc.) and transferred to a polvinylidene difluoride (PVDF) membranes (Immobilon-P transfer membranes; Millipore Corp.) overnight at 0.08 A. Following the transfer, blots were blocked with 5% non-fat dry milk in 50 ml of TNE 50 (100 mM Tris-Cl [pH 8.0], 50 mM NaCl, 1 mM EDTA) plus 0.1% NP-40. Membranes were probed with a 1:200–1:1000 dilution of antibodies at 4°C overnight, followed by three washes with TNE 50 plus 0.1% NP-40. All antibodies used in this study were purchased from Santa Cruz Biotechnology. The next day, blots were incubated with 10 ml of 125I-protein G (Amersham, 50 μl/10 ml solution) in TNE 50 plus 0.1% NP-40 for 2 hrs at 4°C. Finally, blots were washed twice in TNE 50 plus 0.1% NP-40 and placed on a PhosphorImager cassette for further analysis.

Total RNA purification

Cells were grown to mid-log phase of growth (5.0 × 106), pelleted, and washed twice with cold D-PBS without Ca2+/Mg2+. Total RNA was extracted on ice using Trizol Reagent (Life Technologies, Inc.). Purified RNA was then analyzed on a 1% agarose gel for quality and quantity prior to each experiment.

Glass slide microarray

Gene expression analysis was performed using Micromax™: Human cDNA Microarray System I (cat# MPS101, NEN Life Science Products). On a glass microarray slide, 2400 know human genes were arrayed into 4 separate grids (A, B, C, D), containing 600 genes each (gene description and location on microarrays available at NEN website: http://www.nenlifesci.com). All human genes were ~2200 bp cDNAs, and were characterized from 50+ human cDNA libraries (AlphaGene, Inc., Woburn, MA). In addition to the human genes, three plant control genes were spotted on each grid and were utilized to balance the Cyanine-3 (Cy-3) and Cyanine-5 (Cy-5) fluorescence signals.

A total of 8 μg each of H9 (control sample) and H9/Tat (test sample) mRNAs were reverse transcribed into Biotin and Dinitrophenyl (DNP) labeled cDNA, respectively. After cDNA quality and quantities were analyzed, both cDNAs were then pooled and simultaneously hybridized overnight at 65°C onto the glass microarray. The next day, the microarray slide was serially washed in 0.5× SSC (Sodium Citrate-Sodium Chloride) + 0.01% SDS (Sodium Dodecyl Sulfate), 0.06× SSC + 0.01% SDS, and 0.06× SSC. Next, the Tyramide Signal Amplification (TSA™) was then used to amplify the Cy-3 and Cy-5 signals using antibody-enzyme conjugates, α-DNP-Horseradish peroxidase (HRP) and α-Streptavidin-HRP with Tyramide linked Cy-3 and Cy-5. Screening and data analysis was performed by NEN.

cDNA filter hybridization

Gene expression of CEM and ACH2 were performed using Atlas Human cDNA Expression Array (Clontech Laboratories Inc., Palo Alto, CA) according to the manufacturer's directions. One μg of poly A+ RNA each was DNase I treated, purified using a CHROMA SPIN-200 column, and reverse transcribed into 32P-labeled cDNA. The CHROMA SPIN-200 column was used to purify the 32P-labeled cDNA from unincorporated 32P-labeled dNTPs and small (<0.1 kb) cDNA fragments. Each sample was then hybridized to a human cDNA expression array overnight with continuous agitation at 68°C. The next day, the array was washed three times with gentle agitation, first wash with 2× SSC + 1% SDS and the last two washes with 0.1× SSC + 0.5% SDS at 37°C. Array was exposed to a PhosphorImager Cassette and analyzed using ImageQuant software.

Northern blots

Total cellular RNA was extracted using the RNAzol reagent (Gibco/BRL). Total RNA (20 μg) was isolated from various cells and ran on a 1% formaldehyde-agarose gel overnight at 75 V, transferred onto a 0.2 μm nitrocellulose membrane (Millipore Inc.), UV cross-linked, and hybridized overnight at 42°C with 32P-end-labeled 40 mer oligo probes including p21/Waf1, C-myc, Pro-thymosin, Actin, Tat, and Ubiquitin (Loftstrand, Gaithersburg, Md.). Next day, membranes were washed two times for 15 min each, with 10 ml of 0.2% SDS-2XSSC at 37°C, exposed, and counted on PhosphorImager Cassette.

Viral infection and ELISA assay

Both H9 and H9/Tat cells were infected in the presence of 10 ug of polybrene. For PBMC infections, PHA activated PBMCs were kept in culture for 2 days prior to each infection. Isolation and treatment of PBMCs were performed by following guidelines from the CDC (Isolation, culture, and identification of HIV, Procedural Guide, July 1991, Atlanta, GA). Approximately 2 × 10 6 of H9 or H9/Tat cells, and 5 × 10 6 PBMC cells were infected with either an HXB-2 (CXCR4, T-tropic), or BaL (CCR5, Macrophage-tropic) at 5 ng of p24 gag antigen/ HIV-1 strain. Both viral isolates were obtained from the NIH AIDS research and reference reagent program. After 8 hrs of infection, cells were washed and fresh media was added. Samples were collected every 3rd day and stored at -20 C for p24 gag ELISA. Media from HIV-1 infected cells were centrifuged to pellet the cells and supernatants were collected, and diluted to 1:100 to 1:1000 in RPMI 1640 prior to ELISA. The p24 gag antigen level was analyzed by HIVAG™-1 Monoclonal antibody Kit (Abbott Laboratories, Diagnostics Division).

Declarations

Acknowledgments

The authors would like to thank George Pavlakis for H9 and H9/Tat cells. This work was supported by grants from the George Washington University S funds, NIH grants AI44357, AI43894 and 13969 to F.K., and in part by a support from Alexandrine and Alexander Sinsheimer Foundation to CF, KW, and LD.

Authors’ Affiliations

(1)
Department of Biochemistry and Molecular Biology UMDNJ-New Jersey Medical School
(2)
Department of Biochemistry and Molecular Biology George Washington University School of Medicine

References

  1. Schena M, Shalon D, Davis RW, Brown PO: Quantitative monitoring of gene expression patterns with a complementary DNA microarray. Science. 1995, 270: 467-470.PubMedView ArticleGoogle Scholar
  2. Lockhart DJ, Dong H, Byrne MC, Follettie MT, Gallo MV, Chee MS, Mittmann M, Wang C, Kobayashi M, Horton H, Brown EL: Expression monitoring by hybridization to high-density oligonucleotide arrays. Nat Biotechnol. 1996, 14: 1675-1680. 10.1038/nbt1296-1675.PubMedView ArticleGoogle Scholar
  3. Perou CM, Jeffrey SS, van de Rijn M, Rees CA, Eisen MB, Ross DT, Pergamenschikov A, Williams CF, Zhu SX, Lee JC, Lashkari D, Shalon D, Brown PO, Botstein D: Distinctive gene expression patterns in human mammary epithelial cells and breast cancers. Proc Natl Acad Sci U S A. 1999, 96: 9212-9217. 10.1073/pnas.96.16.9212.PubMed CentralPubMedView ArticleGoogle Scholar
  4. Golub TR, Slonim DK, Tamayo P, Huard C, Gaasenbeek M, Mesirov JP, Coller H, Loh ML, Downing JR, Caligiuri MA, Bloomfield CD, Lander ES: Molecular classification of cancer: class discovery and class prediction by gene expression monitoring. Science. 1999, 286: 531-537. 10.1126/science.286.5439.531.PubMedView ArticleGoogle Scholar
  5. Alizadeh AA, Staudt LM: Genomicscale gene expression profiling of normal and malignant immune cells. Curr Opin Immunol. 2000, 12: 219-225. 10.1016/S0952-7915(99)00078-3.PubMedView ArticleGoogle Scholar
  6. DeRisi JL, Iyer VR, Brown PO: Exploring the metabolic and genetic control of gene expression on a genomic scale. Science. 1997, 278: 680-686. 10.1126/science.278.5338.680.PubMedView ArticleGoogle Scholar
  7. Eisen A, Lucchesi JC: Unraveling the role of helicases in transcription. Bioessays. 1998, 20: 634-641. 10.1002/(SICI)1521-1878(199808)20:8<634::AID-BIES6>3.0.CO;2-I.PubMedView ArticleGoogle Scholar
  8. Gray IC, Stewart LM, Phillips SM, Hamilton JA, Gray NE, Watson GJ, Spurr NK, Snary D: Mutation and expression analysis of the putative prostate tumour-suppressor gene PTEN. Br J Cancer. 1998, 78: 1296-1300.PubMed CentralPubMedView ArticleGoogle Scholar
  9. Holstege FC, Jennings EG, Wyrick JJ, Lee TI, Hengartner CJ, Green MR, Golub TR, Lander ES, Young RA: Dissecting the regulatorycircuitry of a eukaryotic genome. Cell. 1998, 95: 717-728. 10.1016/S0092-8674(00)81641-4.PubMedView ArticleGoogle Scholar
  10. Marton MJ, DeRisi JL, Bennett HA, Iyer VR, Meyer MR, Roberts CJ, Stoughton R, Burchard J, Slade D, Dai H, Bassett DE, Hartwell LH, Brown PO, Friend SH: Drug target validation and identification of secondary drug target effects using DNA microarrays. Nat Med. 1998, 4: 1293-1301. 10.1038/3282.PubMedView ArticleGoogle Scholar
  11. Roberts CJ, Nelson B, Marton MJ, Stoughton R, Meyer MR, Bennett HA, He YD, Dai H, Walker WL, Hughes TR, Tyers M, Boone C, Friend SH: Signaling and circuitry of multiple MAPK pathways revealed by a matrix of global gene expression profiles. Science. 2000, 287: 873-880. 10.1126/science.287.5454.873.PubMedView ArticleGoogle Scholar
  12. Kamp W, Berk MB, Visser CJ, Nottet HS: Mechanisms of HIV-1 to escape from the host immune surveillance. Eur J Clin Invest. 2000, 30: 740-746. 10.1046/j.1365-2362.2000.00697.x.PubMedView ArticleGoogle Scholar
  13. Verhoef K, Bauer M, Meyerhans A, Berkhout B: On the role of the second coding exon of the HIV-1 Tat protein in virus replication and MHC class I downregulation. AIDS Res Hum Retroviruses. 1998, 14: 1553-1559.PubMedView ArticleGoogle Scholar
  14. Willard-Gallo KE, Furtado M, Burny A, Wolinsky SM: Down-modulation of TCR/CD3 surface complexes after HIV-1 infection is associated with differential expression of the viral regulatory genes. Eur J Immunol. 2001, 31: 969-979. 10.1002/1521-4141(200104)31:4<969::AID-IMMU969>3.0.CO;2-2.PubMedView ArticleGoogle Scholar
  15. Caldwell RL, Egan BS, Shepherd VL: HIV-1 Tat represses transcription from the mannose receptor promoter. J Immunol. 2000, 165: 7035-7041.PubMedView ArticleGoogle Scholar
  16. Dragoni I, Mariotti M, Consalez GG, Soria MR, Maier JA: EDF-1, a novel gene product down-regulated in human endothelial cell differentiation. J Biol Chem. 1998, 273: 31119-311124. 10.1074/jbc.273.47.31119.PubMedView ArticleGoogle Scholar
  17. Venanzi S, Destree OH, Gigliani F, Battaglia PA: Analysis of HIV-1 Tat effects in Xenopus laevis embryos. J Biomed Sci. 1998, 5: 211-220. 10.1159/000025333.PubMedGoogle Scholar
  18. Duan L, Ozaki I, Oakes JW, Taylor JP, Khalili K, Pomerantz RJ: The tumor suppressor protein p53 strongly alters human immunodeficiency virus type 1 replication. J Virol. 1994, 68: 4302-4313.PubMed CentralPubMedGoogle Scholar
  19. Li J, Wang C, Friedman DJ, Pardee AB: Reciprocal modulations between p53 and Tat of human immunodeficiency virus type 1. Proc Natl Acad Sci U S A. 1995, 92: 5461-5464.PubMed CentralPubMedView ArticleGoogle Scholar
  20. Clark E, Santiago F, Deng L, Chong S, de La Fuente C, Wang L, Fu P, Stein D, Denny T, Lanka V, Mozafari F, Okamoto T, Kashanchi F: Loss of G(1)/S checkpoint in human immunodeficiency virus type 1-infected cells is associated with a lack of cyclin-dependent kinase inhibitor p21/Waf1. J Virol. 2000, 74: 5040-5052. 10.1128/JVI.74.11.5040-5052.2000.PubMed CentralPubMedView ArticleGoogle Scholar
  21. Longo F, Marchetti MA, Castagnoli L, Battaglia PA, Gigliani F: A novel approach to proteinprotein interaction: complex formation between the p53 tumor suppressor and the HIV Tat proteins. Biochem. Biophys. Res. Commun. 1995, 206: 326-334. 10.1006/bbrc.1995.1045.PubMedView ArticleGoogle Scholar
  22. Roy S, Katze MG, Parkin NT, Edery I, Hovanessian AG, Sonenberg N: Control of the interferon-induced 68-kilodalton protein kinase by the HIV-1 tat gene product. Science. 1990, 247: 1216-1219.PubMedView ArticleGoogle Scholar
  23. Zauli G, Secchiero P, Rodella L, Gibellini D, Mirandola P, Mazzoni M, Milani D, Dowd DR, Capitani S, Vitale M: HIV-1 Tat-mediated inhibition of the tyrosine hydroxylase gene expression in dopaminergic neuronal cells. J Biol Chem. 2000, 275: 4159-4165. 10.1074/jbc.275.6.4159.PubMedView ArticleGoogle Scholar
  24. Weissman JD, Brown JA, Howcroft TK, Hwang J, Chawla A, Roche PA, Schiltz L, Nakatani Y, Singer DS: HIV-1 tat binds TAFII250 and represses TAFII250-dependent transcription of major histocompatibility class I genes. Proc Natl Acad Sci U S A. 1998, 95: 11601-11606. 10.1073/pnas.95.20.11601.PubMed CentralPubMedView ArticleGoogle Scholar
  25. Creaven M, Hans F, Mutskov V, Col E, Caron C, Dimitrov S, Khochbin S: Control of the histone-acetyltransferase activity of Tip60 by the HIV-1 transactivator protein, Tat. Biochemistry. 1999, 38: 8826-8830. 10.1021/bi9907274.PubMedView ArticleGoogle Scholar
  26. de La Fuente C, Deng L, Santiago F, Arce L, Wang L, Kashanchi F: Gene expression array of HTLV type 1 infected T cells: Upregulation of transcription factors and cell cycle genes. AIDS Res Hum Retroviruses. 2000, 16: 1695-1700. 10.1089/08892220050193164.PubMedView ArticleGoogle Scholar
  27. Xiao H, Neuveut C, Tiffany HL, Benkirane M, Rich EA, Murphy PM, Jeang KT: Selective CXCR4 antagonism by Tat: implications for in vivo expansion of coreceptor use by HIV-1. Proc Natl Acad Sci U S A. 2000, 97: 11466-11471. 10.1073/pnas.97.21.11466.PubMed CentralPubMedView ArticleGoogle Scholar
  28. Secchiero P, Zella D, Capitani S, Gallo RC, Zauli G: Extracellular HIV-1 tat protein up-regulates the expression of surface CXC-chemokine receptor 4 in resting CD4+ T cells. J Immunol. 1999, 162: 2427-2431.PubMedGoogle Scholar
  29. Bisgaard H: Role of leukotrienes in asthma pathophysiology. Pediatr Pulmonol. 2000, 30: 166-176. 10.1002/1099-0496(200008)30:2<166::AID-PPUL15>3.0.CO;2-L.PubMedView ArticleGoogle Scholar
  30. Martin V, Ronde P, Unett D, Wong A, Hoffman TL, Edinger AL, Doms RW, Funk CD: Leukotriene binding, signaling, and analysis of HIV coreceptor function in mouse and human leukotriene B4 receptor-transfected cells. J Biol Chem. 1999, 274: 8597-8603. 10.1074/jbc.274.13.8597.PubMedView ArticleGoogle Scholar
  31. Owman C, Garzino-Demo A, Cocchi F, Popovic M, Sabirsh A, Gallo RC: The leukotriene B4 receptor functions as a novel type of coreceptor mediating entry of primary HIV-1 isolates into CD4-positive cells. Proc Natl Acad Sci. 1998, 95: 9530-9534. 10.1073/pnas.95.16.9530.PubMed CentralPubMedView ArticleGoogle Scholar
  32. Speth C, Pichler I, Stockl G, Mair M, Dierich MP: Urokinase plasminogen activator receptor (uPAR; CD87) expression on monocytic cells and T cells is modulated by HIV-1 infection. Immunobiology. 1998, 199: 152-162.PubMedView ArticleGoogle Scholar
  33. Harnick DJ, Jayaraman T, Ma Y, Mulieri P, Go LO, Marks AR: The human type 1 inositol 1,4,5-trisphosphate receptor from T lymphocytes. Structure, localization, and tyrosine phosphorylation. J Biol Chem. 1995, 270: 2833-2840. 10.1074/jbc.270.6.2833.PubMedView ArticleGoogle Scholar
  34. Mayne M, Holden CP, Nath A, Geiger JD: Release of calcium from inositol 1,4,5-trisphosphate receptor-regulated stores by HIV-1 Tat regulates TNF-alpha production in human macrophages. J Immunol. 2000, 164: 6538-6542.PubMedView ArticleGoogle Scholar
  35. Everall IP, Hudson L, al-Sarraj S, Honavar M, Lantos P, Kerwin R: Decreased expression of AMPA receptor messenger RNA and protein in AIDS: a model for HIV-associated neurotoxicity. Nat Med. 1995, 1: 1174-1178. 10.1038/nm1195-1174.PubMedView ArticleGoogle Scholar
  36. Kustova Y, Espey MG, Sei Y, Basile AS: Regional decreases [corrected] in AMPA receptor density in mice infected with the LP-BM5 murine leukemia virus. Neuroreport. 1997, 8: 2410-View ArticleGoogle Scholar
  37. Zhang B, MacNaul K, Szalkowski D, Li Z, Berger J, Moller DE: Inhibition of adipocyte differentiation by HIV protease inhibitors. J Clin Endocrinol Metab. 1999, 84: 4274-4277. 10.1210/jc.84.11.4274.PubMedView ArticleGoogle Scholar
  38. Carr A: HIV protease inhibitor-related lipodystrophy syndrome. Clin Infect Dis. 2000, 30: S135-S142. 10.1086/313854.PubMedView ArticleGoogle Scholar
  39. Greco A, Bienvenut W, Sanchez JC, Kindbeiter K, Hochstrasser D, Madjar JJ, Diaz JJ: Identification of ribosomeassociated viral and cellular basic proteins during the course of infection with herpes simplex virus type 1. Proteomics. 2001, 1: 545-549. 10.1002/1615-9861(200104)1:4<545::AID-PROT545>3.0.CO;2-G.PubMedView ArticleGoogle Scholar
  40. Dimitrov DS, Martin MA: HIV results in the frame. CD4+ cell turnover. Nature. 1995, 375: 194-195. 10.1038/375194b0.PubMedView ArticleGoogle Scholar
  41. Choudhury I, Wang J, Stein S, Rabson A, Leibowitz MJ: Translational effects of peptide antagonists of Tat protein of human immunodeficiency virus type 1. J Gen Virol. 1999, 80: 777-782.PubMedView ArticleGoogle Scholar
  42. Irvine JH, horsfield JA, McKinney CZ, Tate WP: A novel strategy to interfere with human immunodeficiency virus type 1 propogation. NZ Med J. 1998, 111: 222-224.Google Scholar
  43. Buck CB, Shen X, Egan MA, Pierson TC, Walker CM, Siliciano RF: The human immunodeficiency virus type 1 gag gene encodes an internal ribosome entry site. J Virol. 2001, 75: 181-191. 10.1128/JVI.75.1.181-191.2001.PubMed CentralPubMedView ArticleGoogle Scholar
  44. Kozak M: Point mutations define a sequence flanking the AUG initiator codon that modulates translation by eukaryotic ribosomes. Cell. 1986, 44: 283-292. 10.1016/0092-8674(86)90762-2.PubMedView ArticleGoogle Scholar
  45. Parkin NT, Cohen EA, Darveau A, Rosen C, Haseltine W, Sonenberg N: Mutational analysis of the 5' non-coding region of human immunodeficiency virus type 1: effects of secondary structure on translation. EMBO J. 1988, 7: 2831-2837.PubMed CentralPubMedGoogle Scholar
  46. SenGupta DN, Berkhout B, Gatignol A, Zhou AM, Silverman RH: Direct evidence for translational regulation by leader RNA and Tat protein of human immunodeficiency virus type 1. Proc. Natl. Acad. Sci. 1990, 87: 7492-7496.PubMed CentralPubMedView ArticleGoogle Scholar
  47. Chen CY, Sarnow P: Initiation of protein synthesis by the eukaryotic translational apparatus on circular RNAs. Science. 1995, 268: 415-417.PubMedView ArticleGoogle Scholar
  48. Cornelis S, Bruynooghe Y, Denecker G, Van Huffel S, Tinton S, Beyaert R: Identification and characterization of a novel cell cycle-regulated internal ribosome entry site. Mol. Cell. 2000, 5: 597-605. 10.1016/S1097-2765(00)80239-7.PubMedView ArticleGoogle Scholar
  49. Bonneau AM, Sonenberg N: Involvement of the 24-kDa cap-binding protein in regulation of protein synthesis in mitosis. J. Biol. Chem. 1987, 262: 11134-11139.PubMedGoogle Scholar
  50. Vagner S, Waysbort A, Marenda M, Gensac MC, Amalric F, Prats AC: Alternative translation initiation of the Moloney murine leukemia virus mRNA controlled by internal ribosome entry involving the p57/PTB splicing factor. J. Biol. Chem. 1995, 270: 20376-20383. 10.1074/jbc.270.35.20376.PubMedView ArticleGoogle Scholar
  51. Cullen BR: HIV-1 auxiliary proteins: making connections in a dying cell. Cell. 1998, 93: 685-692. 10.1016/S0092-8674(00)81431-2.PubMedView ArticleGoogle Scholar
  52. Marshall MS: Ras target proteins in eukaryotic cells. FASEB J. 1995, 9: 1311-1318.PubMedGoogle Scholar
  53. Lewis TS, Shapiro PS, Ahn NG: Signal transduction through MAP kinase cascades. Adv Cancer Res. 1998, 74: 49-139.PubMedView ArticleGoogle Scholar
  54. McCubrey JA, May WS, Duronio V, Mufson A: Serine/threonine phosphorylation in cytokine signal transduction. Leukemia. 2000, 14: 9-21. 10.1038/sj.leu.2401657.PubMedView ArticleGoogle Scholar
  55. Bonni A, Brunet A, West AE, Datta SR, Takasu MA, Greenberg ME: Cell survival promoted by the Ras-MAPK signaling pathway by transcription-dependent and -independent mechanisms. Science. 1999, 286: 1358-1362. 10.1126/science.286.5443.1358.PubMedView ArticleGoogle Scholar
  56. Kwon EM, Raines MA, Blenis J, Sakamoto KM: Granulocyte-macrophage colony-stimulating factor stimulation results in phosphorylation of cAMP response element-binding protein through activation of pp90RSK. Blood. 2000, 95: 2552-2558.PubMedGoogle Scholar
  57. Wu Z, Cavallaro U, Marchisio PC, Soria MR, Maier JA: Fibronectin modulates the effects of HIV-1 Tat on the growth of murine Kaposi's sarcoma-like cells through the down-regulation of tyrosine phosphorylation. Am J Pathol. 1998, 152: 1599-1605.PubMed CentralPubMedGoogle Scholar
  58. Jia H, Lohr M, Jezequel S, Davis D, Shaikh S, Selwood D, Zachary I: Cysteine-rich and basic domain HIV-1 Tat peptides inhibit angiogenesis and induce endothelial cell apoptosis. Biochem Biophys Res Commun. 2001, 283: 469-479. 10.1006/bbrc.2001.4790.PubMedView ArticleGoogle Scholar
  59. Kusdra L, McGuire D, Pulliam L: Changes in monocyte/macrophage neurotoxicity in the era of HAART: implications for HIV-associated dementia. AIDS. 2002, 16: 31-38. 10.1097/00002030-200201040-00005.PubMedView ArticleGoogle Scholar
  60. Yang X, Chen Y, Gabuzda D: ERK MAP kinase links cytokine signals to activation of latent HIV-1 infection by stimulating a cooperative interaction of AP-1 and NF-kappaB. J Biol Chem. 1999, 274: 27981-27988. 10.1074/jbc.274.39.27981.PubMedView ArticleGoogle Scholar
  61. Yang X, Gabuzda D: Regulation of human immunodeficiency virus type 1 infectivity by the ERK mitogen-activated protein kinase signaling pathway. J Virol. 1999, 73: 3460-3466.PubMed CentralPubMedGoogle Scholar
  62. Jacque JM, Mann A, Enslen H, Sharova N, Brichacek B, Davis RJ, Stevenson M: Modulation of HIV-1 infectivity by MAPK, a virion-associated kinase. EMBO J. 1998, 17: 2607-2618. 10.1093/emboj/17.9.2607.PubMed CentralPubMedView ArticleGoogle Scholar
  63. Eckert K, Grunberg E, Immenschuh P, Garbin F, Kreuser ED, Maurer HR: Interleukin-2-activated killer cell activity in colorectal tumor patients: evaluation of in vitro effects by prothymosin alpha1. J Cancer Res Clin Oncol. 1997, 123: 420-428. 10.1007/s004320050081.PubMedGoogle Scholar
  64. Sburlati AR, Manrow RE, Berger SL: Prothymosin alpha antisense oligomers inhibit myeloma cell division. Proc Natl Acad Sci U S A. 1991, 88: 253-257.PubMed CentralPubMedView ArticleGoogle Scholar
  65. Eschenfeldt WH, Manrow RE, Krug MS, Berger SL: Isolation and partial sequencing of the human prothymosin alpha gene family. Evidence against export of the gene products. J Biol Chem. 1989, 264: 7546-7555.PubMedGoogle Scholar
  66. Szabo P, Panneerselvam C, Clinton M, Frangou-Lazaridis M, Weksler D, Whittington E, Macera MJ, Grzeschik KH, Selvakumar A, Horecker BL: Prothymosin alpha gene in humans: organization of its promoter region and localization to chromosome 2. Hum Genet. 1993, 90: 629-634. 10.1007/BF00202480.PubMedView ArticleGoogle Scholar
  67. Tsitsiloni OE, Stiakakis J, Koutselinis A, Gogas J, Markopoulos C, Yialouris P, Bekris S, Panoussopoulos D, Kiortsis V, Voelter W, Haritos AA: Expression of alpha-thymosins in human tissues in normal and abnormal growth. Proc Natl Acad Sci U S A. 1993, 90: 9504-9507.PubMed CentralPubMedView ArticleGoogle Scholar
  68. Dominguez F, Magdalena C, Cancio E, Roson E, Paredes J, Loidi L, Zalvide J, Fraga M, Forteza J, Regueiro BJ: Tissue concentrations of prothymosin alpha: a novel proliferation index of primary breast cancer. Eur J Cancer. 1993, 29: 893-897.View ArticleGoogle Scholar
  69. Wu CG, Habib NA, Mitry RR, Reitsma PH, van Deventer SJ, Chamuleau RA: Overexpression of hepatic prothymosin alpha, a novel marker for human hepatocellular carcinoma. Br J Cancer. 1997, 76: 1199-1204.PubMed CentralPubMedView ArticleGoogle Scholar
  70. Sasaki H, Fujii Y, Masaoka A, Yamakawa Y, Fukai I, Kiriyama M, Saito Y, Matsui H: Elevated plasma thymosin-alpha1 levels in lung cancer patients. Eur J Cardiothorac Surg. 1997, 12: 885-891. 10.1016/S1010-7940(97)00269-8.PubMedView ArticleGoogle Scholar
  71. Vareli K, Tsolas O, Frangou-Lazaridis M: Regulation of prothymosin alpha during the cell cycle. Eur J Biochem. 1996, 238: 799-806. 10.1111/j.1432-1033.1996.0799w.x.PubMedView ArticleGoogle Scholar
  72. Papamarcaki T, Tsolas O: Prothymosin alpha binds to histone H1 in vitro. Papamarcaki T, Tsolas O:. FEBS Lett. 1994, 345: 71-75. 10.1016/0014-5793(94)00439-0.PubMedView ArticleGoogle Scholar
  73. Karetsou Z, Sandaltzopoulos R, Frangou-Lazaridis M, Lai CY, Tsolas O, Becker PB, Papamarcaki T: Prothymosin alpha modulates the interaction of histone H1 with chromatin. Nucleic Acids Res. 1998, 26: 3111-3118. 10.1093/nar/26.13.3111.PubMed CentralPubMedView ArticleGoogle Scholar
  74. Gomez-Marquez J, Rodriguez P: Prothymosin alpha is a chromatin-remodelling protein in mammalian cells. Biochem J. 1998, 333: 1-3.PubMed CentralPubMedView ArticleGoogle Scholar
  75. Caligiuri M, Connolly T, Beach D: Ran1 functions to control the Cdc10/Sct1 complex through Puc1. Mol Biol Cell. 1997, 8: 1117-1128.PubMed CentralPubMedView ArticleGoogle Scholar
  76. Stepanova L, Finegold M, DeMayo F, Schmidt EV, Harper JW: The oncoprotein kinase chaperone CDC37 functions as an oncogene inmice and collaborates with both c-myc and cyclin D1 in transformation of multiple tissues. Mol Cell Biol. 2000, 20: 4462-4473. 10.1128/MCB.20.12.4462-4473.2000.PubMed CentralPubMedView ArticleGoogle Scholar
  77. Mahony D, Parry DA, Lees E: Active cdk6 complexes are predominantly nuclear and represent only a minority of the cdk6 in T cells. Oncogene. 1998, 16: 603-611. 10.1038/sj.onc.1201570.PubMedView ArticleGoogle Scholar
  78. Dai K, Kobayashi R, Beach D: Physical interaction of mammalian CDC37 with CDK4. J Biol Chem. 1996, 271: 22030-22034. 10.1074/jbc.271.26.15451.PubMedView ArticleGoogle Scholar
  79. Moorthamer M, Panchal M, Greenhalf W, Chaudhuri B: The p16(INK4A) protein and flavopiridol restore yeast cell growth inhibited by Cdk4. Biochem Biophys Res Commun. 1998, 250: 791-797. 10.1006/bbrc.1998.9348.PubMedView ArticleGoogle Scholar
  80. Farrell A, Morgan DO: Cdc37 promotes the stability of protein kinases Cdc28 and Cak1. Mol Cell Biol. 2000, 20: 749-754. 10.1128/MCB.20.3.749-754.2000.PubMed CentralPubMedView ArticleGoogle Scholar
  81. O'Keeffe B, Fong Y, Chen D, Zhou S, Zhou Q: Requirement for a kinase-specific chaperone pathway in the production of a Cdk9/cyclin T1 heterodimer responsible for P-TEFb-mediated tat stimulation of HIV-1 transcription. J Biol Chem. 2000, 275: 279-287. 10.1074/jbc.275.1.279.PubMedView ArticleGoogle Scholar
  82. Struhl K: Histone acetylation and transcriptional regulatory mechanisms. Genes Dev. 1998, 12: 599-606.PubMedView ArticleGoogle Scholar
  83. Kadonaga JT: Eukaryotic transcription: an interlaced network of transcription factors and chromatin-modifying machines. Cell. 1998, 92: 307-313. 10.1016/S0092-8674(00)80924-1.PubMedView ArticleGoogle Scholar
  84. Heinzel T, Lavinsky RM, Mullen TM, Soderstrom M, Laherty CD, Torchia J, Yang WM, Brard G, Ngo SD, Davie JR, Seto E, Eisenman RN, Rose DW, Glass CK, Rosenfeld MG: A complex containing N-CoR, mSin3 and histone deacetylase mediates transcriptional repression. Nature. 1997, 387: 43-48. 10.1038/387043a0.PubMedView ArticleGoogle Scholar
  85. Nagy L, Kao HY, Chakravarti D, Lin RJ, Hassig CA, Ayer DE, Schreiber SL, Evans RM: Nuclear receptor repression mediated by a complex containing SMRT, mSin3A, and histone deacetylase. Cell. 1997, 89: 373-380. 10.1016/S0092-8674(00)80218-4.PubMedView ArticleGoogle Scholar
  86. Xu L, Lavinsky RM, Dasen JS, Flynn SE, McInerney EM, Mullen TM, Heinzel T, D Szeto, Korzus E, Kurokawa R, Aggarwal AK, Rose DW, Glass CK, Rosenfeld MG: Signal-specific co-activator domain requirements for Pit-1 activation. Nature. 1998, 395: 301-306. 10.1038/26270.PubMedView ArticleGoogle Scholar
  87. Xu L, Glass CK, Rosenfeld MG: Coactivator and corepressor complexes in nuclear receptor function. Curr Opin Genet Dev. 1999, 9: 140-147. 10.1016/S0959-437X(99)80021-5.PubMedView ArticleGoogle Scholar
  88. Brinkmann AO: Steroid hormone receptors: activators of gene transcription. J Pediatr Endocrinol. 1994, 7: 275-282.PubMedView ArticleGoogle Scholar
  89. Leo C, Chen JD: The SRC family of nuclear receptor coactivators. Gene. 2000, 245: 1-11. 10.1016/S0378-1119(00)00024-X.PubMedView ArticleGoogle Scholar
  90. Shikama N, Lyon J, LaThangue NB: The p300/CBP family: Intergrating signals with transcription factors and chromatin. Trends Cell Biol. 1997, 7: 230-236. 10.1016/S0962-8924(97)01048-9.View ArticleGoogle Scholar
  91. Yao TP, Oh SP, Fuchs M, Zhou ND, Ch'ng LE, Newsome D, Bronson RT, Li E, Livingston DM, Eckner R: Gene dosage-dependent embryonic development and proliferation defects in mice lacking the transcriptional integrator p300. Cell. 1998, 93: 361-372. 10.1016/S0092-8674(00)81165-4.PubMedView ArticleGoogle Scholar
  92. Kawasaki H, Eckner R, Yao TP, Taira K, Chiu R, Livingston DM, Yokoyama KK: Distinct roles of the co-activators p300 and CBP in retinoic-acid-induced F9-cell differentiation. Nature. 1998, 393: 284-289. 10.1038/30538.PubMedView ArticleGoogle Scholar
  93. Kraus WL, Kadonaga JT: p300 and estrogen receptor cooperatively activate transcription via differential enhancement of initiation and reinitiation. Genes Dev. 1998, 12: 331-342.PubMed CentralPubMedView ArticleGoogle Scholar
  94. Hong H, Kohli K, Garabedian MJ, Stallcup MR: GRIP1, a transcriptional coactivator for the AF-2 transactivation domain of steroid, thyroid, retinoid, and vitamin D receptors. Mol Cell Biol. 1997, 17: 2735-2744.PubMed CentralPubMedView ArticleGoogle Scholar
  95. Voegel JJ, Heine MJ, Tini M, Vivat V, Chambon P, Gronemeyer H: The coactivator TIF2 contains three nuclear receptor-binding motifs and mediates transactivation through CBP binding-dependent and -independent pathways. EMBO J. 1998, 17: 507-519. 10.1093/emboj/17.2.507.PubMed CentralPubMedView ArticleGoogle Scholar
  96. Torchia J, Rose DW, Inostroza J, Kamei Y, Westin S, Glass CK, Rosenfeld MG: The transcriptional co-activator p/CIP binds CBP and mediates nuclear-receptor function. Nature. 1997, 387: 677-684. 10.1038/42652.PubMedView ArticleGoogle Scholar
  97. Chen H, Lin RJ, Schiltz RL, Chakravarti D, Nash A, Nagy L, Privalsky ML, Nakatani Y, Evans RM: Nuclear receptor coactivator ACTR is a novel histone acetyltransferase and forms a multimeric activation complex with P/CAF and CBP/p300. Cell. 1997, 90: 569-580. 10.1016/S0092-8674(00)80516-4.PubMedView ArticleGoogle Scholar
  98. Anzick SL, Kononen J, Walker RL, Azorsa DO, Tanner MM, Guan XY, Sauter G, Kallioniemi OP, Trent JM, Meltzer PS: AIB1, a steroid receptor coactivator amplified in breast and ovarian cancer. Science. 1997, 277: 965-968. 10.1126/science.277.5328.965.PubMedView ArticleGoogle Scholar
  99. Spencer TE, Jenster G, Burcin MM, Allis CD, Zhou J, Mizzen CA, McKenna NJ, Onate SA, Tsai SY, Tsai MJ, O'Malley BW: Steroid receptor coactivator-1 is a histone acetyltransferase. Nature. 1997, 389: 194-198. 10.1038/38304.PubMedView ArticleGoogle Scholar
  100. Heery DM, Kalkhoven E, Hoare S, Parker MG: A signature motif in transcriptional co-activators mediates binding to nuclear receptors. Nature. 1997, 387: 733-736. 10.1038/42750.PubMedView ArticleGoogle Scholar
  101. McInerney EM, Rose DW, Flynn SE, Westin S, Mullen TM, Krones A, Inostroza J, Torchia J, Nolte RT, Assa-Munt N, Milburn MV, Glass CK, Rosenfeld MG: Determinants of coactivator LXXLL motif specificity in nuclear receptor transcriptional activation. Genes Dev. 1998, 12: 3357-3368.PubMed CentralPubMedView ArticleGoogle Scholar
  102. Kutsch O, Oh J, Nath A, Benveniste EN: Induction of the chemokines interleukin-8 and IP-10 by human immunodeficiency virus type 1 Tat in astrocytes. J Virol. 2000, 74: 9214-9221. 10.1128/JVI.74.19.9214-9221.2000.PubMed CentralPubMedView ArticleGoogle Scholar
  103. Mahieux R, Lambert PF, Agbottah E, Halanski MA, Deng L, Kashanchi F, Brady JN: Cell cycle regulation of human interleukin-8 gene expression by the human immunodeficiency virus type 1 Tat protein. J Virol. 2001, 75: 1736-1743. 10.1128/JVI.75.4.1736-1743.2001.PubMed CentralPubMedView ArticleGoogle Scholar

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